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Honey as an antimicrobial agent against multi-drug resistant Gram negative bacterial rods By Rahma Ali Saleh Al-Maaini This dissertation is submitted in partial fulfilment of the degree of MPhil in Biomedical Sciences (Microbiology) School of Health Sciences University of Wales Institute Cardiff, UK May 2011 1 Contents Title I Contents II Declaration XI Dedication XII Acknowledgments XIII Poster Presentation XIV Index of Tables XV Index of Figures XIX Abbreviations XXVI Abstract XXX Chapter 1: Introduction 1 1.1 Antimicrobial Resistance: 2 1.2 Extended Spectrum Beta-Lactamases (ESBLs): 3 1.2.1 Classification of ESBL: 4 1.2.1.1 Functional Classification: 4 1.2.1.2 Molecular Classification: 4 1.2.2 Types of ESBL: 5 1.2.2.1 TEM-type ESBLs (class A) 5 1.2.2.2 SHV-type ESBLs (class A) 6 1.2.2.3 CTX-M type ESBLs (class A): 6 1.2.2.4 OXA-type ESBLs (class D) 7 1.2.2. 5 AmpC-type ESBLs (class C) 7 1.2.2.6 Carbapenemases (class A, B, D) 8 2 1.2.3 Emergence of ESBL: 9 1.2.4 Risk factor for ESBL: 9 1.2.5 Treatment of ESBLs: 10 1.3 Acinetobacter: 10 1.3.1 Taxonomy and Historical Features of Acinetobacter: 11 1.3.2 Laboratory Diagnosis: 12 1.3.3 Clinical features of Acinetobacter infections: 12 1.3.4 Pathogenesis of Acinetobacter infection: 14 1.3.4.1 The production of exopolysaccharide: 15 1.3.4.2 Quorum-sensing: 15 1.3.4.3 The property of adhesion to human epithelial cells via 15 the capsule or fimbriae. 1.3.4.4 Surface and mitochondrial porins: 16 1.3.5 Emergence of Resistance: 17 1.3.6 Carbapenem action on Acinetobacter: 18 1.3.7 Mechanisms of Carbapenem Resistance: 18 1.3.8 Acinetobatcer Treatment with Honey: 20 1.4 Alternative Antimicrobial Therapies: 21 1.4.1 Ancient Use of Honey as a Medicine: 22 1.4.2 Honey as a Modern Medicine: 22 1.4.3 Antimicrobial Activity of Honey: 24 1.4.4 Chemical composition of honey: 26 3 1.4.5 Factors Contributing Antibacterial Properties of Honey: 27 1.4.5.1 Osmotic effect: 28 1.4.5.2 Acidity 28 1.4.5.3 Hydrogen peroxide production 29 1.4.5.4 Non-peroxide Components 30 1.4.5.5 Antioxidant activity: 31 1.4.5 Manuka Honey: 34 1.4.6 Omani Honey: 36 1.5 Aims and Objectives: 39 Chapter 2: Materials & Methods: 40 2.1 Characterization of test organisms: 49 2.1.1 Confirmation of the identity of test organisms: 2.1.2 Antibiotics sensitivities: Extended Spectrum Beta- lactamases 49 49 test (ESBLs): 2.1.2.1 Inoculum preparation: 49 2.1.2.2 Disc application: 49 2.1.2.3 Screening test for ESBL: 50 2.1.2.4 Phenotypic confirmatory test for ESBL: 50 2.1.2.5 ESBL/AmpC* confirmation test: 50 2.2 Characterization of honey samples: 51 4 2.2.1 Honey sample collection: 51 2.2.2 Bioassay of antibacterial activity: 51 2.2.2.1 Phenol standards preparation for bioassay: 52 2.2.2.3 Inoculum preparation: 52 2.2.2.4 Plate preparation: 52 2.2.2.5 Sample preparation: 53 2.2.2.6 Samples and standards application: 53 2.2.2.7 Zone measurement: 54 2.2.2.8 Calculation of antibacterial activity of honey: 54 2.2.3 Determination of pH: 55 2.2.4 Sugar and water content: 55 2.2.5 Hydroxymethylfurfural (HMF) concentration: 56 2.2.6 Protein content: 56 2.2.7 Colour: 58 2.2.8 Pollen analysis: 58 2.2.9 Total phenolic content: 59 2.2.9.1 Reagent/standard preparation: 59 2.2.9.2 Assay method: 60 2.2.10 Free radical activity of honey: 61 2.2.10.1 Reagent / Standard Preparations 61 5 2.2.10.2 Assay procedure: 62 2.3 Determination of antibacterial activity of honey samples against test 62 cultures: 2.3.1 Minimum Inhibitory Concentration (MIC) method: 2.3.1.1 Agar incorporation method: 62 62 2.3.1.1.1 Honey selection: 62 2.3.1.1.2 Inoculum preparation: 63 2.3.1.1.3 Plates preparation: 63 2.3.1.1.4 Honey preparation: 63 2.3.1.1.5 Plates reading (MIC determination): 64 2.3.1.2 Broth dilution method: 2.3.1.2.1 Honey selection: 65 2.3.1.2.2 Honey dilution: 65 2.3.2.1.3 Microtitre plate inoculation: 65 2.3.2.1.4 Visual inspection of MIC: 66 2.3.2.1.5 Spectrophotometric determination of MIC: 66 2.3.2 Minimum Bactericidal concentration (MBC) method: 66 2.4 Time Kill Curve Assay: 67 2.4.1 Strain selection: 67 2.4.2 Time-kill curve: 67 6 2.5 Effect of honey on bacterial structure: 68 2.5.1 Scanning Electron Microscopy (SEM): 68 2.5.1.1 Bacterial Selection for SEM 68 2.5.1.2 Preparation of cells in the exponential phase of growth: 69 2.5.1.3 Preparation of cells for scanning electron microscopy: 69 2.5.2 Transmission Electron Microscopy (TEM): 70 2.5.2.1 Bacterial Selection for TEM 70 2.5.2.2 Preparation of cells for transmission electron 71 microscopy: 2.5.2.3 Pallet trimming and sectioning: 71 2.5.2.4 Staining of thin sections 71 2.6 Effect of honey on bacterial proteins: 72 2.6.1 Two Dimensional Gel Electrophoresis: 72 2.6.1.1 Buffers preparation: 73 2.6.1.2 Cell preparation: 74 2.6.1.3 Protein determination of Acinetobacter extracts for each 74 extract: 2.6.1.4 Rehydration and sample application: 76 2.6.1.5 Rehydration in the PROTEAN® IEF Focusing Tray: 76 2.6.1.6 Equilibration and SDS-PAGE: 77 7 2.6.1.7 Staining and gel visualising: 77 2.7 Statistical analysis of the data: 78 Chapter 3: Results 79 3.1 Confirmations of the identity and antibiotics sensitivities of test 80 organisms: 3.2 Characterization of honey samples: 88 3.2.1 Determination of antibacterial activity: 88 3.2.2 Chemical & physical analysis of honey samples 91 3.2.2.1 Pollen analysis 94 3.2.2.2 Antioxidant activity assay: 96 3.3 Determination of antibacterial activity of honey samples against test 97 cultures: 3.3.1 Minimum Inhibitory Concentration (MIC) and Minimum 97 Bactericidal Concentration (MBC) of manuka honey: 3.3.1.1 Agar incorporation method: 97 3.3.1.2 Broth dilution method: 99 3.3.2 Sensitivity of MDR and ESBLs to Omani honey: 3.4 Time Kill Curves 107 115 3.4.1 Inhibition of test organisms by manuka honey monitored by 115 optical density: 3.4.2 Inhibition of test organisms by manuka honey monitored by total 8 119 viable count 3 3.4.2.1 Acinetobacter spp 120 3.4.2.2 E.coli 122 3.4.2.3 Klebsiella 124 3.4.2.4 Citrobacter 126 3.4.2.5 Enterobacter 128 3.4.2.6 Serratia 130 3.5 Effect of honey on bacterial structure: 134 3.5.1 Growth Curves: 134 3.5.2 Scanning Electron Microscopy (SEM): 138 3.5.2.1 SEM of Acinetobacter 138 3.5.2.2 SEM of E.coli 148 3.5.2.3 SEM of Klebsiella 151 3.5.2.4 SEM of Enterobacter 160 3.5.2.5 SEM of Citrobacter 165 3.5.2.6 SEM of Serratia 170 3.5.2 Transmission Electron Microscopy (TEM): 174 3.5.2.1 TEM for Acinetobacter: 174 3.5.2.2. TEM for E.coli: 179 9 3.6 Effect of honey on bacterial proteins: 184 3.6.1 Two Dimensional Gel Electrophoresis: 184 Chapter 4: Discussion 186 4.1 Antibacterial activity of honey samples: 187 4.2. Chemical & physical analysis of honey samples 189 4.3 Effect of honey samples against test cultures: 193 4.4 Inhibition of test organisms by manuka honey using time kill curve assay 201 4.5 Effect of honey on bacterial structure: 202 4.6 Further investigations: 213 Chapter 5: References 215 10 Declaration This work has not previously been accepted in substance for any degree and is not being concurrently submitted in candidature for any degree. Signed ...................................................................... (candidate) Date .......................................................................... STATEMENT 1 This thesis is the result of my own investigations, except where otherwise stated. Where correction services have been used, the extent and nature of the correction is clearly marked in a footnote(s). Other sources are acknowledged by footnotes giving explicit references. A bibliography is appended Signed ..................................................................... (candidate) Date ......................................................................... STATEMENT 2 I hereby give consent for my thesis, if accepted, to be available for photocopying and for inter-library loan, and for the title and summary to be made available to outside organisations. Signed ..................................................................... (candidate) Date ......................................................................... I hereby give consent for my thesis, if accepted, to be available for photocopying and for inter-library loans after expiry of a bar on access approved by UWIC. Signed ..................................................................... (candidate) Date ............................. 11 Dedication This project is lovingly dedicated to my dear parents whose legacy. I will treasure throughout my life. They thought me to strive and do my best in all things that I undertake. They are indeed my inspiration in doing my best in this endeavour. I thank them for bringing me up the best way they could. I fully dedicate this humble accomplishment of mine to them. 12 Acknowledgments I wish to express my special and sincere thanks to my supervisor Prof. Rose Cooper for all her help, supervision, guidance and valuable suggestions during the execution of this project. I owe my deepest gratitude to Mr. John Philips (dean of international office- UWIC) to offer me a research scholarship. I wish also to record my grateful thanks to Mr. Leighton Jenkins for his support and guidance throughout the practical aspects of this dissertation. Special thanks to Dr. Hann (Cardiff University- Cardiff) and Mr. Issa Al-Amri (Sultan Qaboos UniversityOman) for their assistant in using the facility of electron microscopy at their Universities. Great thanks to Dr. Charles Bakheit (Associate Prof. in Statistics- SQU) for his help in statistical analysis. I would like to express my appreciation to my family who support and encourage me to do the best in writing this dissertation. Special thanks to my friends Shafiqa, Suhaila, Kulthom and Rahima. 13 Presented posters Al-Maaini, R. A, Cooper, R. and Burton, N. „Honey as an antimicrobial agent against multi-drug resistant Gram negative bacterial rods‟, poster presented in the Society for Applied Microbiology (SfAM) 2010 Summer Meeting, Brighton, 5-8 July 2010. 14 Index of Tables Title Tables Page Table 1.1 Honey composition 26 Table 1.2 Comparisons between peroxide and non-peroxide honey 33 Table 2.1 Media, Chemicals and Reagents used for general experiment 41 in the project Table 2.2 Chemicals and Reagents used for electron microscopy 42 experiment in the project Table 2.3 Chemicals and Reagents used for 2- dimensional 43 electrophoresis experiment in the project Table 2.4 Equipment used in general experiments in the project 44 Table 2.5 Equipment used in electron microscopy and 2-dimentional 45 electrophoresis experiments in the project 46 Table 2.6 Thirty isolates of MDR Acinetobacter and their resistance pattern Table 2.7a Clinical isolates of E.coli & Klebsiella provided for this 47 study Table 2.7b Clinical isolates of Citrobacter, Enterobacter & Serratia 48 provided for this study Table 2.8 List of honeys used in this project 51 Table 2.9 Preparation of phenol standards 52 Table 2.10 Preparation of gallic acid standard solutions 60 Table 2.11 Preparation of varying concentration of honey solution from 64 40% (w/v) stock honey for MIC method Table 2.12 Preparation of tubes for MICs Table 2.13: Cultures and honey concentrations used in the time-kill curves 15 65 67 Index of Tables (Continued) Title Tables Table 2.14 Reagents and buffers used in 2-D Electrophoresis Table 2.15: Quantity of proteins in Acinetobacter cells with and without Page 73 75 20% honey Table 3.1 a Identification and antibiotics sensitivities of 30 MDR & b: Acinetobacter isolates 8182 Confirmation of identity and antibiotics sensitivity including 83 Table 3.2: ESBL tests for 10 E.coli isolates. Table 3.3: Confirmation of identity and antibiotics sensitivity including 84 ESBL tests for 12 Klebsiella isolates Table 3.4: Confirmation of identity and antibiotics sensitivity including 85 ESBL tests for 12 Citrobacter isolates. Table 3.5: Confirmation of identity and antibiotics sensitivity including 86 ESBL tests for15 Enterobacter isolates. Table 3.6: Confirmation of identity and antibiotics sensitivity including 87 ESBL tests for 8 Serratia isolates. Table 3.7: Antibacterial activity of honey samples 91 Table 3.8: Chemical & physical analysis of different types of Omani 93 honey compared to manuka honey Table 3.9: Represent the identification of flora sources by pollen 94 analysis Table 3.10: Amount of free radical and phenolic content in each honey samples 16 96 Index of Tables (Continued) Title Tables Table 3.11: Susceptibility of Acinetobacter isolates against manuka Page 98 honey Table 3.12: Sensitivity of 30 Acinetobacter isolates treated with manuka 100 honey by broth dilution method Table 3.13: Sensitivity of 10 Klebsiella isolates to manuka honey tested 102 by the broth dilution method Table 3.14: Sensitivity of 8 Serratia and 8 E.coli isolates to manuka 103 honey using a broth dilution method Table 3.15: Susceptibility of 15 Enterobacter isolates to with manuka 105 honey determined by broth dilution method Table 3.16: Susceptibility of 12 Citrobacter isolates to manuka honey Table 3.17: Susceptibility of 30 MDR Acinetobacter isolates against 4 107- Table 3.18: 106 types of Omani honey using broth dilution method 108 Susceptibility of 12 Klebsiella isolates against 4 types of 109 Omani honey using broth dilution method Table 3.19: Susceptibility of 10 E.coli isolates against 4 types of Omani 110 honey using broth dilution method Table 3.20: Susceptibility of 15 Enterobacter isolates against 4 types of 111 Omani honey using broth dilution method Table 3.21: Susceptibility of 12 Citrobacter isolates against 4 types of 112 Omani honey using broth dilution method Table 3.22: Susceptibility of 8 Serratia isolates against 4 types of Omani 113 honey using broth dilution method Table 3.23: Cultures and honey concentrations used in the time-kill curves assay 17 115 Index of Tables (Continued) Tables Title Page Table 3.24: Decimal reduction dose (DRD) for each isolate after 5 h 132 exposure to 2x respective MICs of manuka honey Table 3.25 Comparison of the mean viable cell count between non 133 honey and honey treated cells using paired sample test (Ttest). Table 3.26: Comparison of changes in cell sizes of isolates observed in 173 scanning electron microscopy between untreated and honey treated cells (P value) (Mann-Whitney Test) Table 4.1: The physicochemical analysis of selected honeys tested 190 Table 4.2: Comparison between previous studies and current study on 196197 MIC of different honeys including manuka honey against six bacteria species. Table 4.3: Summary of the growth inhibition, killing rate and ultrastructure changes in EM for six species selected after exposure to 2x MIC (%w/v) of manuka honey: 18 208 Index of Figures Figure Figure 2.1: Title Page Calibration curve for protein determination in honey 58 samples Figure 2.2: Standard curve for total phenolic content in honey samples 60 Figure 2.3: Calibration curve of protein concentration in Acinetobacter 75 with and without 20% manuka honey. Figure 3.1: A typical honey bioassay plate. 88 Figure 3.2: A typical calibration curve of the bioassay 90 Figure 3.3: Image of pollen present in Omani honey samples at 100x 95 magnification. Figure 3.4: The effect of manuka honey on the growth of Acinetobacter 116 Figure 3.5: The effect of manuka honey on the growth of E.coli 116 Figure 3.6: The effect of manuka honey on the growth of Klebsiella 117 Figure 3.7: The effect of honey on the growth of Citrobacter 117 Figure 3.8: The effect of honey on the growth of Enterobacter 118 Figure 3.9: The effect of honey on the growth of Serratia 118 Figure 3.10: The effect of manuka honey on the viability of 121 Acinetobacter. Figure 3.11: The effect of manuka honey on the viability of E.coli 123 Figure 3.12: The effect of manuka honey on the viability of Klebsiella 125 Figure 3.13: The effect of manuka honey on the viability of Citrobacter 127 Figure 3.14: The effect of manuka honey on the viability of Enterobacter 129 19 Index of Figures (Continued) Figure Figure 3.15: Title Page The effect of manuka honey on the viability of Serratia 131 Figure 3.16: Growth curve of Acinetobacter in ISB 135 Figure 3.17: Growth curve of E.coli in ISB 135 Figure 3.18: Growth curve of Klebsiella in ISB 136 Figure 3.19: Growth curve of Enterobacter in ISB 136 Figure 3.20: Growth curve of Citrobacter in ISB 137 Figure 3.21: Growth curve of Serratia in ISB 137 Figure 3.22: SEM micrograph of untreated cells of Acinetobacter after 0 140 minutes at x5,000 magnification Figure 3.23: SEM micrograph of Acinetobacter cells exposed to 20% 140 (w/v) manuka honey of 0 minutes at x5,000 magnification Figure 3. 24: SEM micrograph of untreated cells of Acinetobacter after 141 60 minutes at x5,000 magnification Figure 3.25: SEM micrograph of Acinetobacter cells exposed to 20% 141 (w/v) manuka honey after 60 minutes at x5,000 magnification Figure 3.26: SEM micrograph of untreated cells of Acinetobacter after 142 90 minutes at x5,000 magnification Figure 3.27: SEM micrograph of Acinetobacter cells exposed to 20% 142 (w/v) manuka honey after 90 minutes at x5,000 magnification Figure 3.28: SEM micrographs of untreated cells of Acinetobacter after 150 minutes at x5,000 A & x20,000 B magnification respectively 20 143 Index of Figures (Continued) Figure Title Page Figure 3.29: SEM micrographs of Acinetobacter cells exposed to 20% (w/v) manuka honey after 150 minutes at x5,000A, x10,000B, x20,000C & x25,000D 144 magnification respectively Figure 3.30: SEM micrographs of untreated cells of Acinetobacter after 146 180 minutes at x5,000 A & x10,000 B magnification respectively Figure 3.31: SEM micrographs of Acinetobacter cells exposed to 20% 147 (w/v) manuka honey after 180 minutes at x 5,000 (A) & (B) magnification respectively Figure 3.32: SEM micrograph of untreated cells of E.coli after 30 149 minutes at x5,000 magnification Figure 3.33: SEM micrograph of E.coli cells exposed to 30% (w/v) 149 manuka honey after 30 minutes at x5,000 magnification Figure 3.34 : SEM micrograph of untreated cells of E.coli after 180 150 minutes at x5,000 magnification Figure 3.35 : SEM micrograph of E.coli cells exposed to 30% (w/v) 150 manuka honey after 180 minutes at x5,000 magnification Figure 3.36: SEM micrographs of untreated cells of Klebsiella after 30 152 minutes at x5,000 (A) & 15,000 (B) magnification respectively Figure 3.37: SEM micrographs of untreated cells of Klebsiella after 180 minutes at x5,000 (A) & 15,000 (B) magnification respectively 21 153 Index of Figures (Continued) Figure Figure 3.38 : Title SEM micrographs of Klebsiella cells Page exposed to 30% manuka honey after 30 minutes at x5,000 (A) & 15,000 (B) 154 magnification respectively Figure 3.39: SEM micrographs of Klebsiella cells exposed to 30% 155 (w/v) manuka honey after 180 minutes at x5,000A, x15,000B,C & x20,000D magnification Figure 3.40: SEM micrographs of Klebsiella cells exposed to 40% 157 (w/v) Omani honey after 30 minutes at x5,000 A & x15,000 B magnification respectively Figure 3.41 : SEM micrographs of Klebsiella cells exposed to 40% 158 (w/v) Omani honey after 180 minutes at x5,000 A & x 20,000 B,C & D magnification respectively Figure 3.42: SEM micrographs of untreated cells of Enterobacter after 161 30 minutes at x5,000 A & x15,000 B magnification respectively Figure 3.43: SEM micrographs of Enterobacter cells exposed to 30% 162 (w/v) manuka honey after 30 minutes at x5,000 A & B magnification respectively Figure 3.44: SEM micrographs of untreated Enterobacter cells after 180 163 minutes at x5,000 A & x20,000 B magnification respectively Figure 3.45: SEM micrographs of Enterobacter cells exposed to 30% 164 (w/v) manuka honey after 180 minutes at x5,000 (A & B) magnification respectively Figure 3.46: SEM micrographs of untreated cells of Citrobacter after 30 minutes at x5,000 A & x15,000 B magnification respectively 22 166 Index of Figures (Continued) Figure Title Page Figure 3.47: SEM micrographs of Citrobacter cells exposed to 20% (w/v) manuka honey after 30 minutes at x10,000 A & 167 x15,000 B magnification respectively Figure 3.48: SEM micrographs of untreated Citrobacter cells after 180 168 minutes at x5,000 (A & B) magnification respectively Figure 3.49: SEM micrographs of Citrobacter cells exposed to 20% 169 (w/v) manuka honey after 180 minutes at x5,000 A & x15,000 B magnification respectively Figure 3.50: SEM micrograph of untreated cells of Serratia after 30 171 minutes at x5,000 magnification Figure 3.51: SEM micrograph of Serratia cells exposed to 30% (w/v) 171 manuka honey for 30 minutes at x 5,000 magnification Figure 3.52: SEM micrograph of untreated cells of Serratia after 180 172 minutes at x5,000 magnification Figure 3.53: SEM micrograph of Serratia cells exposed to 30% (w/v) 172 manuka honey after 180 minutes at x5,000 magnification Figure 3.54: Transmission micrographs of untreated cells of 175 Acinetobacter after 1 h incubation with isosensitest borth (ISB) at 16,000x magnification Figure 3.55: Transmission micrographs of Acinetobacter incubated with 176 isosensitest borth (ISB) containing 20% (w/v) manuka honey for 1 h at 16,000x magnification. Figure 3.56: Transmission micrographs of untreated cells of Acinetobacter incubated with isosensitest borth (ISB) after 3 h at 16,000x magnification 23 177 Index of Figures (Continued) Figure Title Figure 3.57: Transmission micrographs of Acinetobacter incubated with isosensitest borth (ISB) containing 20% (w/v) manuka Page 178 honey after 3 h at 16,000x magnification Figure 3.58: Transmission micrographs of untreated cells of E.coli after 180 1 h incubation with isosensitest borth (ISB) at 16,000x magnification Figure 3.59: Transmission micrographs of E.coli incubated with 181 isosensitest borth (ISB) containing 20% (w/v) manuka honey after 1 h at 16,000x magnification Figure 3.60: Transmission micrographs of untreated cells of E.coli after 182 3 h incubation with isosensitest borth (ISB) at 16,000x & 30,000x magnification Figure 3.61: Transmission micrographs of E.coli incubated with 183 isosensitest borth (ISB) containing 20% (w/v) manuka honey after 3 h at 16,000x magnification Figure 3.62: 2-D protein electrophoresis gel of Acinetobacter cells 185 without honey treatment Figure 3.63: 2-D protein electrophoresis gel of Acinetobacter cells 185 exposed to 20% (w/v) manuka honey Figure 4.1: Mean MIC and MBC (%w/v) for 30 Acinetobacter strain 198 against 5 types of Hone Figure 4.2: Mean MIC and MBC (%w/v) for 12 Klebsiella strain 198 against 5 types of honey Figure 4.3: Mean MIC and MBC (%w/v) for 10 E.coli strain against 5 types of honey 24 199 Index of Figures (Continued) Figure Figure 4.4: Title Mean MIC & MBC (%w/v) for 12 Citrobacter strain Page 199 against 5 types of honey Figure 4.5 Mean MIC and MBC (%w/v) for 15 Enterobacter strain 200 against 5 types of honey Figure 4.6: Mean MIC and MBC (%w/v) for 8 Serratia strain against 5 types of honey 25 200 Abbreviations list AHL-N-acylhomoserine-lactone ATCC- American Type Culture Collection APF - Antibacterial phenolic fraction AIF- Apoptosis inducing factor AMP- Ampicillin AK- Amikacin AZT- Aztreonam BDMA- Benzyl dimethylamine BSA- Bovine serum albumin CDC- Centres for Disease Control CAZ- Ceftazidime CE – Cephradin CFU- Colony forming unit CHAPS--[3-cholamidopropyl)dimethylammonio]-1-propanesulfonate CLA- Clavulanic acid CLSI- Clinical and Laboratory Standards Institute CRO- Ceftriaxone CTX- Cefotaxime CPM- Cefepem DDSA- Dodecenyl Succinic Anhydride DDT- DL-Dithiothreitol DPPH- Di(4-tert-octylphenyl)-1-picryl-hydrazyl DRD- Decimal reduction dose 26 ESBL- Extended spectrum beta lactamase ERT- Ertapenem EDTA- Ethylenediaminetetraacetic acid EMB- Eosin Methylene Blue FOX- Cefoxitin GN- Gentamicin HPA- Health Protection Agency HMF- hydroxymetheyl furfural IMP- Imipenem IEF- Iso- electric focusing ISB- Isosensitest broth MALDI-TOF- MS- Matrix-assisted laser desorption ionisation-time-of-flight mass spectroscopy MBC- Minimum bactericidal concentration MDR- Multi-drug resistant MEM- Meropenem MG or MGO- Methyglyoxal MH- Mueller-Hinton MIC- Minimum inhibitory concentration MOPS- Morpholino-Propansulfonsaure acid MRAB-C Imipenem resistant Acinetobacter baumannii- Carbapenemases MRD- Maximum recovery diluent MRSA- Methicillin resistant Staph. aureus MSSA- Methicillin sensitive Staph. aureus 27 MW- Molecular weight NB- Nutrient broth NDM-1- New delhi metalobetalactamases NCTC- National Collection Type Culture NHB- National honey board NPARU- National Pollen And Research Unit OH- Omani honey OMPs- Outer membrane proteins OSO4- Osmium tetroxide OXA- Oxacillinases PBPs- Penicillin binding protein pI- Iso- electric point ROS- Reactive oxygen species RTI- Respiratory tract infection SEM- Scanning electron microscopy SD- Standard deviation SDS- Sodium dodecylsulphate SDS- PAGE – Sodium dodecyl sulphate polyacrylamide gel electrophoresis SHV- Sulphydryl variable SXT- Septrin TEM- Transmission electron microscopy TAZ- Piperacillin-tazobactam TSB- Tryptone Soya Broth TVC- Total viable count 28 TEM- Temoneira UTI- Urinary tract infection UMF- Unique manuka factor VRE- Vancomycin resistant Enterococcus VSE- Vancomycin sensitive Enterococcus V/V- Volume per volume W/V- Weight per volume 29 Abstract Honey has been shown to have therapeutic properties, which include immunomodulatory and antibacterial activity in vitro and anti-inflammatory, antipyretic and wound healing properties in vivo. A complex mix of factors such as acidity, osmolality and hydrogen peroxide content contribute to antibacterial activity. Unusually manuka honey has been shown to contain methylglyoxal which is derived from nectar collected from the blossom of manuka trees and this confers high antibacterial activity. Manuka honey is used in licensed wound dressings in the UK. Its ability to inhibit staphylococci has been reported, but its efficacy with Gram negative bacteria is less well documented. Since these bacteria are difficult to control and commonly infect military wounds and burns, there is a need to investigate their susceptibility to manuka honey. The main aim of this study is to assess the antimicrobial potential of manuka honey against multi-drug resistant (MDR) Gram negative rods with the potential to infect wounds. Eighty five clinical isolates were tested in this study (30 MDR Acinetobacter and 55 extended spectrum beta-lactamases [ESBL] producing members of the Enterobacteriaceae). The minimum inhibitory concentration (MIC) of manuka honey for each isolate was determined by agar incorporation and broth dilution methods, as well as the minimum bactericidal concentration (MBC). The kinetics of inhibition of selected isolates with high MIC values was monitored by total viable counts. Also, ultrastructural changes in cell morphology were studied before and after exposure to manuka honey using scanning (SEM) and transmission electron microscopy (TEM). Electron micrographs were examined for structural changes, such as altered shape, surface abnormalities and evidence of cell division. Eight Omani honeys were assayed for their antibacterial activity using bioassay, MIC and MBC methods. Omani honeys were also analysed for their chemical and physical properties such as pH, protein, water and sugar contents, hydroxymetheylfurfural (HMF), colour and antioxidant properties. Pollen analysis was also used for identifying the flora origin of honey. All Omani honeys were found to possess peroxide activity nonetheless it exhibited a bactericidal mode of activity against all MDR and ESBLs tested. In addition honey analysis revealed unadulterated and natural honey. A study of anti-radical activity and phenolic contents demonstrated that Omani honey could be used to promote a rapid wound healing and aid its antibacterial activity. The proximity of MIC and MBC values indicates that manuka honey had a bactericidal mode of action against these isolates and this was confirmed by the time to kill curves. The SEM and TEM of images of representative isolates after treatment with manuka honey showed some physical membrane damage, septa formation and irregular shape; whereas non honey treated cells (control) did not appear to be obvious damage. In conclusion manuka honey possesses strong antibacterial activity against the antibiotic-resistant wound pathogens tested here and further investigation into cellular target sites is needed. Both manuka and selected Omani honeys have clinical potential to inhibit pathogens that commonly colonise wounds. 30 Chapter 1 Introduction 31 1.1 Antimicrobial Resistance: An antimicrobial agent is a substance that inhibits or kills microbial growth; unfortunately, the introduction of a new antimicrobial agent into clinical practice is usually followed by the rapid emergence of resistance. Resistance in bacteria can be intrinsic, because not all bacterial species are naturally sensitive to all antimicrobials, or it can be acquired, based on genetic mutation or genetic transfer from other organisms (Forbes et al., 2007). The production of drug-inactivating enzymes, alteration of an active target site, acquirement of a target bypass system, decrease cell permeability and an efflux pump in cell membrane are the five mechanisms which admit microorganisms to acquire resistance through a biochemical basis (Sefton 2002). The mechanisms by which β lactam resistance is manifest in bacteria involve enzymatic inactivation, or by altered receptors of penicillin binding proteins (Winn et al., 2006). Resistance to antimicrobial agents is not a new incident. Soon after penicillin has established as an antibiotic in the 1940s, the rate of penicillin resistance had risen to 14%, and is over 90% for Staphylococcus aureus today (Aksoy 2007). In the past, resistant strains were believed to be a problem confined to hospitals, however today resistance has increased in the community (Aksoy 2007). Urinary tract infections (UTI), respiratory tract infections (RTI), and tuberculosis are considered to be problem diseases both in the community and the hospital setting with regard to antimicrobial resistance. Misuse of antibiotics by healthcare professionals, unprofessional doctors, poor drug quality, poor hygienic conditions and inadequate surveillance measures account for the emergence of resistant bacteria. All of these factors contribute to the spread of multidrug resistant (MDR) organisms, 32 such as methicillin resistant Staphylococcus aureus (MRSA), vancomycin resistant Enterococcus species (VRE), Extended spectrum β-lactamase (ESBL) producing Enterobacteriaceae, Pseudomonas aeruginosa, and Acinetobacter baumannii (Madigan et al., 2009). According to the Centre for Disease Control and Prevention (CDC), more than 70% of bacteria that are concidered now as a sources of hospital acquired infections are resistant to at least one of the drugs that are most commonly used to treat them (Aksoy 2007). 1.2 Extended Spectrum Beta-Lactamases (ESBLs): ESBLs are enzymes that inactivate or hydrolyse β-lactam antibiotics by cleaving the C-N bond on the β-lactam ring. Most of these enzymes are plasmid mediated; they hydrolyze penicillins, cephalosporins, and aztreonam and are inhibited by βlactamase inhibitors, such as clavulanate, sulbactam and tazobactam, (Moland et al., 2008). Beta lactamases are commonly circulated in nature and are generally classified according to the main compounds that they inactivate (e.g., as penicillinases or cephalosporinases) (Baron 1996). The enzymes can be produced in either a constitutive or an inducible manner. Infections with ESBLs can vary from urinary tract infections (UTIs) to more complicated deadly sepsis (Bhattacharya 2006). Many β-lactamase resistance genes of Gram negative bacteria are present on the chromosome and some are carried on plasmids which can be transferred to other organisms. A recently discovered transfer mechanism is the transposon which carries genes between the chromosomes and the plasmids (Greenwood et al., 2007) and an increasing number of β-lactamases have been associated with integrons. Today, ESBL producing bacteria have spread worldwide and have emerged as significant 33 community-and hospital acquired pathogens (Murray et al., 2007). European countries recorded higher incidence of ESBL producing Enterobacteriaceae than the USA, especially for Klebsiella strains (Canton et al., 2008). More than 100 European intensive care units (ICUs) were involved in a study on the prevalence of ESBLs in Klebsiella. Sweden demonstrated the lowest prevalence of ESBL with 3%, whereas Portugal obtained the highest value with 34% (Paterson & Bonomo 2005) 1.2.1 Classification of ESBL: There are many different β -lactamases, and they can be differentiated according to their substrate and inhibitor specificities, physical factors (pH, isoelectric point) and immunological differences. These factors makes classification very difficult (Scholar & Pratt 2000), but two schemes are currently used to classify β-lactamases, which are the Bush-Medeiros-Jacopy system (functional classification) and the Ambler system (molecular classification) (Murray et al., 2007). 1.2.1.1 Functional Classification: A classification scheme for β-lactamases based on functional characteristics was categorized on three major groups of enzymes. These enzymes have been defined by the effects of their substrate and inhibitor product: group one cephalosporinases which are inhibited by clavulanic acid; group two penicillinases, cephalosporinases and broad spectrum β-lactamases are inhibited by active site-occupied β-lactamase inhibitors and the group three metallo-β-lactamases which hydrolyze penicillins, cephalosporins, and carbapenems and weakly inhibited by nearly all β-lactamases inhibitors (Bush, Jacopy & Medeiros 1995) 1.2.1.2 Molecular Classification: 34 Beta-lactamases in this classification are depended on the nucleotide and amino acid sequences built in these enzymes under the Ambler system. Four classes have been recognized (A-D), which associate with the functional classification. Classes A, C, and D have serine residues at the active site, similar to penicillin binding proteins (PBPs), whereas class B or metallo-β-lactamases use a metallic ion, preferentially zinc for their action (Amabile-Cuevas 2007; Murray et al., 2007). 1.2.2 Types of ESBL: 1.2.2.1 TEM-type ESBLs (class A) TEM-1 is the most common β-lactamase found in Gram-negative bacteria; it was first deteced from a patient named Temoneira in 1965. At least 90% of ampicillin resistance in Escherichia coli was found to be due to TEM-1 production, which has an iso-electric point (pI) of 5.4 (Amabile-Cuevas 2007). TEM-1 inactivate most penicillins and first generation cephalosporins such as cephalothin, cefaclor and cephaloridine but does not hydrolyse more stable cephalosporins, like cefotaxime, cefuroxime, cefixime, ceftriaxone, cefepime and ceftazidime and the monobactam, aztreonam (Moland et al., 2008). There are two TEM-ESBL families, one derived from TEM-1 and other derived from TEM-2. These enzymes are plasmid-mediated β-lactamases and can be produced by several members of the Enterobacteriaceae. TEM enzymes involve more than 160 different ESBLs. TEM is commonly distributed because it seems to have emerged by point mutations, and it is also easily created in the laboratory (Amabile-Cuevas, 2007). More than 100 derived of TEM β -lactamases have been identified on a world wide basis (Greenwood et al., 2007) 35 1.2.2.2 SHV-type ESBLs (class A) SHV is an abbreviation for sulphydryl variable (Paterson and Bonomo, 2005). The SHV-1 β-lactamase has been most commonly found in Klebsiella pneumoniae isolates and plasmid-mediated ampicillin resistance has accounted for more than 20% of this enzyme in this species. This enzyme can also be produced by Citrobacter diversus, Escherichia coli, and P. aeruginosa. SHV or a related gene is usually incorporated into the bacterial chromosome, but it has also been found in plasmids (Jacopy and Munoz-Price 2005). The majority of SHV family variant ESBLs producers are differentiated by point mutation with the replacement of a serine for glycine at position 238 (Bradford 2001). Recently outbreaks of SHV-producers have been reported in Acinetobacter spp, and P. aeruginosa (Amabile-Cuevas 2007). Currently, there are approximately 100 SHV- variants β-lactamases (Moland et al., 2008). 1.2.2.3 CTX-M type ESBLs (class A): CTX-M ESBLs are not mutated forms of broad spectrum β -lactamases but are derived from chromosomal enzymes found in rare bacteria known as Kluyvera species. The encoding gene of this enzyme is also commonly located on plasmids with different sizes (7-160 kb). At present approximately half of the CTX-M enzymes have been discovered to be plasmid encoded (Amabile-Cuevas 2007). CTX-M was first detected in 1990 and it spread between Enterobacteriaceae such as E.coli, K. pneumoniae, Salmonella, Shigella, Citrobacter freundii, Enterobacter and Serratia marcescens (Murray et al., 2007). More than 90 molecular variants of CTXM have been described (Zong and Yu 2010). It is called CTX (a common abbreviation for cefotaxime) because many CTX-M enzymes are able to hydrolyse 36 cefotaxime faster than ceftazidime; however, a few CTX-Ms significantly hydrolyse ceftazidime (e.g., CTX-M-15, -19, -25 and -32). CTX-M carried on specific bacterial genotypes was related to different geographical regions (Hawkey & Jones 2009). CTX-M-14 and-15 seems to be the most pandemic genotypes in recent times (Hawkey 2008). Moreover, these enzymes were more readily inhibited by tazobactam compared to other β-lactamase inhibitors such as sulbactam and clavulanate (Bradford 2001). This may explain the higher sensitivity of some CTXM producers to piperacillin-tazobactam than to cefepime (Amabile-Cuevas 2007). 1.2.2.4 OXA-type ESBLs (Class D) OXA ESBLs are enzymes that hydrolyse oxacillin and cloxacillin. These ESBLs occur commonly in the Enterobacteriaceae, Acinetobacter and P. aeruginosa. They belong to molecular class D which dishtinguishes them from the TEM and SHV enzymes (Murray et al., 2007). Although resistance to ceftazidime is a phenotypic indicator in the detection of this type of ESBL, their detection can be difficult because of the weak inhibition by clavulanate (Moland et al., 2008). 1.2.2. 5 AmpC-type ESBLs (Class C) AmpC β-lactamases enzyme (also termed class C or group 1) are commonly isolated from Gram-negative bacteria that are resistant to extended-spectrum cephalosporins. This enzyme is usually determined on the chromosome of many Enterobacteriaceae including Citrobacter, Serratia and Enterobacter species and usually has inducible expression; whereas in E. coli it is not usually inducible, even if it is hyper- expressed. Thus, AmpC β-lactamase genes of Gram-negative bacteria have been transferred onto plasmids and have spread worldwide by increasing their number and variety (Hawkey 2008). 37 AmpC β-lactamases, compared to ESBLs are able to hydrolyse third generation cephalosporins but are not inhibited by β-lactamase inhibitors such as clavulanic acid, sulbactam and tazobactam (Murray et al., 2007). The detection of the ESBL gene in the Enterobacteriaceae can be difficult if AmpC plasmids are present in the same isolate, as well as ESBL gene. To avoid this cefepime or cefpirome (AmpCstable cephalosporins) can be used in combination with β-lactamases inhibitors such as clavulanate or boronic acid, even though this detection is not 100% perfect when using these combinations (Hawkey 2008). 1.2.2.6 Carbapenemases (class A, B, D) Carbapenems have been suggested as the most effective treatment for the most extended-spectrum-β-lactamases. However, increasing reports of carbapenemases enzymes that are able to hydrolyse oxyimino-cephalosporins, cephamycins and carbapenems makes treatment difficult (Murray et al., 2007). Carbapenemases belong to three molecular classes: A, B and D. Class A carbapenemases can hydrolyse imipenem but are inhibited by clavulanic acid. Most of this class has chromosomal genes, but some are plasmid-mediated, such as KPC-1 which is found mainly in K. pneumoniae. Class B such as IMP or VIM group are not inhibited by clavulanic acid (Murray et al., 2007). Recently Yong et al., (2009) was first to report a new subgroup case of class B of metallo βlactamases called NDM-1 isolated from New Delhi, India. This mobile gene was detected on a plasmid and found mainly in K. pneumoniae. NDM-1 with 28 kDa can hydrolyse all β-lactams antibiotics except aztreonam and it represents a potential public health problem (Kumarasamy et al., 2010). Class D carbapenamases are mostly found in Acinetobacter baumannii. However, they can develop resistant to carbapenems if there is an alteration in a porin. 38 1.2.3 Emergence of ESBL: The production of the TEM and SHV β-lactamases in plasmid mediated resistance strains initiated many clinical problems after the introduction of ampicillin in the 1960s. In the early 1980s, third generation extended spectrum cephalosporins, such as cefotaxime and ceftazidime had been developed and offered reliable treatment for patients infected with Enterobacteriaceae. However, in the mid 1980s the first ESBL producing organisms (resistant to third generation cephalosporins) were isolated. Very rapidly mutations in amino acids in both TEM and SHV genes occurred, which spread specifically between Klebsiella species and some strains of E. coli. As a result in the emergence of the ESBL mutant, derivatives of these widely spread βlactamases that were capable of hydrolysing third generation cephalosporins and monobactams appeared (Hawkey 2008). Both excessive use of antibiotics and environmental conditions were therefore consider to be main reasons for the emergence and spread of resistance. ESBL have also been reported in Enterobacter, Salmonella, Proteus, Citrobacter, Morganella morganii, Serratia marcescens, Shigella dysenteriae, Pseudomonas aeruginosa, Burkholderria cepacia and Acinetobacter baumannii (Moland et al., 2008). 1.2.4 Risk factors for ESBL: To determine the risk factors of ESBL producing organisms, several studies were conducted in different countries. It was found that ESBL-producing strains were associated with low patient outcome and crowded hospitals and were also linked to improper first line treatment (Amabile-Cuevas 2007). The risk factors for most ESBLs are excessive previous use of multiple ranges of antibiotics, including third 39 generation cephalosporins, cotrimoxazole and ciprofloxacin, severely ill patients with prolonged hospital stay, or patients with indwelling medical devices such as the presence of urinary catheters, placement of endotracheal tubes for more than 10 days and old age (Hawkey 2008; Paterson & Bonomo 2005). 1.2.5 Treatment of ESBLs: Due to high rates of resistance of ESBL-producing bacteria to fluoroquinolones, the treatment can be complicated. If an ESBL-producing strain is detected in an isolate of K. pneumoniae, E.coli or P. mirabilis, the CLSI recommends the laboratory to report it as resistant to all penicillins, cephalosporins, and aztreonam, even if it showed sensitivity (Moland et al., 2008). Carbapenems have been recommended as the drug class selected for serious infections caused by ESBL producing Enterobacteriaceae strains. However, in the case of carbapenemases emergence, tigecycline revealed excellent potential activity against ESBL producing Enterobacteriaceae and Acinetobacter (Hawkey 2008). Recently, according to the survey of 104 isolates the presence of world wide a resistant strain to tigecycline was not reported (Castanheira 2008). If CTX-M ESBL is not prevalent, cefepime has been suggested as another treatment choice (AmabileCuevas 2007). 1.3 Acinetobacter: During the last two decades, bacteria of the genus Acinetobacter have been selected as one of the most important nosocomial pathogens, especially in ICU units. They have been also involved in many infections such as bacteraemia, urinary tract infection, pneumonia, skin and tissue infections and in secondary meningitis. 40 Acinetobacter spp are widespread in water and soil as free-living saprophytes (Hawkey & Bergogne-Berezin 2006). Acinetobacter is now also involved in aggressive situations such as war district zones or earthquake areas (Dallo and Weitao 2010). 1.3.1 Taxonomy and Historical Features of Acinetobacter: Acinetobacter was first described under the group of "Micrococcus calcoaceticus" by Beijerinck in 1911. In 1956 these bacteria were then classified under the name of Moraxella in France, but at the same time a group of French researchers had recognised a genus named Acinetobacter. In 1968 a phenotypic study of 106 strains was completed by Baumann which resulted in the recognition of only a single species named Acinetobacter baummanii (Towner 1997). In the early 1970's, most isolates of Acinetobacter were sensitive to many antimicrobial agents (Greenwood et al., 2003). However during the same period many microbiologists in hospitals noticed that these organisms were pathogenic and implicated in various nosocomial infections. In 1986, Bovetand and Grimont were compeleted a basic subdivision of the genus Acinetobacter and identified 12 genomic species by DNA-DNA hybridization. However, today there are at least 19 genomic species of Acinetobacter (Murray et al., 2007). Although, Acinetobacter baumannii is known to be the most clinically important strains among species, there are other important nosocomial pathogens called the „A. baumannii A. calcoaceticus complex‟ (referred to the genomospecies 1, 2, 3 and 13 of Tjernberg and Ursing) (Gerischer 2008). This complex is accountable for many epidemic infections throughout the world because of the multi-resistant gene that it contains. Other species are not very important because they are rarely involved in 41 outbreaks of human disease (Brauers et al., 2005; Joly-Guillou, 2005; Murray et al., 2007). 1.3.2 Laboratory Diagnosis: Morphologically, Acinetobacter are aerobic, non motile Gram-negative coccobacilli and are usually found in diploid shape or chains of different length. They are strictly aerobic and grow simply on all common media at temperatures from 20 to 30oC for most strains, the optimum temperature for this bacterium at 33-35oC (Winn et al., 2006). They are oxidase-negative, catalase-positive, indole-negative and nitratenegative. Furthermore, the initial clue in recognising these bacteria is the appearance of tiny (1.0x 0.7 µm) diplococci with the Gram stain (Koneman et al., 1997). Colonies appear smooth, opaque, sometimes mucoid and slightly smaller than those of members of the family Enterobacteriaceae on blood agar. Most strains appear colourless, slightly pink or lavender in colour on MacConkey agar due to lactose oxidation (Engelkirk 2007). The genus of Acinetobacter can be therefore subdivided into two groups. Acinetobacter that are able to oxidise glucose are called saccharolytic, with those that are unable called asaccharolytic (Engelkirk 2007). Most glucose-oxidizing non-haemolytic clinical strains are A. baumannii, most glucose-negative non-haemolytic ones are A. lwoffii, and most haemolytic ones are A. haemolytic (Murray et al., 2007). 1.3.3 Clinical features of Acinetobacter infections: Acinetobacter species particularly Acinetobacter baumannii, can cause many clinical disorders, including pneumonia, secondary meningitis, bacteraemia, wound infections in burn patients and UTI. They are also isolated from skin, throat and 42 many secretions of normal people and are part of the commensal flora (Hawkey & Bergogne-Berezin 2006). Other species such as A. lwoffii, A. johnsonii, and A. radioresistens, seem to be natural inhabitants of human skin and as commensals in the oropharynx and vagina (Winn et al., 2006). They are considered as less resistant to antibiotics and easier to eliminate. Two recent species have been described which are associated with infections; these are A. ursingii and A. schindleri (BergogneBerezin et al., 2008). Acinetobacter can only be obtained from soil, water, food and sewage (Towner 1997) and are also able to live for long periods in lifeless environments (Greenwood et al., 2003). In the case of wound infections, bacteraemia within 3-5 days following infection can often develop. In several large case series, 4-27% of all Acinetobacter that caused bacteraemia occurred as a result of infected surgical or burn wounds (Gillespie 2004; Hawkey & Bergogne-Berezin 2006). Such infections are often difficult to treat because of the ability of Acinetobacter to become rapidly resistance to multiple antibiotics, including aminoglycosides, expanded-spectrum cephalosporins, carbapenems and fluoroquinolones (Gerischer 2008). Inappropriate or excessive use of antibiotics therapy (i.e third generation cephalosporin), surgery, use of medical machinery (e.g. ventilators), insertion of intravenous or urinary catheters, and prolonged hospital stay are all identified as risk factors for colonization and infection with Acinetobacter (Hawkey & BergogneBerezin 2006). Soap and water hand washing and alcohol based gels, could therefore reduce the spread of this strain (Joly-Guillou 2005). Acinetobacter has been detected from a large selection of clinical samples, including blood, urine, faeces, cerebrospinal fluid and sputum (Gillespie 2004). It is an opportunistic pathogen and is commonly found in patient samples. However, serious infection caused by Acinetobacter depends upon the site of infection as well as the patient‟s immunity to infection (Murray et al., 2007). Furthermore, Chiang, et al., 43 (2008) added increased serum creatinine level and malignancy as risk factors associated with increased mortality in patients with bacteraemia caused by Acinetobacter. A European survey of the main cause of nosocomial pneumonia carried out in seven countries has established an overall incidence of approximately 10% for Acinetobacter (Hawkey & Bergogne-Berezin 2006). Also, during a study period from 2003 to 2006 for over 270 patients admitted every year in a burn clinic, an increased trend of Acinetobacter strains was confirmed (Babik et al., 2008). Recently, over 21,000 American army personnel who were injured during the Iraq war have suffered severe wound infections, mostly from resistant strains of Acinetobacter baumanii (Murray et al., 2008). Scientists examined Iraq and Kuwait soil for the presence of this pathogen but it proved negative. The source of this outbreak could therefore be from European hospitals (Silberman 2007). However, this bacterium caused bacteraemia, osteomyelitis and respiratory infections for the soldiers. Also this pathogen is able to form a biofilm which will reduce its susceptibility to systemic antibiotics and make treatment more difficult (Dallo and Weitao 2010). In this situation significant Acinetobacter infections have increased worldwide and the outbreaks of resistant strains of Acinetobacter have been described in the medical literature (Bergogne-Berezin et al., 2008). 1.3.4 Pathogenesis of Acinetobacter infection: Bacteria produce many substances and molecules that allow them to survive and grow in a host. These molecules are proteins, enzymes, capsules, toxins and surface carbohydrates (Bergogne-Berezin et al., 2008). Acinetobacter spp. were thought to be relatively low-grade pathogens, but a number of virulence factors have been identified. These include: 44 1.3.4.1 The production of exopolysaccharide: The presence of exopolysaccharide capsule helps in the protection of bacteria from host defences. A capsule is produced by approximately 30% of Acinetobacter strains and it consists of L-rhamnose, D-glucose, D-glucuronic acid, and D-mannose, which make the cell surface of strains more hydrophilic (Joly-Guillou 2005; Hawkey & Bergogne-Berezin 2006). Acinetobacter strains which produce exopolysaccharide are known to be more dangerous than those without. This is because this capsule can block the entry of complement to the bacterial cell wall and interrupt the alternative pathway of complement activation (Joly-Guillou 2005). 1.3.4.2 Quorum-sensing: Quorum-sensing is defined as the ability of bacteria to initiate the transcription of certain genes only when a certain population density is reached. It is known as a widely distributed regulatory mechanism in Gram-negative bacteria such as Pseudomonas aeruginosa (Wilson et al., 2002). Acinetobacter isolates in the stationary growth phase have demonstrated four different signal molecules of quorum sensing involved in activating N-acylhomoserine-lactone (AHL) biosensors. The AHLs system can therefore act as a main mechanism for auto-induction of several virulence factors in an opportunistic pathogen such as Acinetobacter. This process need to be studied for its clinical implications (Joly-Guillou 2005). 1.3.4.3 The property of adhesion to human epithelial cells via the capsule or fimbriae. The initial step in the infection process is the ability of bacteria to penetrate the host. This step depends on the adherence capacity and the survival time of microorganisms on mucosal surfaces of the host. Bacterial adherence involves the possession of 45 fimbriae, the production of capsular polysaccharides and cell wall components (Bergogne-Berezin et al., 2008). Recently, two different types of adherence were observed in A. baumannii to epithelial cells of human bronchial. The first one was diffusing adherence of bacteria to the cell surface and the other type was a group of clusters of bacteria that adhered to a localized area of the cell by producing small colonies (Bergogne-Berezin et al., 2008). 1.3.4.4 Surface and mitochondrial porins: On the outer membrane of the surface of Gram negative bacteria there are special channels consisting of protein molecules called porins. Depending on bacterial species, porins play a role in the maintenance of the cell structure, bacteriophage and resistance mechanisms of antimicrobial agent (Bergogne-Berezin et al., 2008). Surface porins allow the passive diffusion of low molecular weight components to penetrate through this membrane. Large antibiotic molecules penetrate slowly, which may account for the high antibiotic resistance of A.baumannii. For example, the permeability of the outer membrane varies from one Gram negative species to another; in Pseudomonas aeruginosa (which is extremely resistance to antibiotics) the outer membrane is 100 times less permeable than in E.coli (Brooks et al., 2001). A study showed the permeability of the outer membrane of Acinetobacter for a cephalosporin was 2-7 times lower than in P.aeruginosa (Vila 1998). Many considerations that involve host factors, the bacterial load, the virulence of strains and the production of lipase enzymes such as butyrate esterase, caprylate esterase and leucine arylamidase which may damage tissue lipids may play important roles in initiating infection in colonised patients (Towner 2002). 46 1.3.5 Emergence of Resistance: A.baumannii and related species have acquired resistance to multiple antibiotics rather than being inherently resistant. When these species were first introduced as pathogens to human, most strains were sensitive to ampicillin and cephalosporins. In 1975, less than 20% of these strains were resistant to ticarcillin. However, at the end of the 1970s and early 1980s, A.baumannii caused increase resistance to second generation cephalosporins which being used to control nosocomial infections. When the third generation cephalosporins were first introduced, A.baumannii developed resistance to cefotoxime and ceftazidime. This bacterium therefore has an excessive acquired resistance to β-lactam drugs (Towner 1997). There are no specific treatment guidelines for Acinetobacter spp. due to the large variation in antibiotic resistance. To determine the best mode of treatment for a particular isolate, antimicrobial susceptibility testing must be performed (Forbes 2007). Although, carbapenems have been the drug of preference in the treatment of Acinetobacter infections numerous reports in the medical and scientific literature have documented resistant strains to carbapenems such as imipenem and meropenem (Costa et al., 2000; Levin 2002; Perez et al., 2007). According to the Health Protection Agency in the UK (HPA) a survey of 1,225 cases of bacteraemia due to Acinetobacter spp were reported from England, Wales and Northern Ireland in 2007, with total incidence rate of 2.2 per 100,000 populations. In the same survey 12% of Acinetobacter spp were shown to be resistant to imipenem, whereas the prevalence of ciprofloxacin and gentamicin resistance was 16% and 12% respectively (HPA 2008) Currently, several surveys have studied the prevalence, mode of transmission and risk factors of multi-drug resistant A. baumannii in ICUs and burn clinics. They reported an increased incidence of an outbreak clone of A. baumannii (Babik et al., 47 2008; Bacakoglu et al., 2009; Barchitta et al., 2009; Cootz and Marra 2008; Fontana et al., 2008). 1.3.6 Carbapenem action on Acinetobacter: Carbapenem is the most effective broad spectrum antibiotic among all of the βlactams and imipenem is one of the most important carbapenems (Bergogne-Berezin et al., 2008). Imipenem is an active agent against many organisms including Gram positive and Gram negative aerobes and anaerobes. It is a bactericidal agent that kills or destroys bacteria at 2-4 times the MIC for most species (Greenwood et al., 2003). The initial step of drug action in destroying bacteria is drug binding to the cell wall receptors known as penicillin binding proteins (PBPs). The transpeptidation process is stopped and peptidoglycan synthesis is blocked after β-lactam drug binding to one or more receptors. The next step involves the removal or suppression of autolytic enzymes inhibitor in the cell wall. This activates the lytic enzyme which results in lysis of cells leads to cell death (Brooks et al., 2001). 1.3.7 Mechanisms of Carbapenem Resistance: There are several complex mechanisms and genetics of resistance acquired by this species which involve several plasmid-borne β-lactamases and aminoglycoside modifying enzymes, as well as variation in membrane permeability and alteration in penicillin-binding proteins. The possession of these multiple mechanisms may be due to the physiological capability of Acinetobacter and it can obtain DNA by transformation in vivo (Finch 2003) 48 In the last few years resistant strain of A. baumannii to carbapenem have been reported globally and known as imipenem and meropenem resistant A. baumannii (IMRAB). The epidemic strains of IMRAB demonstrated three different mechanisms of β-lactamases, these are: plasmid mediated enzymes (TEM-1), chromosomal mediated enzyme (Noval OXA-type) and cephalosporinase ampC-type enzyme (Bou et al., 2000) Major carbapenem-resistant Acinetobacter species have metallo-enzyme and OXAtype enzymes (Bou et al., 2000). However, OXA-type β-lactamases which belong to class D β-lactamase have a poor activity against carbapenems; such enzymes discovered in A. baumannii isolates from Argentina, Belgium, Kuwait, Scotland, Spain and Singapore. Many of this group of enzymes have been classified to form a subgroup in class D β-lactamases, currently including the OXA-23, -24, -25, -26, -27 and -40 types (Song et al., 2004). There are several factors that determine the acquisition of multi- resistance in A. baumannii. One is the intrinsic resistance of microorganisms, due to low level diffusion of certain antibiotics through the outer membrane because of low number of porins present (Levin 2002). Another is due to the acquisition genetic elements; there are 3 types of mobile genetic elements have been found in Acinetobacter. These are plasmids, transposons and integrons (Vila 1998). The plasmids contains 3 resistance genes; genes encoding ß-lactamase TEM-1, TEM-2, and CARB-5 (Bou et al., 2000). The plasmid encoded β-lactamases have attracted great attention in which the resistance of this bacterium occurs by a single genetic event. However, this type of resistance occurs mostly in the highly selective environment of the hospital (Greenwood 2000). Integrons, which are chains of genes with a greater mobility to transfer from one location of A.baumannii chromosome to another with help of a transposon, carry this component (Vila 1998). This may be an important factor in the 49 ability of Acinetobacter species to survive in human and environmental reservoirs in which the genes of resistance may be transferred (Vila 1998). For multi-drug resistant Acinetobacter infections, several studies have demonstrated clinical effectiveness of sulbactam in combination with ampicillin or cefoperazone. The only effective antibacterial agent to this bacterium is colistin (Winn et al., 2006). One report has demonstrated the efficiency and safety of colistin in patients with Acinetobacter infection that was not susceptible to carbapenem and shown that 57% of patients cured with colistin therapy, without prolonged neuro-muscular blockade as a side effect of therapy (Torres et al., 2007) Recently Enoch and his colleges (2008) completed a six month study of the outbreak caused by multi-drug-carbapenem-resistant Acinetobacter baumanii (MRAB-C) strain in UK hospitals. This outbreak would have increased the rate of mortality if not controlled properly. However, isolation of the patients infected with MRAB-C, education of staff dealing with those patients, early patient and environmental screening, and effective hygiene all helped to control this outbreak. Also, patients infected with MRAB-C were treated with colistin and tigecycline and improved. 1.3.8 Acinetobacter Treatment with Honey: Due to the emergence of bacteria resistant to antibiotics, the bactericidal properties of manuka honey have been extensively researched. Currently, few studies have reported the antibacterial activity of honey against Acinetobacter. George & Cutting, (2007) initiated an in-vitro study of the antibacterial activity of Medihoney against 130 clinical isolates of multi-drug resistant organisms including Acinetobacter. The study showed that the concentration needed to inhibit the resistant Acinetobacter strains was 8% (v/v) of honey. 50 More recently, a study was carried out using Malaysian tualang honey in comparison to manuka honey against wound pathogens including Acinetobacter. The antibacterial activity for both honeys was same with the MIC ranges between (11.25 & 12.5% w/v) (Tan et al., 2009). Although Acinetobacter spp. have been found to be susceptible to honey, more objective evidence derived from clinical trails and animal models to determine whether honey has a similar antimicrobial effect in-vivo are required. 1.4 Alternative Antimicrobial Therapies: As concerns about antimicrobial resistance increase, efforts of the pharmaceutical industry to develop new drugs have diminished and the possibility of running out of effective antimicrobial agents has increased. It takes 10-12 years for new antibiotic to be developed and costs approximately £250 million for each one (Greenwood 2003). Yet the chance of developing a new drug that will have excellent bactericidal properties without causing the emergence of resistance is impossible. The introduction and application of honey into clinical practice several years ago has put attention on using it for treatment of various infections. An extensive review of clinical studies by Molan suggested that honey might be successfully used as an antimicrobial agent and also in promoting healing of wounds (Molan 2006). 1.4.1 Ancient Use of Honey as a Medicine: Honey has been used for many thousands of years as a food, a medicine and it has been incorporated into cosmetics. A large number of different cultures have extensively used honey as a medicine for many disorders. It has been used in wound 51 care since the time of ancient Egyptians, as suggested by an inscription on a Sumarian clay tablet. Honey was also mentioned in the Holy Koran, the Talmud, the Bible, as well as the sacred books of India, China, Persia and Egypt (Zumla & Lulat 1989). All the clues point to the medicinal use of honey throughout human history. 1.4.2 Honey as a Modern Medicine: In the last 30 years interest in the use of honey as a treatment agent has increased. Most research that has been undertaken has focused on the employment of honey in wound treatment (Ahmed et al., 2003; Berguman et al., 1983; Dumronglert, 1983; Emarah, 1982; Haffejee & Moosa, 1985; Ingle et al., 2006; Wadi et al., 1987). In 1988, Efem reported the first large clinical cohort study involving 59 patients who had a variety of wounds such as Fournier‟s gangrene, burns and ulcers. The use of honey on these patients resulted in successful wound healing and the clearance of infection. In addition Subrahmanyam (1993, 1994, 1996, 1998) and Subrahmanyam et al., 2001, 2003, 2007) reported several clinical trials on burns patients with honey compared to various different treatments. Clinically, many researchers have studied the uses of honey in wound management and it has been reported to clear wound pathogens rapidly (Al-Waili and Saloom, 1999; Lusby et al., 2002), to stimulate immune response and to reduce inflammation (Molan and Betts 2001; Tonks et al., 2003) and to support the debridement of wounds by autolysis (Stephen-Haynes 2004). In addition, honey has been reported to have a deodorising property on wounds, due to the oxidation of glucose by bacteria resulting in production of lactic acid rather than malodorous compounds such as ammonia, sulphur compounds and amines produced by the breakdown of amino acids (Cooper 2005; Molan 2002; Stephen-Haynes 2004). Moreover, honey has been used effectively on skin grafts (Schumacher 2004), diabetic foot ulcers (Eddy & 52 Gideonsen 2005), malignant ulcers (Simon et al., 2005) and abscesses (Okeniyi et al., 2005). Some researchers have observed that honey promotes tissue regeneration through the stimulation of angiogenesis and the growth of fibroblasts and epithelial cells (Efem, 1988, 1993; Stephen-Haynes 2004; Subrahmanyam, 1994, 1998). Fast healing can therefore minimise the need for skin grafts (Subrahmanyam 1998). Recently, (Gethin et al., 2008) observed that the use of manuka honey as a wound dressing reduced wound pH which in turn decreased protease activity, increased fibroblast activity and released more oxygen from haemoglobin to promote rapid wound healing. Furthermore, after honey is applied to the wound, it forms a film of liquid between the wound and the dressing that prevents the dressing from sticking to the wound, reducing pain and not damaging the newly formed cells. As honey has no adverse effects on tissue, it can be used on wounds safely and introduced into cavities and sinuses to clear infection (Molan 2000). Despite, extensive anecdotal evidence to support the topical used of honey in treating wounds, systematic review of the clinical evidence has not been so supportive (Bardy et al., 2008; Jull et al., 2008; Moore et al., 2001). 1.4.3 Antimicrobial Activity of Honey: The antibacterial activity of honey was first identified by Van Ketel in 1892 (Dustmann 1979). After that several studies established the antibacterial activity of honey against various bacterial pathogens and fungi (Cooper et al., 1999; Efem, et al., 1992; Molan, 1992a; Molan, 1992b; Mulu et al., 2004; Lusby et al., 2005; Wilkinson and Cavonagh 2005). It was shown that honey inhibits various bacterial 53 species. There are many reports of it being bacteriostatic and bactericidal (Alandejani et al., 2009; Henriques et al., 2009; Molan 1992b). Undiluted honey was shown to prevent the growth of Candida albicans and demostrated potential as a topical treatment of external fungal infections such as ringworm and superficial candidiases (Brady et al., 1997; Efem 1992; Irish et al., 2006; Wahdan 1998). Cooper et al., (1999) showed that honey has an effective antibacterial activity against the major wound infecting species including Staphylococcus aureus. A year later the sensitivity of multi-resistant strains of Burkholderia cepacia isolated from cystic fibrosis patients to manuka honey at concentrations below 6% (v/v) was reported (Cooper et al.,2000). Cooper et al., (2002a) compared the antimicrobial activity of artificial honey ( a sugar solution) and two natural honeys (manuka and pasture honey) against 18 strains of MRSA isolated from wounds, 20 strains of vancomycin-resistant enterococci (VRE) and 7 strains of vancomycin-sensitive enterococci (VSE). The study showed the minimum inhibitory concentration (MIC) which is the concentration required to inhibit the growth for the natural honeys was below 10% (v/v) and < 30% (v/v) with artificial honey for all strains. This means the antibacterial activity of honey is not limited to osmolarity. Also in the same study it was concluded that there was no difference in the MIC values between the sensitive and resistant Gram positive strains. Furthermore, the antimicrobial activity of the same two natural honeys was tested against 17 strains of Pseudomonas aeruginosa isolated from burns. Both honeys maintained bactericidal activity when diluted more than 10-fold (Cooper et al., 2002b). In addition, a study showed that manuka honey (MIC 3.4±0.5% (v/v)) has a potential activity to control and prevent infection with coagulase-negative staphylococci (French et al., 2005) 54 Nezeako & Hamdi, (2000) tested six commercial honey samples against control organisms, Staph.aureus, E. coli, P. aeruginosa and various clinical isolates. They found that some samples had high broad-spectrum antimicrobial activity which resisted refrigeration temperature for six months and being boiled for 15 minutes. In addition Mullai and Menon (2007) tested the antibacterial effect of different types of honey against 150 strains of P. aeruginosa isolated from otitis media, diabetic foot ulcers and burns wound. MIC of 20% (v/v), 11% (v/v) and 20% (v/v) were determined from manuka, khadikraft and heather honey respectively. Recently, Blair et al., (2009) studied the antimicrobial activity of Leptospermum Medihoney with high levels of hydrogen peroxide-dependent activity or Comvita manuka woundcare 18+ against MRSA, Acinetobacter and 6 strains of multi-drug resistant Enterobacteriaceae. MICs ranged from 4 to 5% w/v, 6.0 to 9.3% w/v and 6.3 to 14.8% w/v respectively. This indicated that active Leptospermum honey is potentially active against antibiotic-resistant clinical pathogens. A survey was carried out with regard to 345 samples of New Zealand honey to assess the antibacterial activity of honey. Four types of honey were shown to have high antibacterial activity equivalent to phenol standard. In this assay, antibacterial activity was not detected in almost all honeys when catalase was added to remove hydrogen peroxide. However, manuka and vipers bugloss honeys showed measurable amount of hydrogen peroxide which is believed to aid antibacterial activity (Allen et al., 1991). 1.4.4 Chemical composition of honey: Honey is a combination of sugars, water, and other compounds (Table 1.1), the specific composition depending largely on the mix of flowers foraged by the bees. It 55 has been reported that approximately 181 substances are present in honey (Terrab et al., 2003). Table 1.1: Honey composition Substance Percentages % Water 17.1 Fructose 38.5 Glucose 31.0 Maltose and other reducing disaccharides 7.2 Sucrose 1.5 Tri-saccharides and other carbohydrates 4.2 Minerals, Vitamins & Enzymes 0.5 Sammataro and Avitabile (1998) The composition of honey varies from one honey to another depending on several factors. A major factor is the floral source, as the nectar from different plants will contain different compositions of the main sugars and trace elements. These compositions are influenced by soil type, climatic conditions (seasons) and the environment surrounding the plant (Crane 1979). It is recognized that some chemical changes occur when the nectar is transformed to honey. These changes are mainly because of some bee enzymes deposited in the honey. These enzymes are invertase that hydrolyses sucrose into glucose and fructose, amylase or diastase enzymes and glucose oxidase that generate gluconic acid and hydrogen peroxide from glucose in diluted honey. Other enzymes which are also present in the honey are catalase and acid phosphatase (Sammataro and Avitabile 1998). 56 In addition, honey contains several B vitamins such as riboflavin, niacin, folic acid, and B6. Moreover, honey contains a number of minerals such as calcium, iron, zinc, potassium, phosphorus, magnesium, selenium, chromium and manganese (Atrouse et al., 2004; White 1975). Cooper and Jenkins, (2009) compared the antibacterial activity of medical grade honey with 18 table honeys collected from different regions. They found that all table honeys have less antibacterial activity compared to medical grade honey. Moreover, all table honeys were non sterile and contained various bacterial species such as mesophilic aerobic bacteria, coliforms and clostridia. 1.4.5 Factors Contributing Antibacterial Properties of Honey: Until 1963, it was thought that the antimicrobial properties of honey were mainly because of hydrogen peroxide, but further studies have indicated that other physical factors like acidity, osmolarity (Molan 1992a) and electrical conductivity, and chemical factors including volatile compounds (Yao et al., 2003), antioxidant (Gheldoff et al., 2002; Henriques et al., 2006), beeswax, propolis and pollen (ViudaMartos et al., 2008) play a considerable role in antimicrobial activity. 1.4.5.1 Osmotic effect: Honey is a super saturated solution of sugar (80%) and water (17%). The osmolarity of honey inhibits microbial growth because of the strong interaction of sugar molecules with water molecules thus, insufficient water molecules are available to support microbial growth. This availability is known as water activity (aw). Water involved in many metabolic processes in many organisms. Depending on the 57 permeability of cell membrane in each organism the water activity (aw) of many bacterial species is vary between 0.94-0.99. The water activity of honey is 0.6 because of high sugar molecules and low water thus many species cannot grow in that environment. Fungi can tolerate a lower aw than bacteria, so reports of antifungal activity with diluted honey reveal that there are more factors involved than only the sugar content of honey. Also, Staph aureus has a high tolerance of low aw (0.86) ie. can tolerate high NaCl level but not high sugar therefore, it considered as one of the most susceptible species to the antibacterial activity of honey (Molan 1992a). 1.4.5.2 Acidity Honey is quite acidic; normally, it has an average pH of 3.9 (with a typical range of 3.2 to 4.5). It has been known that this acidity is a result the conversion of glucose to gluconic acid with help of glucose oxidase enzyme (Molan 2001b). The optimum pH for growth of many bacterial species is 7.2 – 7.4. However, the lowest pH value for growth of some wound pathogens is 4.3 for E .coli and 4.4 for P. aeruginosa. The low pH of honey is therefore important to slow down or inhibit bacterial growth (Bogdanov 1996; Molan 2000a). Since 2001, the osmotic effect was thought to be the main factor for antimicrobial activity (Molan 2001b). However, in 2005 a study compared honey and sugar solution of same osmotic effect on coagulase negative staphylococci. The study confirmed that antimicrobial properties are not exclusively due to osmotic effect (French et al., 2005). It has been noted that the pH of honey also generates and maintains good environment for fibroblast activity (Lusby et al., 2002). 1.4.5.3 Hydrogen peroxide production In 1919, Sackett reported that in diluted honey the antibacterial properties of honey were increased. This is because when honey is diluted, hydrogen peroxide is released 58 with the help of an enzyme (glucose oxidase) that is found in honey (Molan 1992b). This enzyme is secreted by the hypopharyngeal gland of bees and added to nectar during honey formation (Borland 2000). Glucose + H2O + O2 glucose oxidase gluconic acid + H2O2 Hydrogen peroxide (H2O2) is considered to be one of the main factors in antibacterial activity of honey. It is involved in cell multiplication in different cell types in the body as certain a concentration of H2O2 can support epithelial cells and fibroblast growth to repaire damage or injury (Burdon 1995). It also promotes wound healing by regeneration of new capillaries (Tur et al., 1995). The enzyme (glucose oxidase) is inactive in full strength honey due to the low pH, so the diluting action of fluids produced by the wound is thought to activate glucose oxidase to produce hydrogen peroxide. In addition, it stays in the honey during storage without losing activity. Hydrogen peroxide was used for long time to disinfect wounds in hospitals. This chemical causes damage to the tissues and inflammation due to free radical that is produced. The levels of H2O2 in honey are around 1000 times lower than those applied as antiseptic on wounds (Molan 2001b). As a result it does not inflame a wound or damage the tissue (Bang et al., 2003). Weston (2000) suggested that the level of H2O2 was related to floral source, and that it depended on the balance between the production and destruction rate of H2O2. Destruction of H2O2 is due to catalase which derives from both the pollen and the nectar of plants, and the amount of catalase in different sources is variable. In addition, Brudzynski (2006) studied the effect of H2O2 on the antibacterial activity of 42 honey samples from Canada. She found that the antibacterial activity was correlated with production of H2O2 in honey. 59 1.4.5.4 Non-peroxide Components Several efforts were made to identify the non-peroxide antibacterial components present in the honey (Allen et al., 1991). Weston et al., (1999) separated the antibacterial phenolic fraction (APF) from the honey which consisted of benzonic acids, cinnamic acids and flavonoids. It was determined that APF plays a small role in manuka honey as non-peroxide antibacterial component, therefore, there are other factors which were need to be identified. Honey contains a variety of polyphenolic compounds that may be capable of chelating metal ions and decreasing oxidation (Gheldof et al., 2002). Two important classes of phenolic compounds are flavonoids and phenolic acid which are known as natural antioxidants (Molan 1992a; Pyrznska and Biesaga 2009; Yao et al., 2003). In a study performed by Wahdan (1998), two phenolic acids were extracted for the first time; these were caffeic acid and ferulic acid. Flavonoids had shown a range of biochemical and pharmacological actions, which affect the inflammatory cells and the generation of inflammatory processes (Viuda-Martos et al., 2008). The use of flavonoids in medicine is increasing due to their ability to trap free radicals, to stimulate hormones and neurotransmitters, and to inhibit specific enzymes which produce superoxide anions (Pyrznska and Biesaga 2009). However, it has been identified that several organic components in the ether extract of honey possess antibacterial activity; these include 3,5-dimethoxy-4-hydroxy benzoic acid (syringic acid), and methyl 3,5-dimethoxy-4- hydroxy benzoate (methyl syringate) (Russel et al., 1988). By using high performance liquid chromatography (HPLC), some other flavonoids and phenolic acids have also been identified in different honeys, for example, pinocembrin, pinobanksin and chrysin (Bogdanove et al., 1989), gallic acid and abscisic acid (Yao et al., 2003) caffeic acid and ferulic acid 60 (Wahdan 1998), and vanillic acid, cinnamic acid, and benzoic acid (Weston et al., 1999; Weston et al., 2000). 1.4.5.5 Antioxidant activity: Antioxidants are substances that protect wound tissues from being damaged by oxygen radicals. The free radicals may be produced by hydrogen peroxide and cause cellular damage. Free radicals are involved in cell toxicity and can alter cell biomolecules such as proteins, carbohydrates, lipids and nucleic acids causing cell death (Nagai et al., 2001). Gheldof et al., (2002) analysed the antioxidant activity in different honey fractions and determined that most of the antioxidant components were found in the watersoluble fraction. These include gluconic acid, protein, ascorbic acid, hydroxymethylfuraldehyde, and the combined activities of the enzymes glucose oxidase, catalase and peroxidase. The same study also showed that the phenolic compounds in honey contributed very significantly to its antioxidant capacity. When honey is diluted the release of high levels of hydrogen peroxide may lead to tissue damage by formation of free radicals such as hydroxyl and superoxide. Many honeys including manuka honey have the ability to quench free radicals. This property may play a role in reducing inflammation and chronic wound infection (Henriques et al., 2006) A recent study was completed by Van de Berg et al., (2008) with regard to the antioxidant level in buckweat honey showing that this type of honey reduced the level of reactive oxygen species (ROS) which affect the wound healing process. Also, beside the low pH and high acidity buckwheat honey was shown to contain high amounts of phenolic components that aid the antimicrobial mechanisms and 61 block the oxidative reaction system (Inoue et al., 2005). In addition, several reports demonstrated the relationship between the antioxidant and the colour of honey, where darker honey exhibited higher antioxidant content (Bogdanov et al., 2004; Estevinho et al., 2008; Turkmen et al., 2006). It has been thought that non-hydrogen peroxide activity in manuka honey may be due to plant derived components such as flavonoids and phenolic compounds. Recently, two research groups have reported that the activity of Leptospermum honeys correlates with the presence of methyglyoxal (MG), an alpha-oxoaldehyde that reacts with macromolecules such as DNA, RNA and proteins (Adams et al., 2008; Mavric et al., 2008). High amount of MG was present in some manuka honey which is equivalent to the non-peroxide activity. MG was, therefore, known as a bioactive complex responsible for the antibacterial activity in manuka honey (Mavric et al., 2008). Recently Atrott and Henle (2009) studied the presence of methylglyoxal in 61 samples of manuka honey. They found that the antibacterial activity ranged between 12.4% to 30.9% equivalent to phenol concentration. More recently Kwakman et al., (2010) discovered an antibacterial bee peptide called bee defensin-1 in honey. To date this peptide has been isolated only from a honey used in the production of Revamil and it was confirmed that this protein exhibits most of the antibacterial activity. The exact mechanism of bee defensin-1 on bacteria is not yet known. 62 Table 1.2: Comparisons between peroxide and non-peroxide honey Form Effected by heat & light Effected by long storage Origin: Bee Origin: Flora Mode of action Peroxide honey Non-peroxide honey H2O2 Polyphenolic compounds Sensitive Thermostable Yes No glucose oxidase Honey acidity, diastase & invertase enzymes - Flavonoids, phenolic acids active only when diluted, Antioxidant, MGO tissue repair High level Bad- release of free radical Good- more scavenging (quenching properties) Example Almost all honey Manuka, Jelly bush honey 63 1.4.5 Manuka Honey: Manuka honey comes from the tree (Leptospermum scoparium) and is currently approved for therapeutic use in many countries. The honey mainly derived from nectar taken from trees of L.scoparium variety is referred to as manuka; a closely related shrub is Kunzea ericoides commonly referred to as kanuka. These are shrubs which form bushes with height of 12-15 ft. They belong to the Myrtaceae family and are native to New Zealand although other species of Leptospermum are found in Australia. A survey of 345 New Zealand honeys found that antibacterial activity of manuka honey was retained in the presence of catalase, and was called non-peroxide activity, while most other types of honey were found to be inactive when catalase was added. The later honeys were called peroxide honeys. In this study antibacterial assays were performed using phenol as a standard and Staphylococcus aureus as the test strain. This developed a measure of activity relating to percentage of phenol which had the same degree of antibacterial activity (Allen et al., 1991). This system was then granted by New Zealand government as the UMF or „Unique Manuka Factor‟ to give a standard for customers. It is now recommended to use honey with a UMF of 10 or higher (equivalent activity of 10% phenol) to ensure sufficient activity circulate into deeper tissues where severe wounds are involved. Higher UMF ratings indicate higher levels of antibacterial activity (Molan 2001b). Recently, several rating systems developed by increasing the companies that produce manuka honey. Methylglyoxal (MG) and Molan Gold Standard are new registered trademarks from different organizations to rate the potency (http://www.molangoldstandard.co.nz/article, 2010). 64 of manuka honey Another study compared the effectiveness of manuka honey with other peroxide honey against 7 Helicobacter pylori strains isolated from biopsies of stomach ulcers. The MIC was 5% (v/v) for manuka honey & >40% (v/v) for other honey (Al Somal et al., 1994). Some studies have reported the in vitro effectiveness of manuka honey against biofilms produced by 3 species; Pseudomonas aeruginosa, methicillin resistant Staphylococcus aureus (MRSA) & methicillin sensitive Staphylococcus aureus (MSSA) with killing rate of 91%, 63% and 82%, respectively (Alandejani et al., 2009; Okhiria et al., 2009). The high level of methyl syringate in manuka honey was proved to scavenge superoxide anion radicals (Inoue et al., 2005). In addition, Stephens and his colleagues (2009) have analysed the phenolic components in manuka and kanuka honeys. Both honeys have six phenolic acids in common as a primary component. In the same study elevated levels of MG in manuka honey acted as a source of antibacterial activity. Both of these components (MG and phenolic compounds) could contribute to the bacterial effect of honey in medical use. The conclusion from these observations is that certain honeys contain antimicrobial factors such as methylglyoxal and bee defensin-1 in addition to sugar content, low pH and hydrogen peroxide generation. However, in order for honey to be accepted as an alternative to antimicrobial, it is desirable to characterise the components that are responsible for its activity. Although many constituents of the antibacterial activity of honey are known, such as the sugars, pH, hydrogen peroxide, and more recently MG and bee defensin-1, these do not account for the total antibacterial activity observed in many honeys. However, complete identification of the antibacterial components has not been achieved 65 because of the complexity of honey itself and the possible interaction between different substances present in the honey. Recently, a few studies concentrated on the effect of honey against certain bacteria by looking into the intracellular change in order to find the mechanism of action and the target site of the honey. They found that 10% (w/v) of manuka honey was able to cause marked structural changes to Gram positive S.aureus. The mechanism was not fully understood however; the inhibition of the cell cycle with increased septa formation is obvious in this study and is considered as one mechanism leading to cell death (Henriques et al., 2009). A similar study with P. aeruginosa has demonstrated that manuka honey induced cell lysis (Henriques et al., 2010). 1.4.6 Omani Honey: Beekeeping has been practised since ancient times in Oman. Oman has a wideranged landscape characterized in its dried-up river beds, hills, plains and deserts in which grow the plants and trees that supply the honey bee with the nutrients it requires. Such trees are palm trees, coconut palms, cereals, limes, vegetables, sugar cane, frankincense and gum trees (Al-Taie et al., 1999) In particular, trees such as the Simr (Acacia tortilis), Sidr (Ziziphus spina-christi), Ghaf (Prosopis cineraria), coconut palm, prickly pear and papaya trees make the primary ingredients that give Omani honey its distinctive flavour (Al-Taie et al., 1999). Honeycombs are formed within one and half months and harvested twice a year, which is long enough not to be mixed with the date formation period. Acacia tortilis take part in the production of honey, because it flowers at a different time of year compared to other trees. This expands the season in which bees can collect nectar and produce their honey. Total polyphenols, flavonoids and antioxidant levels 66 of raw honey samples from Acacia, have been evaluated. Phenolic content, expressed as caffeic acid equivalents, ranged from 3 to 11 mg/100 g in Acacia. Total flavonoids in 100 g Acacia honey were in the range of 0.45–1.01 mg CE (Blasa et al., 2006) Two types of bees have been identified in Oman these are Apis mellifera and Apis florae. The specialist beekeepers of northern Oman have build up a huge skill in gaining honey and proliferating bee colonies in a controlled approach (Sajwani et al., 2007a). The distribution area of A. florae is commonly restricted to warm climates. In the west, this species is found in the warmer parts of Oman, Iran and Pakistan, through India and Sri Lanka (Akratanakul 1990). A recent 3 year melissopalynological study of 48 Omani honey samples collected from 14 locations in the Muscat and Al Batina regions of Oman was conducted. It was found that 32 honey samples among 48 are monofloral types and the other 16 were multifloral. Overall 122 pollen types from 50 plant families were recognized (Sajwani et al., 2007a). In addition, sugar and protein profiles of same Omani honeys were measured (Sajwani et al., 2007b) Al-Jabri et al., (2003) compared the antibacterial activity of 16 honeys from different parts of Oman, and 8 from different countries in Africa, against three organisms Staph.aureus, E. coli, P. aeruginosa. It was found that Dhofar honey (Oman) and eucalyptus honey (Uganda) had the highest level of activity against the three test organisms. Another study was performed by the same group on the interaction of honey and bovine milk against S.aureus (Al-Jabri et al., 2005b). In addition, anti-Staphylococcal activity of thirty types of Omani honey was tested alone and in combination with gentamicin. It was observed that thirteen of the Omani honeys had high anti-Staphylococcus aureus activity. The killing rate for the best honey was 38% of Staphylococcus aureus using 50% (w/v) concentration honey in 67 30 minutes. Gentamicin (4µg/ml) killed 70% of isolate; honey and gentamicin were combined to give excellent killing rate at 92% in the same duration (Al-Jabri et al., 2005a). The first study of the ability of honey to prevent bacterial adherence in-vitro was done by Al-Naqdy et al., (2005). Four different types of Omani honey were used in this study of growth inhibition. Bacterial adherence was examined using Salmonella enteritidis that had been incubated first with honey and then with intestinal epithelial cells. Results showed decreases in the number of bacteria attached to the treated epithelial cells from 25.6±6.5 to 6.7±3.3 bacteria per epithelial cell (P<0.001). The efficacy of Oman honey against antibiotic resistant strains of wound pathogens has not been investigated, and antibacterial activity has not been compared to that of medical grade manuka honey 68 1.5 Aims and Objectives: The aim of this study was to investigate the inhibition of MDR bacteria including ESBLs by a medical grade honey and a selection of Omani honeys. The following objectives were identified: 1. To investigate the effect of a medical grade manuka honey on MDR bacteria possessing ESBLs by determining: The MIC and MBC of manuka honey against selected organisms The bactericidal activity of manuka honey using time-to-kill curves assay The surface and intra-structural morphological changes of bacterial cells after treatment with manuka honey using scanning and transmission electron microscopy. the physiological effect of manuka honey against selected organisms using two-dimensional electrophoresis 2. To investigate the potential of Omani honeys for their use in wound care in Oman by: Characterizing the physical and chemical properties of selected Omani honey. Investigating the antimicrobial activity of Omani honey against MDR and ESBLs bacteria Investigating the antioxidant potential activity of selected Omani honey 69 Chapter 2 Materials & Methods 70 The materials used throughout this study are listed as chemicals and reagents (Table 2.1, 2.2 & 2.3), equipment and apparatus (Table 2.4 & 2.5), and MDR and ESBL clinical isolates (Table 2.3 and 2.4, respectively). Table 2.1: Media, Chemicals and Reagents used for general experiment in the project: Name of Chemical Suppliers Nutrient agar CM 0003 Oxoid Mueller-Hinton agar (MH) CM0337 Oxoid Eosin Methylene Blue agar (EMB) CM0069 Oxoid Iso-sensitest broth (ISB) CM 0473 Oxoid Tryptone Soya Broth (TSB) Oxoid Maximum recovery diluent (MRD) Oxoid Catalase 010M7010 Sigma-Aldrich Nutrient broth (NB) Oxoid Phenol Fisher Staph aureus – Oxford strain- NCTC 6571 Selectrol Bovine albumin serum (BSA) Sigma DPPH (2,2-Di(4-tert-octylphenyl)-1-picryl-hydrazyl) Sigma-Aldrich Free radical – 257621 71 Table 2.2: Chemicals and Reagents used for electron microscopy experiment in the project: Name of chemicals / reagents Suppliers Phosphate Buffered Saline (PBS) Oxoid Glutaraldehyde 3% Fluka-Sigma Osmium tetroxide 1% (OsO4) Agar scientific Ethanol Sigma-Aldrich Filter membrane (0.02mm pore size) Agar scientific Resin (no propylene oxide) Agar scientific Araldite resin CY212 Agar scientific DDSA Agar scientific BDMM/propylene oxide Agar scientific Uranyl acetate Sigma Reynolds lead citrate Sigma 72 Table 2.3: Chemicals and Reagents used for 2- dimensional electrophoresis experiment in the project Name of chemicals / reagents Suppliers DC protein assay reagent A - 8473 BioRad DC protein assay reagent B - 500-0114 BioRad 2,4,6-Tris(2-pyridyl)-s-triazine- T1253 Sigma-Aldrich Trizma®base (C4H11NO3) BCBC0475 Sigma-Aldrich Iodoacetamide (C2H4INO) 030M5300 Sigma-Aldrich MOPS (3-Morpholino-Propansulfonsaure acid – 69947 Fluka, Sigma-Aldrich DL-Dithiothreitol (C4H10O2S2) D9163 Sigma-Aldrich Trizma®hydrochloride (C4H11NO3) T3253 Sigma-Aldrich Sodium dodecylsulfate (C12H25NaO4S) L3771 Sigma-Aldrich CHAPS (C32H58N2O75) C9426 Sigma-Aldrich Simply Blue™ Safe stain LC6060 Invitrogen Ethylenediaminetetraacetic acid tetrasodium sodium Sigma-Aldrich salt dihydrate E6511 Glycerol G8773 Sigma-Aldrich Sodium chloride NaCl Fisher scientific Urea (CH4 N2O) 46504 Sigma-Aldrich Bromophenol Blue B0126 Sigma-Aldrich Agarose- low melting point A9414 Sigma-Aldrich 73 Table 2.4: Equipment used in general experiments in the project: Name of Materials Suppliers Automatic pipettes Eppendorf Volumetric flasks Volac-UK Conical flasks PYREX-UK Autoclave LTE scientific Micro-centrifuge Sanyo-MSE Weighing scale DP-300 Fisher brand Microtitre plate/96wells Nunc (flat bottomed) Fisher scientific Nuclon™ Surface Bioassay plate CORNING 43110 Multipoint inoculator MAST Spectrophotometer/Plate reader MRX Revelation, Dynex BBL Sens-Disc for ESBL BBL Oxoid Sens-Disc Oxoid Spectrophotometer JENWAY 6705UV Vis Disc dispenser Oxoid AmpC & ESBL ID set D68C MAST Diagnostic-UK Incubator 37 oC BINDER pH meter 3510 JENWAY Water refractometer Atago HHR-2N Sugar refractometer (40-85%) Bellingham & Stanley Water bath 37 oC/100 OLS200-Grant BioPak (Synergy UV) B0901 74 Table 2.5: Equipment used in electron microscopy and 2-dimentional electrophoresis experiments in the project: Name of materials Suppliers Critical point dryer (CPD) Balzers CPD-030 Gold sputter coater AE 1232 EM Scope UK Scanning electron microscopy (SEM) JEOL 5600V SEM- UK Transmission electron microscopy (TEM) Leica-Reichert- Jung UK & JEOL 1230 TEM- UK Ready strip™ 11cm pH 3-10 BioRad Protean IEF cell & Tank BioRad Refrigerated superspeed centrifuge Sorvell® RC-5B Thirty isolates of baumannii/calcoaceticus Acinetobacter complex that baumannii were resistant and to Acinetobacter third generation cephalosporins (3rd G cephalosporin) were kindly provided by the Department of Medical Microbiology in the University of Wales Hospital at Heath Park, Cardiff. Antibiotic sensitivities had already been evaluated in the hospital using antibiotic sensitivity discs for cefotaxime (CTX 30µg), ceftazidime (CAZ 30µg), ceftriaxone (CRO 30µg) & cefoxitin (FOX30µg). This information was provided with the isolates (Table 2.6). 75 Table 2.6: Thirty isolates of MDR Acinetobacter S. no. Identification of isolates 1. Acinetobacter baumannii /calcoaceticus complex 2. Acinetobacter baumannii/calcoaceticus complex 3. Acinetobacter baumannii 4. Acinetobacter baumannii 5. Acinetobacter baumannii 6. Acinetobacter baumannii/calcoaceticus complex 7. Acinetobacter baumannii/calcoaceticus complex 8. Acinetobacter baumannii/calcoaceticus complex 9. Acinetobacter baumannii/calcoaceticus complex 10. Acinetobacter baumannii/calcoaceticus complex 11. Acinetobacter baumannii 12. Acinetobacter baumannii/calcoaceticus complex 13. Acinetobacter baumannii 14. Acinetobacter baumannii 15. Acinetobacter baumannii/calcoaceticus complex 16. Acinetobacter baumannii/calcoaceticus complex 17. Acinetobacter baumannii/calcoaceticus complex 18. Acinetobacter baumannii 19. Acinetobacter baumannii 20. Acinetobacter baumannii 21. Acinetobacter baumannii 22. Acinetobacter baumannii 23. Acinetobacter baumannii 24. Acinetobacter baumannii 25. Acinetobacter baumannii 26. Acinetobacter baumannii 27. Acinetobacter baumannii 28. Acinetobacter baumannii 29. Acinetobacter baumannii 30. Acinetobacter baumannii 76 Fifty five clinical isolates belonging to the Enterobacteriaceae family that were resistant to third generation cephalosporins (3rd G cephalosporin) with their mechanisms of ESBL production by molecular method were also provided for this study (Table 2.7a & 2.7b). Isolates were stored at -80ºC on Protect beads until required. When needed, one bead was introduced into 10 ml nutrient broth and incubated overnight at 37oC. The broth culture was either used directly or streaked onto nutrient agar and incubated at 37ºC overnight. Table 2.7a: Clinical isolates of E.coli & Klebsiella provided for this study Identification of isolates Mechanisms 31. Escherichia coli CTX-M 32. Escherichia coli CTX-M 33. Escherichia coli CTX-M 34. Escherichia coli CTX-M 35. Escherichia coli CTX-M 36. Escherichia coli TEM 37. Escherichia coli TEM 38. Escherichia coli AMPC 39. Escherichia coli N.A 40. Escherichia coli N.A 41. Klebsiella pneumoniae SHV 42. Klebsiella pneumoniae CTX-M 43. Klebsiella pneumoniae CTX-M 44. Klebsiella pneumoniae CTX-M 45. Klebsiella oxytoca CTX-M 46. Klebsiella pneumoniae SHV 47. Klebsiella pneumoniae SHV 48. Klebsiella oxytoca SHV 49. Klebsiella pneumoniae Plasmidic ampC 50. Klebsiella oxytoca K1 51. Klebsiella pneumoniae N.A NA = not available 77 Table 2.7b: Clinical isolates of Citrobacter, Enterobacter & Serratia provided for this study Identification of isolates Mechanisms 52. Citrobacter farmeri CTX-M 53. Citrobacter farmeri Hyper ampC expression 54. Citrobacter farmeri Hyper ampC expression +CTX-M 55. Citrobacter farmeri Hyper ampC expression +TEM 56. Citrobacter farmeri Hyper ampC expression +CTX-M 57. Citrobacter farmeri Hyper ampC expression 58. Citrobacter farmeri Hyper ampC expression 59. Citrobacter farmeri Hyper ampC expression 60. Citrobacter farmeri Hyper ampC expression 61. Citrobacter farmeri Hyper ampC expression 62. Citrobacter farmeri Hyper ampC expression +TEM 63. Citrobacter farmeri Hyper ampC expression +CTX-M 64. Enterobacter cloacae CTX-M 65. Enterobacter cloacae CTX-M 66. Enterobacter cloacae CTX-M 67. Enterobacter cloacae CTX-M 68. Enterobacter hormaechi CTX-M 69. Enterobacter cloacae CTX-M 70. Enterobacter cloacae CTX-M 71. Enterobacter aerogenes AMPC 72. Enterobacter cloacae TEM 73. Enterobacter cloacae Hyper ampC expression 74. Enterobacter cloacae Hyper ampC expression 75. Enterobacter cloacae Hyper ampC expression 76. Enterobacter cloacae Hyper ampC expression 77. Enterobacter cloacae Hyper ampC expression 78. Serratia plymuthica CTX-M 79. Serratia marcescens Hyper ampC expression 80. Serratia marcescens Hyper ampC expression 81. Serratia marcescens Hyper ampC expression 82. Serratia marcescens Hyper ampC expression 83. Serratia marcescens Hyper ampC expression 84. Serratia marcescens Hyper ampC expression +SHV 85. Serratia marcescens Hyper ampC expression 78 2.1 Characterization of test organisms: 2.1.1 Confirmation of the identity of test organisms: To confirm the identity of these isolates, each culture was tested with API 20E (BioMerieux, Becton & Dickinson) according to the manufacturer‟s instructions. To verify that the kits gave reliable results, two known organisms (Escherichia coli NCTC 10410 and Klebsiella oxytoca NCTC 8167) were tested on each occasion. 2.1.2 Antibiotics sensitivities: Extended Spectrum Betalactamases test (ESBLs): Antibiotic sensitivity of the clinical isolates was also confirmed and the method used was that of Clinical and Laboratory Standard Institute (CLSI 2006). 2.1.2.1 Inoculum preparation: Three to four similar colonies were selected from a pure overnight nutrient agar plate culture and transferred with inoculation loop into 4-5 ml of nutrient broth and incubated at 37°C for 2-6 h. The inocula were standardized photometrically to obtain turbidity equivalent to the 0.5 McFarland standards. 2.1.2.2 Disc application: A sterile cotton wool swab was dipped into the standardised inocula and excess culture removed by pressing against the edge of the culture bottle. The entire agar surface of a Mueller Hinton plate was streaked in three directions to produce an even lawn plate. Then, the appropriate discs (Oxoid Sens-Disc) of carbapenem (imipenem 10µg and meropenem 10µg), third and fourth generation cephalosporins (cefotaxime CTX 30µg, ceftazidime CAZ 30µg and cefepime FEP 30µg) respectively, aminoglycosides (amikacin AK 30µg & gentamicin CN 10µg) and piperacillintazobactam TZP 100/10 µg were applied for all isolates by disc dispenser. 79 Appropriate discs (BD BBLTM Sens-Disc) of ceftazidime (CAZ 30µg), cefotaxime (CTX 30µg), ceftazidime with clavulanic acid (CAZ/CLA 30/10µg) and cefotaxime with clavulanic acid (CTX/CLA 30/10µg) were also dispensed for the 55 Enterobacteriaceae isolates. The plates were placed in the 37°C incubator within 15 minutes and incubated for 16-18 h. After incubation, the plates were examined and zone diameters were recorded. Antibiotic sensitivity was determined by reference to the (CLSI). 2.1.2.3 Screening test for ESBL: If the zones for each of CAZ 30µg ≤ 22mm, CTX 30µg ≤ 27mm and CRO 30µg ≤ 25mm, ESBL production was indicated. 2.1.2.4 Phenotypic confirmatory test for ESBL: A confirmatory test was required for each of ceftazidime and cefotaxime in combination with clavulanic acid. For comparison with zone sizes without clavulanic acid a ≥ 5 mm increase in zone diameter for either antimicrobial agent tested in combination with clavulanic acid versus its zone when tested alone confirmed an ESBL producer. A positive control (ESBL producer) of Escherichia coli ATCC 13353 and a negative control (non-ESBL producer) Escherichia coli NCTC 10418 were used for quality control of this method. 2.1.2.5 ESBL/AmpC* confirmation test: This test was used for the detection of AmpC and/or ESBL enzyme production. Four discs were applied: cefpodoxime (10 µg), cefpodoxime (10µg) with ESBL inhibitor, cefpodoxime (10µg) with AmpC inhibitor and cefpodoxime (10µg) with ESBL and AmpC inhibitor. The interpretation of results was determined using software product of ESBL/AmpC calculator (EAC) programme provided by MAST manufacturer. 80 2.2 Characterization of honey samples: 2.2.1 Honey sample collection: A medical grade honey (manukacare 18+), which was kindly provided by Comvita UK, was used throughout this study. Eight samples of raw and unprocessed Omani honey (labelled OH-B to OH-I) were collected from different regions of Oman (Table 2.8). The floral source was estimated by beekeepers. All samples were stored at 4°C in the dark until tested. Table 2.8: List of honeys used in this project: Batch Number Flora Source Country Regions A Manuka New Zealand - OH-B Multi-flora Oman Batina OH-C Honey dew Oman Dakhilyia OH-D Honey dew Oman Batina OH-E Honey dew Oman Dhahira OH-F Citrus Oman Sumail OH-G Honey dew Oman Batina OH-H Acacia Oman Sharqiya OH-I Market honey Oman Not known 2.2.2 Bioassay of antibacterial activity: The antibacterial activity of all honey samples was determined by the method described by Allen et al., (1991). 81 2.2.2.1 Phenol standards preparation for bioassay: 10% (w/v) of phenol (a reference antiseptic) (Fisher) was prepared by weighing 5 g of phenol made up to 50 ml with deionised water. This solution of phenol was used to prepare the standard solutions of 2%, 3%, 4%, 5%, 6% and 7% (Table 2.9).These standards were stored at 4oC till one month. Table 2.9: Preparation of phenol standards Final Phenol Conc (%w/v) Volume of 10% Volume of H2O/ml Phenol/ml 2% 2 8 3% 3 7 4% 4 6 5% 5 5 6% 6 4 7% 7 3 2.2.2.3 Inoculum preparation: One bead of a freeze dried culture of Staph.aureus NCTC 6571(Selectrol) was dispensed into 10 ml nutrient broth (Oxoid) using aseptic technique and incubated at 37oC for 18 h. Staph. aureus was universally used in antibiotic sensitivity testing. 2.2.2.4 Plate preparation: Nutrient agar (Oxoid) was prepared by weighing 3.45g of nutrient agar and dissolving in 150 ml of deionised water. The agar was mixed and sterilised by autoclaving at 120oC. After autoclaving, the agar was kept at 50oC in water bath for 30 minutes. While waiting for the agar, the nutrient broth with Staph. aureus (working culture) was adjusted to an absorbance of 0.5 measured at 540 nm in a Cecil spectrophotometer using sterile nutrient broth as a blank. 100 µl of working culture of Staph. aureus was added to the molten nutrient agar at 50oC. Then the agar was mixed thoroughly and 82 transfered into a large square assay plate (Corning 43110) on flat surface. When the agar had set, the plate was layed upside down at 4oC and left overnight. 2.2.2.5 Sample preparation: Eight universal containers were labelled as A1, B1, C1, D1, E1, F1, G1, H1 and I1 one for each of the eight types of Omani honey used in this project. Stock honey solution was prepared by adding 10g of well mixed honey to 10 ml of deionised water, therefore the final honey concentration was 50% w/v. The solution was then placed in a water bath at 37oC for 30 minutes to aid dissolving and mixing. To prepare further dilutions, another eight universal containers were labelled as A2, B2, C2, D2, E2, F2, G2, H2 and I2 and was transferred 1 ml of 50% honey (stock solution) to 1 ml of deionised water to make the final concentration of 25% honey. For non peroxide activity testing 0.02g of catalase from bovine liver (Sigma) was made up to 10 ml with deionised water. The solution was mixed gently. Then eight universal containers were labelled as A3, B3, C3, D3, E3, F3, G3, H3 and I3. 1 ml of 50% honey (stock honey) was transferred to these tubes aseptically and 1 ml of catalase solution was added to these tubes to make 25% (w/w) honey and catalase solution. 2.2.2.6 Samples and standards application: The bioassay plate was placed over a quasi-latin square as a template after it was removed from the cold room (4oC). A flamed, cooled 8 mm cork borer was used to cut out 64 wells of the agar. Cut agar was removed with a sterile blade into a discard pot. A 100 µl of each sample was added to each of 4 wells with the same number assigned on the assay plate. Thus, each sample was tested in quadruplicate. Similarly, 100 µl phenol standards (2%-7%) were tested in duplicate. The plate was then incubated at 37oC for 18 h. 83 2.2.2.7 Zone measurement: After incubation, the plate was placed back over black paper to measure the diameter of the zones of inhibition with digital calipers. Each zone of inhibition was measured twice (horizontal and vertical reading) at 90°angles. 2.2.2.8 Calculation of antibacterial activity of honey: After measurement of the clear zone around each phenol standard twice, the mean diameter was calculated and squared. A standard graph was plotted of % (w/v) phenol against the square of the mean diameter of the clear zone. A best straight line shape was plotted using Cricket graph software and the equation of this line was used to obtain the activity of each diluted honey sample. The diameter of the clear zone was measured and squared. However, the dilution factor is correlation to the density of honey thus this value was multiplied by a factor of 4.69. In short to obtain the dilution from 50% w/w solution of honey, 10 ml of water were added to 10 g of honey. Ten g of honey is actually equal to 7.41 ml where the average density of honey is 1.35 g/ml i.e. 10/1.35 = 7.41. Therefore, 50% honey solution should be made by adding 10 ml of water to 7.41 ml of honey which was actually equal to 42.56% (v/v) and 25% honey solution was equal to 21.28% (v/v). To obtain the phenol percentage equivalent of full strength honey it required to multiply by a factor of 4.69 i.e 100/21.28. Then the activity of honey obtained from the assay was expressed as the equivalent phenol concentration (% w/v) (Molan, personal communication). 84 2.2.3 Determination of pH: This method was derived from the method described by the International Honey Commission (Bogdanov, 2002). All honey samples were removed from the fridge and kept at 20°C for 24 hrs in an airconditioned laboratory prior to testing. A 50% (w/v) solution of honey was made by weighing 5g of honey and dissolved in ultrapure water (BioPak- B0901) to 10 ml. The solution was gently shaken until the honey sample had completely dissolved. A JENWAY instrument 3510 pH meter was calibrated at pH 4, 7 and 10 using reference buffers (Fisher). After calibration the probe was inserting into the diluted sample. Each sample was tested in triplicate. Between each sample the probe was rinsed under running water and dried. Before testing the next sample, the probe was then placed in deionised water. 2.2.4 Sugar and water content: This method was established from the method described by the International Honey Commission (Bogdanov 2002). Sugar and water content were determined using a Bellingham & Stanley 40-85% sugar refractometer and an Atago HHR-2N moisture refractometer. Sugar and moisture content are usually tested at 20°C. Each of the honey samples were allowed to set to 20°C for 24 hours before the testing started. The whole honey sample was mixed with a sterile spatula then a drop of honey was placed in the lens of each of the refractometers. To confirm an equal distribution of the sample over the lens with no air bubbles, the lids above the lens were carefully closed. To read the scale, the refractometers were held directed to the light and the spot of the line was recorded. The refractometers were cleaned with running water and dried with clean tissue between each sample. 85 2.2.5 Hydroxymethylfurfural (HMF) concentration: The method used was that of White & Rudji (1978). Into 50 ml volumetric flasks, five grams from each of the honey samples were weighed with a total of 25 ml of deionised water. Then 0.50 ml of Carrez solution I (15 g potassium ferrocyanide in 100 ml of water) was added to each flask and mixed well. After mixing, 0.50 ml of Carrez solution II (30 g zinc acetate in 100 ml of water) was added to each flask. The solutions were diluted to volume with water and filtered through Whatman filter paper, discarding the first 10 ml. Then 5 ml of the remaining filtrate were added to each of two test tubes (18 x 150 mm). 5 ml of water were added to the first tube labelled as sample, and 5 ml of 0.20% sodium bisulphite (breaks down HMF) were added into second tube lablled as blank. Then a vortex mixer was used to mix the solutions and the absorbance was read in a Cecil spectrophotometer at 284 and 336 nm. The HMF value was calculated using the following formula: HMF (mg/Kg honey) = (A284 - A336) x 14.97 x 5/weight of sample in g. 2.2.6 Protein content: This method was established from the DC Protein assay kit (BioRad) that is based on the Lowry method for the determination of protein content in honey (White and Rudji 1978). Cellulose dialysis tubing is a selective membrane which allows low molecular weight molecules such as sugar to pass through this membrane. However, protein molecules cannot cross the membrane and remain in the tubing because of the pore size of membrane is smaller than the size of protein. The diameter of the inflated tube was 16 mm and a cut off of 12 kDa MWCO. The tubing was cut into lengths of 30-33 cm and placed under running tap water to hydrate and open the tubing. Two knots were tied 86 once the tubing opened at one end and it was stored until required in a beaker of tap water. To prepare the honey solution for dialysis, 5 g of honey was dissolved with 10 ml of deionised water into a small beaker. Honey solution was poured into a section of the inflated tubing. To facilitate the transfer of the solution, the tubing was clipped to a funnel. Then total volume of 10 ml of water were used to rinse the beaker twice and washed out any residue. This water was transferred into the tubing. The air was expelled from the dialysis sac and two knots tied above the liquid. The tubing was inverted several times to ensure mixing of the solution. The dialysis sac was then kept in a beaker with running tap water for 16 h. After dialysis was completed, A Erlenymeyer flask (50 ml capacity) was weighed to 0.01 g and the weight recorded. A dialysis sac was removed from the beaker and held over a funnel directed into a flask. The lower end of the sac was cut with a blade, ensuring that the flow of solution released was lead into the funnel. The remaining residual liquid was removed from the tubing using fingers. To obtain the weight of the protein solution the flask was reweighed. Five µl of these solutions (protein) were distributed into the wells of a 96 well microtitre plate. Then 25 µl of reagent A (alkaline copper tartrate) were added to the wells. After that 200 µl of reagent B (dilute Folin reagent) were also added to the same wells. The plate was then incubated at room temperature for 15 minutes and read in a microtiter plate reader (DYNEX Revelation 4.21) at 620 nm. A calibration curve of the best fit line was obtained from the standard solutions of bovine serum albumin (Sigma) (Fig. 2.1). The concentration of proteins in the honey samples was determined from the equation of the calibration curve line. Each sample was repeated in triplicate. 87 Figure 2.1: Calibration curve for protein determination in honey samples 2.2.7 Colour: The colour of all honey samples was established using the optical density method recommended by the National Honey Board. The absorbance of a 50% (w/v) honey solution was determined at 560 nm in a Cecil spectrophotometer. To obtain the actual absorbance value of the undiluted solution, the absorbance was multiplied by 2. Honey were then categorised according to a Townsend classification system (1969). 2.2.8 Pollen analysis: This method was derived from that of Loveaux et al. (1978). Ten grams of honey were dissolved in 20 ml of deionised water and centrifuged in a Sanyo-MSE centrifuge at 2500 rpm (3.8 G) for 10 mins. Then the supernatant was decanted and re-suspended in 10 ml of deionised water. The solution was recentrifuged as above and the supernatant was decanted and discarded. The sediment 88 was re-suspended in 1 ml liquefied glycerine-gelatine, transferred to a glass slide using a Pasteur pipette and mounted with a cover slip. Using a light microscope at least 100 pollen grains in each sample were identified, examined and counted. The samples were classified according to the predominant pollen present in the sample (›45% pollen grains). Advice about the identity of the pollen grains was kindly provided by National Pollen And Research Unit (NPARU) at Worcester University. 2.2.9 Total phenolic content: This method was used that described by Berreta et al. (2005). 2.2.9.1 Reagent/standard preparation: A 10% (w/v) stock honey solution was prepared by weighing 0.5 g of each honey sample and diluted with 5ml of warm (45oC) deionised water, then mixed for 5 mins. A Folin-Ciocalteau reagent (1:10) was prepared by adding 10 ml of Folin reagent to 90 ml of deionised water. Gallic acid standards (10-250 µg/ml): A stock solution of 0.005 M gallic acid (Sigma) was prepared by weighing 0.017g of gallic acid and made up to 20 ml using water:methanol solution (1:1). A range of gallic acid standards (10-250 µg/ml) was prepared (Table 2. 10) 89 Table 2.10: Preparation of gallic acid standard solutions Working standard solution (µg/ml) Standard stock solution (µl) Deionised water: methanol (µl) 0 0 4000 10 47 3953 25 118 3882 50 235 3765 100 470 3530 150 705 3295 200 940 3060 250 1176 2824 Figure 2.2: Standard curve for total phenolic content in honey samples Standard curve for total phenolic content y = 0.0013x R² = 0.9974 0.4 Absorbance at 750nm 0.35 0.3 0.25 0.2 0.15 0.1 0.05 0 0 50 100 150 200 250 300 Concentration of gallic acid standard (ug/ml) 2.2.9.2 Assay method: 100 µl of 10% of each honey solution was added to 1 ml of Folin-phenol reagent (1:10) in a test tube. The mixture was mixed for 2 mins and incubated for 20 mins at room temperature. After incubation, the absorbance was read at 750 nm against reagent blank (100 ml of water:methanol) on a Cecil spectrophotometer. The 90 difference between this absorbance and the sample blank (honey solution with deionised water) was calculated to get the net absorbance. The solutions with gallic acid in the range of 10-250 µg/ml were used for calibration (standard graph). Total phenolic content was expressed as µmol of gallic acid eq/kg honey. Each honey sample was tested in duplicate and the average net absorbance was calculated (A). Determination for honey colour interference with the assay: Two honey solutions were made for each sample as follows: A: 1000 µl distilled water: methanol + 100 µl honey solution B: 1100 µl distilled water: methanol The honey colour (H) was calculated as the difference in absorbance between A and B at 750nm. Net absorbance (N) for each sample was calculated as follows: N = (A) – (H), and this value (N) was used to determine phenolic content from the calibration curve. The standard graph was plotted and phenolic content value for test was obtained from the standard graph. 2.2.10 Free radical activity of honey: This method was established from the method described by Chen et al. (2000) and Aljadi & Kamaruddish (2004). 2.2.10.1 Reagent / Standard Preparations DPPH (2,2-Di(4-tert-octylphenyl)-1-picryl-hydrazyl) 0.09 mg/ ml (Sigma) was prepared by weighing 0.009 g of DPPH and made up to 100 ml with methanol. Deionised water: methanol (1:1) was prepared by adding 5 ml of deionised water to 5 ml of methanol. 91 A 10 % (w/v) honey solution was made by weighing 5 g of honey and added to 5 ml of warmed deionised water. The solution then mixed for 5 minutes. 2.2.10.2 Assay procedure: To assay free radical activity 0.75 ml of each 10 % (w/v) honey solution was mixed with 1.5 ml of 0.09 mg/ml DPPH in methanol in a test tube. Mixture was then incubated at 25°C for 5 minutes. The absorbance was measured at 517 nm against a test blank (honey solution + 1.5 of deionised water:methanol). The absorbance of 1.5 ml of DPPH radical control was measured with 0.75 ml of distilled water: methanol against DPPH radical control blank (2.25 ml of distilled water: methanol). The anti radical activity (ARA) was expressed as a percentage inhibition of DPPH radical by honey and calculated as follows: Anti –radical Activity (ARA%)= {(A-B) / A} x 100 Where A= Average absorbance of DPPH radical without honey (DPPH control absorbance) and B = Average absorbance of DPPH radical with honey (Test absorbance). 2.3 Determination of antibacterial activity of honey samples against test cultures: 2.3.1 Minimum Inhibitory Concentration (MIC) method: 2.3.1.1 Agar incorporation method: 2.3.1.1.1 Honey selection: From the bioassay results, two honeys were selected according to their antibacterial activity: Manuka honey with non peroxide activity equivalent to 18.0% (w/v) phenol 92 and Omani honey (B) with hydrogen peroxide activity equivalent to 17.7% (w/v) phenol 2.3.1.1.2 Inoculum preparation: One to five colonies of test organism were inoculated into 10 ml nutrient broth and incubated at 37oC overnight. Subculture was performed for each isolate onto nutrient agar plates to confirm the purity. 2.3.1.1.3 Plates preparation: 300 ml of double strength nutrient agar was prepared by weighing 14.8 g of nutrient agar into 300 ml of deionised water. The mixture was mixed and boiled to dissolve the agar then it was kept in a water bath at 50oC for 15 minutes. An automatic pipette was used to dispense 10 ml of nutrient agar into each of 22 universal containers and autoclaved at 121oC for 15 minutes. After autoclaving, it was put in water bath at 50oC for 20 minutes. 2.3.1.1.4 Honey preparation: A stock honey solution of 40% (w/v) was prepared either by adding 20 g of manuka honey (A) to a volumetric flask, and making up to 50 ml with sterile deionised water, or by adding 12 g of honey (B) to a volumetric flask, and making up to 30 ml with sterile deionised water. Nutrient agar plates containing honey varying from 0 -10% (w/v) were prepared (Table 2.11). 93 Table 2.11: Preparation of varying concentration of honey solution from 40% (w/v) stock honey for MIC method % of honey Quantity of double Quantity of 40% Quantity of sterile (w/v) strength N.A (ml) stock honey (ml) water (ml) 0% 10 0 10.0 1% 10 0.5 9.5 2% 10 1.0 9 3% 10 1.5 8.5 4% 10 2 8 5% 10 2.5 7.5 6% 10 3 7 7% 10 3.5 6.5 8% 10 4 6 9% 10 4.5 5.5 10% 10 5 5 The plates were allowed to set at room temperature for 30 min and then placed in 37oC incubator to remove excess moisture. The plates of varying honey concentration were then inoculated with 1 µl of each test organism (typically 1x105 cfu/ml) in triplicate using multipoint inoculator. The plates were placed in an incubator at 37oC for 24 h to allow for growth. 2.3.1.1.5 Plates reading (MIC determination): After overnight incubation, the growth was recorded for each dilution. Positive growth was confluent growth within the inoculated area and negative growth was recorded when no colonies where present. The MIC was deduced as the lowest concentration of honey that inhibited growth, and the average for all assays on each test organism was calculated. 94 2.3.1.2 Broth dilution method: 2.3.1.2.1 Honey selection: Four honeys were selected according to their antibacterial activity: Manuka honey with non peroxide activity equivalent to 20.0% (w/v) phenol and Omani honeys B, C, G & F with hydrogen peroxide activity equivalent to 22.85, 21.8, 20.1 and 20.8 % (w/v) phenol respectively. 2.3.1.2.2 Honey dilution: 40% (w/v) stock solutions of honey were prepared as described above and solutions ranging from 6% to 15% honey diluted with iso-sensitest broth (ISB) were prepared as shown in (Table 2.12). Table 2.12: Preparation of tubes for MICs. Honey Conc. (%w/v) Quantity of 40% honey (ml) Quantity of ISB (ml) Final Volume (ml) 6 0.225 1.275 1.5 7 0.262 1.237 1.5 8 0.3 1.2 1.5 9 0.337 1.163 1.5 10 0.375 1.125 1.5 11 0.412 1.08 1.5 12 0.45 1.05 1.5 13 0.487 1.012 1.5 14 0.525 0.975 1.5 15 0.562 0.937 1.5 2.3.2.1.3 Microtitre plate inoculation: One 96 well microtitre plate was used for 3 test organisms and each organism was tested in duplicate. 200 µl of each honey solution was dispensed to wells in row (A) 95 for honey control, rows (B&C) for isolate 1, rows (D&E) for isolate 2 and rows (F&G) for isolate 3 in [columns 1-10]. 200 µl of ISB was dispensed to wells in rows (A – G) and columns (11&12) only. 1 µl of isolates 1, 2 & 3 was added to wells in rows B&C, D&E and F&G respectively in columns 1-11. After the wells have been inoculated the plate was incubated at 37°C for 24h. This procedure was repeated for all other isolates. 2.3.2.1.4 Visual inspection of MIC: Plates were removed from the incubator and inspected visually for growth. Growth was assessed by turbidity in the wells and comparing them to the negative control (ISB only). Wells showing turbidity were considered to contain growth and marked as positive. Wells showing no turbidity were assessed to have no growth and marked as negative. 2.3.2.1.5 Spectrophotometric determination of MIC: The microtitre plates were placed in a plate reader (DYNEX Revelation 4.21) and optical density was measured at 405 nm filter for test and 620 nm filter as reference. The printout of the reading were obtained and used to confirm the MIC. 2.3.2 Minimum Bactericidal concentration (MBC) method: Wells that appeared to have no growth (no turbidity) by visual inspection were streaked onto nutrient agar plates using sterile 10 µl plastic loops. The plates were incubated at 37°C for 24 h. After incubation any growth on the plates was marked as positive and no growth marked as negative. The plates with the lowest concentration of honey showing no growth was recorded as the MBC. 96 2.4 Time Kill Curve Assay: 2.4.1 Strain selection: One culture of each of the six types of bacterial strains was selected according to the highest MIC and the MIC was approximately doubled as shown in (Table 2.13) below: Table 2.13: Cultures and honey concentrations used in the time-kill curves Strain ID MIC (%w/v) Test conc. used Acinetobacter 15 9 20 E.coli 7 (2139) 13 30 Klebsiella 5 (3042) 13 30 Enterobacteria 9 (5865) 13 30 Citrobacter 2 (3031) 10 20 Serratia 4 (3036) 15 30 Manuka honey (Comvita) UMF 18 equivalent to 18 % (w/v) phenol was used in this assay. 2.4.2 Time-kill curve: An overnight broth culture of each test organism in 10 ml ISB was prepared by inoculating a colony from a pure culture and incubating at 37oC for 18 h. After incubation each culture was diluted with ISB to an optical density of 0.5 at 550 nm. 50 ml of sterile ISB was added to conical flask labelled as control for each isolate. A 50 ml of appropriate honey solution (approximately 2xMIC) was prepared in another conical flask and labelled as test for each isolate. Then 5 ml from the diluted overnight culture was transferred into each flask. The mixture was then incubated at 37°C in shaking water bath. One ml from each flask were removed into a microcuvette and absorbance was recorded at 550 nm every 30 mins for the first 2 h and every 1 hr until 4 h had passed. Finally, a graph of optical density versus time was plotted to allow the 97 exponential growth phase to be identified. Also, a total viable count for each collected specimen was determined as follows: 20 µl of the specimen was diluted in a decimal dilution series from 10-1 to 10-7 using maximum recovery diluent (Oxoid). For each dilution 3 x 20 µl aliquots were plated to the respectively labelled seven segments of a nutrient agar plate. Following this, the plates were left to dry before incubating for 24 h at 37°C. After incubation the colonies in different sections were counted and recorded and used to calculate the number of CFU/ml at each time point. Time-kill curves of total viable count versus time were plotted. A T-test was applied to establish the statistical difference between untreated cells and honey treated cells in the selected 6 species. 2.5 Effect of honey on bacterial structure: 2.5.1 Scanning Electron Microscopy (SEM): SEM is one of the multipurpose equipement that is used for the analysis and examination of ultrastructure features of solid object. It allows the observer to see entire specimen and larger part of an object (Williams and Carter 2009). 2.5.1.1 Bacterial Selection for SEM The same test organisms as selected for time-kill assays were used for morphological studies. 98 2.5.1.2 Preparation of cells in the exponential phase of growth: 1 ml of an overnight culture was inoculated into each of two flasks containing 50 ml of ISB. The flasks were labelled as either control (no honey) or test (with honey). The culture was incubated in a 37oC shaking water bath for 3 h when it was estimated that cells would be in the exponential phase of growth. Honey solution (Table 2.13) was then aseptically added into the flask labelled as test and the flasks continued to be incubated with shaking at 37oC. The point at which the honey was added to the test flasks was recorded as time 0. Absorbance was measured every 30 mins till 4 h had passed (0, 30, 60, 90, 120, 150 and 180 mins at 550 nm) and 4 ml was removed at each time point and distributed equally into 4 sterile eppendorff tubes. The tubes were centrifuged at 13,000 rpm (19.89 G) for 2 mins the supernatant was decanted and the pellet re-suspended in 250 µl of PBS. The contents from all tubes were combined into 1 ml tube, which was then centrifuged. The resulting pellet was re-suspended in 1 ml of PBS and centrifuged again. After removing the supernatant, the pellet was fixed with 750 µl of 3% glutaraldehyde for 1 h at 4oC. After fixation the cells were washed twice (2 x 2 mins) with 1 ml PBS. Washed cells were suspended in PBS were then stored on a shaker overnight at 4oC. At this point samples were transferred to Cardiff University for electron microscopy. 2.5.1.3 Preparation of cells for scanning electron microscopy: All samples were centrifuged at 13,000 rpm (19.89 G) for 2 mins. The resulting pellet was re-suspended in 0.5 ml of 1% osmium tetroxide in PBS for 1 h. After the post fixation, the cells were spun down as above and the osmium tetroxide solution was decanted. The cells in pellet were dehydrated in a graded series of ethanol concentrations as follows: 99 50%, 70%, 80% and 90% for 5 mins, 100% for 10 mins (twice). The samples were added to small plastic containers (labelled by cutting an identification number into it) that were fitted with 0.22 µm filter membrane attached to blotting paper to trap cells for critical point drying. A small volume of ethanol was added to the containers taking care not to let the sample completely dry. The dehydrated samples were dried for 16 h under a high pressure (100 bars) in a critical point dryer (CPD 030; Balzers, Lerchtenstein) using CO2. The dried samples were then mounted on metal stubs with carbon – double sided - sticky tape and coated with gold in sputter-coater (EMscope AE 1232, Kent, UK). Structural observations of cells size and shape were performed using a scanning electron microscopy (JEOL 5600V SEM-UK) operated at 20 kV accelerating voltage with magnifications ranging from 5000x to 10,000x magnification. More than 2000 cells for each isolate were observed and examined. The percentage of structural differences between untreated and treated cells was determined using SMile View programme-JEOL (Version 2). The results were analysed statistically for significance using the Mann-Witney test in Mini Tab Statistical package (version 15). 2.5.2 Transmission Electron Microscopy (TEM): TEM allow the observer to see the internal structure of an object with high magnification and greater degree (Williams and Carter 2009). 2.5.2.1 Bacterial Selection for TEM Two isolates were selected in this method. Acintobacter isolate no. 15 and E. coli isolate no.7 with 20% (w/v) and 30% (w/v) of manuka honey respectively. 100 2.5.2.2 Preparation of cells for transmission electron microscopy: Fixed cells with and without honey were prepared as described for scanning microscopy in section 2.5.1.2 and 2.5.1.3 up until dehydration was completed. When ethanol replacement was completed, pellets were released into a fresh 10 ml glass container of 100% ethanol with a cocktail stick. The pellet was allowed to stand 15 minutes in 100% ethanol and then transferred to fresh 100% ethanol for further 5 min. The pellet was transferred to 5 ml propylene oxide and left for 15 min. The pellet was transferred to 50:50 propylene oxide/araldite resin (5 g of araldite resin and 5 g of DDSA were preheated, mixed together and 0.15 g of BDMA/propylene oxide about 9 ml per sample and left overnight in the arbitrator. The infiltrated pellet were then transferred into 5 ml of fresh resin (no propylene oxide) and left for 12 hours into the arbitrator. After incubation, the pallets were transferred into moulds previously filled with full strength resin. The moulds were then incubated in the oven for 3 days at 60°C. 2.5.2.3 Pallet trimming and sectioning: The samples were trimmed in order to remove the excess resin around the samples and to expose the pellet of cells. Using glass knives and ultratome III ultra thin sections were cut and placed onto uncoated 3.00 mm copper grids. 2.5.2.4 Staining of thin sections A paraffin sheet was placed onto either a ceramic tile or Petri dish. A drop of 2% uranyl acetate solution was placed on the paraffin sheet. The grids were floated on the drop by placing the thin sections side faced down ward. The grids were covered and stained in a similar manner with Reynolds lead citrate for 5 minutes, then, washed twice in distilled water. The grids were dried with filter paper. 12 blocks containing 101 Acinetobacter test & control were prepared (3 blocks at each time point). The same was done also for E.coli. At least 8 grids from each sample were stained and examined. Eleven TEM micrographs were taken for each sample at each time point. Ten grids were captured by TEM under 16,000 x magnification and one under 32,000 x magnification using (TEM, Philips-PW60100, 10EM 208). A total of 400 cells for each sample were observed and examined for structural differences between honey treated cells and untreated cells, and the presence or absence of septa was recorded. 2.6 Effect of honey on bacterial proteins: The effect of exposure to 20% (w/v) manuka honey on proteins was tested in selected test organisms using 2-D gel electrophoresis. 2.6.1 Two Dimensional Gel Electrophoresis: 2.6.1.1 Buffers preparation: The following reagents were prepared (Table 2.14) 102 Table 2.14: Reagents and buffers used in 2-D Electrophoresis Re-hydration buffer Per 10 ml Urea 8 M 4.8 g CHAPS 2% w/v 0.2 g DDT 50 mM 0.08 g Biolyte ampholytes 0.2% w/v 0.05 ml Equilibration buffer 1 Per 10 ml Urea 6 M 3.6 g Tris-HCl, pH 8.8, 0.375M 0.592 g SDS 2% 0.2 g Glycerol 20% 2 ml DTT 2% w/v 0.2 g Equilibration buffer 2 Per 10 ml Urea 6 M 3.6 g Tris-HCl, pH 8.8, 0.375M 0.592 g SDS 2% 0.2 g Glycerol 20% 2 ml Iodoacetamide 2.5% w/v 0.252 g Overlay Agarose 0.04 g Bromophenol blue 100 ml water 1:20 of BPB in MOPS Add 0.12 ml of agarose MOPS running buffer Per 1000 ml MOPS 10.45 g Tris base 6.06 g SDS 1.00 g EDTA 0.30 g NaCl Per 100 ml 20% 20 g 103 2.6.1.2 Cell preparation: 10 ml of TSB (Oxoid) was inoculated with 2-4 pure colonies of Acinetobacter and incubated at 37oC for 18 h. 2 ml of overnight culture was added to 50 ml of ISB in a 500 ml flask and 2 ml was used to inoculate a second flask containing 50 ml ISB with 20% (w/v) manuka honey. The cultures were incubated at 37oC with shaking (100 rpm for 24 h). After incubation, either 50 ml of TSB or 50 ml containing 20% manuka honey was added to each respective culture and incubated for a further 3 h with shaking (100 rpm) to ensure that the cells were in the exponential phase of growth. Cells were harvested by centrifugation in a Sorvell centrifuge (10,000 rpm [15.3 G] for 6 min) and the cells were re-suspended in 10 ml deionised water, the OD of the resulting supernatant was recorded at 550 nm using water as a blank. The proteins were extracted by sonicating (Jencons, Sonics VCX 500) with 500 watts power, 20 kHz frequency and 30% amplitude for 2.5 min. In every 30 seconds each sample was tacked off to Eppendorff tube and kept on ice to cool and reduce air bubbles. The cells were spun down in a microfuge on top speed (13,000 G for 4 mins). Then, the supernatant was removed into sterile 1.5 ml Eppendorf tubes and stored at -20oC. A protein determination was performed for each extract as described above. 2.6.1.3 Protein determination of Acinetobacter extracts for each extract: Five µl of each sample to be analysed was dispensed into wells of a 96 well microtitre plate, then 25 µl of reagent A (alkaline copper tartrate) were added followed by 200 µl of reagent B (dilute Folin reagent). The plate was incubated at room temperature for 15 minutes and then read in a microtiter plate reader (DYNEX Revelation 4.21) at 620 nm. Suitable standard solutions (low standard 3mg/ml) of bovine serum albumin (Sigma) were used and calibration curve obtained, to which a best-fit line was added and the equation of this line was used to obtain the concentration of proteins in the 104 samples (Fig 2.3). Each sample was run in triplicate. The results from the protein assay (Table 2.15) were used to calculate the value needed to give 150 µg of protein in each sample for 2-D gel electrophoresis. Table 2.15: Quantity of proteins in Acinetobacter cells with and without 20% honey Protein sample of Acinetobacter Protein conc. (mg/ml) Volume of protein sample µl Volume of rehydration buffer µl Control cells (no honey) 4.55 32 168 Test cells (20% honey) 4.2 35.7 164.3 Figure 2.3: Calibration curve of protein concentration in Acinetobacter with and without 20% manuka honey. 105 2.6.1.4 Rehydration and sample application: The rehydration tray was prepared and protein samples were pipetted as a line along the edge of one of the rehydration channels, leaving 1 cm free at each end of the channel and ensuring that there were no bubbles. The cover sheet was peeled from the IPG strip using forceps. The strips were placed gel side down onto samples and ensure „‟+‟‟ and pH range are clear and legible with no bubbles. The lid was placed back onto the rehydration tray. Then the samples were kept for 60 min to be fully absorbed. Mineral oil was dripped carefully over the plastic back of the IPG strip to fully cover the strip. The rehydration tray was covered with the lid and left for 11-16 h (overnight) to allow rehydration/loading to be fully completed. 2.6.1.5 Rehydration in the PROTEAN® IEF Focusing Tray: A paper wick was placed over each of the electrodes using forceps, and 10 µl of deionised water (18 megohoms-cm) was pipetted on each wick. Using forceps, the IPG strip was removed from the rehydration channel and held vertically for 10 seconds to drain. The lower end of the strip was touched onto blotting paper. The IPG strip was transferred to the prepared channel ensuring the gel was facing down and the „‟+‟‟ sign is at the positive end of the tray. The IPG strip was covered with 2 ml of fresh mineral oil ensuring there are no bubbles. The lid was put on the tray and the tray was put in an iso-electric focusing cell. The IEF cell was programmed as per sheet provided (35000 volt for 24 h); this was suitable for 11 cm pH 3-10. After completion, the IPG strip was removed with forceps, and it was held vertically for 10 seconds to drain, the lower end was touched onto blotting paper to remove the excess of mineral oil. To ensure that all the oil was removed, the IPG strip was placed on dry filter paper gel side up and plotted gently with wet filter paper. To store the gels at this point, the IPG strip was transferred to a clean rehydration/equilibration tray (gel side up). The 106 tray was covered and wrapped in saran wrap and placed in a -70oC freezer. The gel was defrosted for not more than 15 min before SDS-PAGE separation, as proteins will migrate. 2.6.1.6 Equilibration and SDS-PAGE: 3 ml of equilibration buffer 1 (Table 2.14) was transferred to a lane in the rehydration tray then the IPG strip was slid into the buffer (gel side up), ensuring there were no bubbles. The lid was placed on the rehydration tray and put on an orbital shaker and shacked gently for 30 min at room temperature. The used buffer 1 was decanted from the squared end of the tray until the tray was vertical. 3 ml of equilibration buffer 2 was added to the strip and placed on an orbital shaker and shaken gently for 30 min at room temperature. The used buffer 2 was decanted from the squared end of the tray until the tray was vertical. The overlay agarose was made as mentioned above and melted by gentle heating. A measuring cylinder was filled with MOPS buffer. Any excess water from the SDS page gel was removed by pipetting and blotting gently. The IPG strip was removed from the rehydration tray and dipped briefly into the cylinder of running buffer. The IPG strip was placed gel facing forwarded onto the back plate of the 2-D gel and pushed down carefully with forceps so that it made contact with the gel. The IPG strip was covered with overlay agarose and allowed setting for 10 mins. The gel was mounted in the electrophoresis criterion cell, and the reservoirs were filled with 60 ml MOPS buffer and allowed for 55 min for the run to complete (200 volts). 2.6.1.7 Staining and gel visualising: The gel was placed in 100 ml ultrapure water and microwaved on full power for 1 min. The gel was shaken in an orbital shaker for 1 min, and then the water was discarded. The last two steps were repeated twice. 20-30 ml of simplyBlue™ safe stain 107 was added to the gel and microwaved on high power for 45 seconds to 1 min. The gel was placed on an orbital shaker and shaken gently for 5-10 mins before discarding the stain. 100 ml of ultrapure water was added to the gel and placed on an orbital shaker for 10 min, the water was discarded after use. 20 ml of 20% NaCl was added and the gel was placed back onto the orbital shaker for 5-10 mins. After staining, the gel was visualised using the UVP AutoChemi, gel system and analysed using PDQuest Basic 8.0 software. 2.7 Statistical analysis of the data: In time-kill assay the statistical difference in cell count of two variables (honey treatment and non honey treatment) in term of two factors (time and isolates) was applied using T-test. In SEM the percentage of structural differences (length of cells) between untreated and treated cells was determined using SMile View programme-JEOL (Version 2). The results were analysed statistically for significance using the Mann-Witney test in Mini Tab Statistical package (version 15). 108 Chapter 3 Results 109 3.1 Confirmations of the identity and antibiotics sensitivities of test organisms: Before the effects of honey on test organisms were investigated, the identity of each isolate was checked using BBL kits, and antibiotic susceptibilities were confirmed by antibiotic disc sensitivity tests. Results for Acinetobacter, Escherichia coli, Klebsiella, Citrobacter, Enterobacter and Serratia are presented in Tables 3.1, 3.2, 3.2, 3.4, 3.5 and 3.6 respectively. Identification and antibiotics sensitivities of thirty multi-drug resistant isolates of Acinetobacter baumannii and Acinetobacter baumannii/calcoaceticus complex provided from University of Wales Hospital (Table 3.1a & 3.1b) Identification and antibiotics sensitivity tests for the fifty six clinical isolates of extended spectrum beta-lactamases (ESBL) of Enterobacteriaceae with resistant to third generation cephalosporins (3rdG cephalosporin) that were provided from University of Wales Hospital did confirm that all cultures conformed to their assigned labels (Table 3.2 to 3.6) 110 Table 3.1a: Identification and antibiotics sensitivities of 15 MDR Acinetobacter isolates 1. Identification of isolates Resistance Pattern Acinetobacter baumannii CAZ, CTX, CE, CXM, CIP, AMP /calcoaceticus complex 2. CAZ, CTX, CXM, FOX, ERT, TAZ,AZT, AMP Acinetobacter baumannii /calcoaceticus complex 3. Acinetobacter baumannii CAZ, CTX, CXM, FOX, ERT,AZT, AMP 4. Acinetobacter baumannii CAZ, CTX, AK, CN, FOX, CXM, , AMP 5. Acinetobacter baumannii CAZ, CTX, FOX, CXM, ERT, AMP 6. Acinetobacter baumannii CAZ, CTX, FOX, CN, TAZ, ERT, CIP /calcoaceticus complex 7. CAZ, CTX, CN, FOX, TAZ, ERT, CIP, AMP Acinetobacter baumannii /calcoaceticus complex 8. CAZ, CTX, FOX, CXM, ERT, AZT, AMP Acinetobacter baumannii /calcoaceticus complex 9. CAZ, CTX, FOX, TAZ, ERT, AZT, AMP Acinetobacter baumannii /calcoaceticus complex 10. CAZ, CTX, CN, FOX, TAZ,ERT, CIP, AZT Acinetobacter baumannii /calcoaceticus complex 11. Acinetobacter baumannii CAZ, CTX, CN, FOX, TAZ, ERT, CIP, SXT 12. Acinetobacter baumannii CAZ, CTX, CN, FOX, TAZ, ERT, CIP, SXT /calcoaceticus complex 13. Acinetobacter baumannii CAZ, CTX, CN, FOX, TAZ, ERT, CIP, SXT 14. Acinetobacter baumannii CAZ, CTX, CN, FOX, TAZ, ERT, CIP, AZT 15. Acinetobacter baumannii CAZ, CTX, FOX, TAZ, ERT, CIP, AZT, CN 111 Table 3.1b: Identification and antibiotics sensitivities of 15 MDR Acinetobacter isolates 16. Identification of isolates Resistance Pattern Acinetobacter baumannii CAZ, CTX, CXM, FOX, TAZ, ERT, CIP, SXT, CN /calcoaceticus complex 17. Acinetobacter baumannii CAZ, CTX, CN, FOX, TAZ, ERT, CIP, SXT /calcoaceticus complex 18. Acinetobacter baumannii CAZ, CTX, FOX, TAZ, ERT, CN,CIP, SXT, AZT 19. Acinetobacter baumannii CAZ, CTX, FOX, CXM, ERT, AZT, AMP 20. Acinetobacter baumannii CAZ, CTX, FOX, CXM, AZT, ERT, AMP, SXT 21. Acinetobacter baumannii CAZ, CTX, FOX, CXM, AZT, ERT, AMP, SXT 22. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 23. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 24. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 25. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 26. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 27. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 28. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 29. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP 30. Acinetobacter baumannii CAZ, CTX, CRO, CE, CXM, AK, CN,CIP, AMP cefotaxime (CTX 30µg), ceftazidime (CAZ 30µg), cefoxitin (FOX 30µg), cefuroxime (CXM 30µg), gentamicin (CN 10µg), ciprofloxacin (CIP 5µg), ampicillin (AMP 10µg), ertapenem (ERT 10µg), aztreonam (AZT 10µg), tazobactam (TAZ 110µg), septrin (SXT 25µg), amikacin (AK 30µg). All isolates were sensitive to imipenem (IMP 10µg), meropenem (MEM 10µg) & colistin (CT10µg). 112 Table 3.2: Confirmation of identity and antibiotics sensitivity including ESBL tests for 10 E.coli isolates. Isolate No. Identification of isolates Resistance Pattern CAZ CTX CPM TZP ESBL test ESBL/ AmpC* test ESBL (+) - 1. Escherichia coli R R R S 2. Escherichia coli R R R S ESBL (+) - 3. Escherichia coli R R S S ESBL (+) - 4. Escherichia coli R R R R ESBL (+) - 5. Escherichia coli R R R R ESBL (+) ESBL 6. Escherichia coli R R S S ESBL (+) AmpC 7. Escherichia coli R R S R ESBL (+) ESBL 8. Escherichia coli R R S R ESBL (+) - 9. Escherichia coli R R S S ESBL (+) ESBL 10. Escherichia coli R R S S ESBL (+) ESBL R- Resistant, S - Sensitive All cephalosporin tested (CAZ, CTX & CPM) should be reported resistant if ESBL test positive. 113 Table 3.3: Confirmation of identity and antibiotics sensitivity including ESBL tests for 11 Klebsiella isolates Isolate No. Identification of isolates 1. Resistance Pattern ESBL test ESBL / Amp C* test CAZ CTX CPM TZP Klebsiella pneumoniae R R S S ESBL (+) - 2. Klebsiella pneumoniae R R S S ESBL (+) - 3. Klebsiella pneumoniae R R R R ESBL (+) ESBL 4. Klebsiella pneumoniae R R R R ESBL (+) - 5. Klebsiella oxytoca R R R R ESBL (+) - 6. Klebsiella pneumoniae R R S S ESBL (+) - 7. Klebsiella pneumoniae R R S S ESBL (+) ESBL 8. Klebsiella oxytoca R R S R ESBL (+) - 9. Klebsiella pneumoniae R R S R ESBL (+) ESBL 10. Klebsiella oxytoca R R S R ESBL (+) - 11. Klebsiella pneumoniae R R R S ESBL (+) - R- Resistant, S - Sensitive All cephalosporin tested (CAZ, CTX & CPM) should be reported resistant if ESBL test positive. 114 Table 3.4: Confirmation of identity and antibiotics sensitivity including ESBL tests for 12 Citrobacter isolates. Identification of isolates Resistance Pattern CAZ CTX CPM TZP ESBL test ESBL/ AmpC* test 1. Citrobacter farmeri R R S R ESBL (+) ESBL 2. Citrobacter farmeri R R S S ESBL (-) AmpC 3. Citrobacter farmeri R S S S ESBL (-) AmpC 4. Citrobacter farmeri R R S S ESBL (-) AmpC 5. Citrobacter farmeri R R S R ESBL (-) AmpC 6. Citrobacter farmeri R R S R ESBL (-) AmpC 7. Citrobacter farmeri R R S R ESBL (-) AmpC 8. Citrobacter farmeri R R S S ESBL (-) AmpC 9. Citrobacter farmeri R R S S ESBL (-) AmpC 10. Citrobacter farmeri R R S R ESBL (-) AmpC 11. Citrobacter farmeri R R S S ESBL (-) AmpC 12. Citrobacter farmeri R R S R ESBL (-) AmpC R- Resistant, S - Sensitive All cephalosporin tested (CAZ, CTX & CPM) should be reported resistant if ESBL test positive. 115 Table 3.5: Confirmation of identity and antibiotics sensitivity including ESBL tests for 15 Enterobacter isolates. Identification of isolates Resistance Pattern CAZ CTX CPM TZP ESBL test ESBL/ AmpC* test 1. Enterobacter cloacae R R S R ESBL (+) - 2. Enterobacter cloacae R R S R ESBL (+) ESBL 3. Enterobacter cloacae R R S R ESBL (+) - 4. Enterobacter cloacae R R S R ESBL (+) - 5. Enterobacter hormaechi R R S R ESBL (+) - 6. Enterobacter cloacae R R S R ESBL (+) - 7. Enterobacter cloacae R R S R ESBL (+) ESBL & AmpC 8. Enterobacter aerogenes R R S R ESBL (+) - 9. Enterobacter cloacae R R S R ESBL (+) AmpC 10. Enterobacter cloacae R R S R ESBL (-) AmpC 11. Enterobacter cloacae R R S R ESBL (-) AmpC 12. Enterobacter cloacae R R S R ESBL (-) AmpC 13. Enterobacter cloacae R R S R ESBL (+) AmpC 14. Enterobacter cloacae R R S R ESBL (+) AmpC 15. Enterobacter cloacae R R S R ESBL (+) AmpC R- Resistant, S – Sensitive All cephalosporin tested (CAZ, CTX & CPM) should be reported resistant if ESBL test positive. 116 Table 3.6: Confirmation of identity and antibiotics sensitivity including ESBL tests for 8 Serratia isolates. Identification of isolates Resistance Pattern CAZ CTX CPM TZP ESBL test ESBL/ AmpC* test 1. Serratia plymuthica R R S R ESBL (+) ESBL 2. Serratia marcescens R R S R ESBL (-) AmpC 3. Serratia marcescens R R S R ESBL (-) AmpC 4. Serratia marcescens R R S R ESBL (-) AmpC 5. Serratia marcescens R R S R ESBL (-) AmpC 6. Serratia marcescens R R S R ESBL (-) AmpC 7. Serratia marcescens R R S R ESBL (+) AmpC 8. Serratia marcescens R R S R ESBL (-) AmpC R- Resistant, S – Sensitive All cephalosporin tested (CAZ, CTX & CPM) should be reported resistant if ESBL test positive. ESBL/AmpC* confirmation test was used for the negative ESBL double-disk test. cefotaxime (CTX 30µg), ceftazidime (CAZ 30µg), cefepem (FEP 30µg). All isolates (MDR and ESBLs) were sensitive to imipenem (IMP 10µg) and meropenem (MEM 10µg). The identity of these isolates was confirmed using API 20E identification kit. 117 3.2 Characterization of honey samples: 3.2.1 Determination of antibacterial activity: The antibacterial activity of honey samples was determined by the method of Allen et al (1991). Essentially in this bioassay a reference strain of Staphylococcus aureus (NCTC 6571) was seeded into agar, and the extent of inhibition induced by honey samples were compared to that induced by phenol. An example of an incubated plate is given in Fig 3.1. Figure 3.1: A typical honey bioassay plate. Zones of inhibition 118 The diameter of the zones of inhibition of the phenol standards were measured (horizontal and vertical) and plotted against the phenol concentration. A linear relationship between honey concentration and the diameter of the zone of inhibition was determined and the equation (Fig 3.2) was used to calculate the potency relating to phenol of the honey samples. Three bioassay plates were used in total, with the manuka honey sample included on each plate for consistency. Each Omani honey sample was tested in quadruplicate on a plate. Good agreement was found between the three bioassay plates (R2=0.9482, 0.9657 & 0.9743 respectively) Honey samples were diluted with and without catalase to determine whether the zones of inhibition were due to the generation of hydrogen peroxide or not. Hence, total activity was determined when the honey sample was diluted in deionised water, and non-peroxide activity was calculated when the honey was diluted with catalase (Table 3.7). 119 Figure 3.2: A typical calibration curve of the bioassay. Phenol Standard Curve y = 2.1643x + 5.3857 R² = 0.9719 Mean Diameter (mm) 25 20 15 10 5 0 0 1 2 3 4 % (W/V) Phenol The data obtained from this method was repeated twice 120 5 6 7 8 Table 3.7: Antibacterial activity of honey samples Type of honey Total activity phenol Non- peroxide activity equivalent %w/v phenol equivalent % w/v Manuka honey-(plate1) 20.4 20.6 Manuka honey-(plate2) 22.1 20.2 Manuka honey-(plate3) 21.3 19.3 Mean ± SD(n) 21.3± 0.9 (3) OH-B (plate1) 21.5 3.7 OH-B (plate2) 24.2 <2* Mean ± SD(n) 22.9± 1.9 (2) - OH-C 21.8 3.7 OH-D 3.7 3.7 OH-E 13.3 < 2* OH-F 20.8 < 2* OH-G 20.1 < 2* OH-H 10.1 < 2* OH-I < 2* < 2* 20.0± 0.8 (3) *No zone of inhibition was detected of the bioassay. The antibacterial activity of the eight Omani honey samples used in this study varied from < 2% to 22.9% (w/v) phenol equivalent, if the values obtained on plates 1 and 2 are averaged. The medical grade manuka honey sample used here was included in each bioassay plate and demonstrated a non-peroxide honey with 20.0±0.8 (%w/v) phenol equivalent, unlike the Omani honey samples. Seven of the eight Omani honey samples exhibited peroxide activity, but none had marked non-peroxide activity. Every Omani honey was tested in quadruplicate in each bioassay plate and OH-B 121 was tested on 2 plates. Omani honeys B & C demonstrated the highest total activity of (22.9% & 21.8% (w/v) phenol equivalent) respectively. Omani honeys (F & G) have almost same activity. There was no activity detected in Omani honey I. 3.2.2 Chemical & physical analysis of honey samples As well as antibacterial activity, honeys were analysed for their chemical and physical characteristics. All Omani honey samples were tested for their pH, water, sugar content, protein content, HMF level, colour, pollen and anti-oxidant activity these were compred to reference manuka honey (Tables 3.8, 3.9 & 3.10). pH was tested in triplicate using 50% (w/v) honey solutions and the mean was recorded. The pH was ranged between 3.5 to 6.27 with mean of 4.76 ±0.93. This indicates that all honeys fall within acidic range that able to inhibits the growth of most microorganisms. Sugar and water content were tested using refractometer. Mean sugar was 81%±2.86 with range between 75% and 85%. While mean water content was 15.8% ± 1.9 with range between 12.5% and 19.5%. Again low water and high sugar make the survival of bacteria are imposible. HMF test was used to determine the quality and history of honey or if it was subjected to heat treatment while processing (Sanz et al., 2003). An elevated level of HMF was expected in the Omani honeys due to the hot climate in Oman; nevertheless HMF level was not unduly elevated (Table 3.8). The mean range was 11.1±11.9 with a range between 2.9 and 38.5 mg/kg. Conversely the mean protein level was quite high (4.7±1.5 mg/g) (Table 3.8) compared to values previously established (White & Rudyj 1978). The colour of each honey sample was primarily visually inspected and then the optical density of 50% (w/v) from each sample was read at 560 nm and worked out according to the Townsend‟s classification (Townsend, 1969). The results were completely matched 122 with visual estimation. The colour of Omani honeys was ranged between extra light amber and dark amber (Table 3.8). The darker honey the highest antibacterial activity presents (Molan 1992). All parameters indicated that all honeys fell within the ranges normally expected for pH, sugar, water content, protein and HMF from National Honey Broad (NHB) (Table 3.8). Table 3.8: Chemical & physical analysis of different types of Omani honey compared to manuka honey Honey Sample pH Water content %(w/v) Sugar content % (w/v) Protein (mg/g) HMF (mg/kg) Colour OH-B 4.6 15.1 82 5.8 5.7 Amber OH-C 4.3 16 81 5.2 3.5 Amber OH-D 4.7 15.1 82.5 2.6 7.1 Light amber OH-E 3.9 15.3 82 6.2 2.9 Dark amber OH-F 4.6 12.5 85 6.3 10.4 Dark amber OH-G 6.2 17 80.5 2.6 38.5 Extra light amber OH-H 3.5 15.8 80 5.8 4.2 Dark amber OH-I 5.9 19.5 75 3.5 16.7 Extra light amber Range 3.5-6.2 12.519.5 75-85 2.6-6.3 2.9-38.5 Extra light amber to Dark amber Mean ± 4.7± 15.8± 81.0± 4.7± 11.1± - SD (n) 0.9(8) 1.9(8) 2.9(8) 1.6(8) 11.9(8) Manuka honey 3.5 20 78 10 3 123 Light amber 3.2.2.1 Pollen analysis Floral sources reported by beekeepers did not completely match to confirmed identities provided by the National Pollen And Research Unit (NPARU) at Worcester university (Table 3.9). Images from each honey samples were taken and the grains were classified according to the predominant pollen (›45% pollen grains) (Fig 3.3) Table 3.9: Represent the identification of flora sources by pollen analysis Honey Beekeepers National Pollen And Research Unit (NPARU) Sample Identification Identification OH-B Multi-flora Graminae (the grasses), Acacia (thorn trees, part of mimosoideae family) Asteraceae (daisy/sunflower family), Balsam (scented trees and shrubs), Tilia (lime) OH-C Honey dew Calendula arvensis (marigold), Graminae, Mimosa (subfamily of legume family), Myrtacae Eucalpyus, rosaceae (rose) Graminae was very high OH-D Honey dew little pollen was found on the slide OH-E Honey dew Myrtacae eucalyptus, Asteraceae inc. Bellis (daisy) and Ambrosia (ragweed) Fabaceae legume family) – specific to this slide Brassica (cabbage /mustard /rape) OH-F Citrus High proportions of Brassica types, Mimosa and Allium OH-G Honey dew little pollen was found on the slide OH-H Acacia High proportion of Acacia, Brassica and Ambrosia OH-I Honey dew little pollen was found on the slide 124 Figure 3.3: Image of pollen present in Omani honey samples at 100x magnification. OH-B Lime Graminae Acacia OH-C Marigold Graminae Rose OH-D Not Known OH-E Eucalyptus Daisy Brassica OH-F Brassica Mimosa Allium OH-H Acacia 125 3.2.2.2 Antioxidant activity assay: All honey samples were analysed for antioxidant activity which included total phenolic content and anti- radical activity (Table 3.10). The indication of linearity of the calibration curve (R2= 0.997) was evident between 0 and 250 µg/ml of gallic acid (Fig 2.2). From that equation total phenolic content was calculated for each honey sample equivalent to gallic acid. A positive correlation between the antioxidant and phenol content was found (Table 3.10) which suggests that a higher amount of phenolic content present in honey can deactivate free radicals and thus provide protection against diseases. Also differences in phenolic content between honeys were observed marked with a mean of 89.7±64.8. OH-H which contain high proportaion of acacia pollen and exhibit dark colour had the highest phenolic content approaching 244.6 mg gallic acid /Kg of honey and approximately same antioxidant activity as manuka honey. The least phenolic content and antioxidant activity was observed in OH-I with 46.1eg/kg and 59.5% respectively. This is because the antioxidant activity of honey varies and depends mainly on floral source, climate and environment conditions. Table 3.10: Amount of free radical and phenolic content in each honey samples Honey sample Anti- radical activity % Phenol content (eq/kg) OH-B 67.3 73.0 OH-C 68.1 80.7 OH-D 61.8 56.9 OH-E 64.7 63.0 OH-F 71.7 99.2 OH-G 62.6 53.8 OH-H 61.4 244.6 OH-I 59.5 46.1 Mean ±SD (n) 64.6±4.1 89.7±64.8 Manuka honey 61.1 65.4 126 3.3 Determination of antibacterial activity of honey samples against test cultures: 3.3.1 Minimum Inhibitory Concentration (MIC) and Minimum Bactericidal Concentration (MBC) of manuka honey: Using sterile manuka MIC and MBC was determined for all of the clinical isolates. Initially MICs were performed by agar incorporation (Table 3.11), but the method was found to require large amounts of honey, it was time consuming and MBCs could not be determined. A broth dilution method was therefore adopted. 3.3.1.1 Agar incorporation method: In this assay, two honeys were selected according to initial bioassay results (Table 3.7). These were manuka honey and Omani honey-B. However, because Omani honey did not give clear results and required too large an amount of honey to reach the correct MIC, only manuka honey was tested here against 10 Acinetobacter clinical isolates (Table 3.11). 127 Table 3.11: Susceptibility of Acinetobacter isolates against manuka honey Isolates MIC % (w/v) E.coli NCTC 10418 5 5 5 Mean MIC% (w/v) 5 K. oxytoca NCTC 8167 9 9 9 9 0 Acinetobacter 1 7 7 7 7 0 Acinetobacter 2 7 8 8 7.6 0.57 Acinetobacter 3 7 7 7 7 0 Acinetobacter 4 6 6 6 6 0 Acinetobacter 5 8 8 8 8 0 Acinetobacter 6 7 7 8 7.3 0.57 Acinetobacter 7 7 7 7 7 0 Acinetobacter 8 7 7 7 7 0 Acinetobacter 9 7 7 8 7.3 0.57 Acinetobacter 10 7 7 9 7.6 1.15 7.18 0.28 Mean of Means MIC SD *(n) 0 *(n) number of isolates tested, this expirement was done in triplicate The MICs of 10 Acinetobacter isolates ranged between 6% (w/v) and 8% (w/v) manuka honey. This indicates a medium variation of 2% (w/v) and standard deviations showed good reproducibility. Clinical isolate four had the lowest MIC at 6% (w/v), whereas the highest MIC was for clinical isolate five at 8% (w/v). The mode MIC was 7% (w/v) with four isolates inhibited at this concentration. The overall mean average of MIC was 7.18 ± 0.28 % (w/v) manuka honey. 128 3.3.1.2 Broth dilution method: The minimum inhibitory concentration (MIC) and Minimum Bactericidal Concentration (MBC) for all MDR & ESBL clinical isolates against manuka can be seen in Tables 3.12 to 3.16. A microtitre plate assay was preferred to the agar incorporation method because of the small quantity of honey used and the ability to perform replicate assays in the same plate. Besides that, MBC values could be easily found by sub-culturing from non turbid wells onto nutrient agar plates. Also, examining MIC/MBC ratios obtained by broth dilutions can be used as an indicator of mode of inhibition (bacteriostatic or bactericidal). The antimicrobial agent considered to have a bactericidal action is when MIC/MBC ratio < 4 while the bacteriostatic action is when this ratio become >4 (Levison 2004). From all MIC/MBC observations (Table 3.12 to 3.16), manuka honey was considered to have a bactericidal mode of action. The mean MIC and MBC and standard deviation for 30 MDR stains of Acinetobacter data derived from triplicate experiments were illustrated (Table 3.12) 129 Table 3.12: Sensitivity of 30 Acinetobacter isolates treated with manuka honey by broth dilution method Isolates No. Mean MIC Mean MBC %(w/v) %(w/v) ±SD(3) ±SD (3) 1. 7 ±1 7 ±1.7 2. 7.3 ±1.5 3. Isolates No. Mean MIC Mean MBC %(w/v) %(w/v) ± SD(3) ±SD (3) 16. 6 ±0 7 ±1 8 ±1.7 17. 6 ±0 7 ±0 7 ±1 8 ±1.7 18. 8 ±1 9 ±1 4. 6 ±0 10 ±1 19. 7 ±2.6 9 ±1.7 5. 8 ±1 10 ±0 20. 8 ±2 10 ±1.7 6. 7.5 ±1.5 9 ±1 21. 7 ±1.7 10 ±2 7. 7 ±1 9 ±1 22. 7 ±1 7 ±1 8. 7 ±0 10 ±0 23. 7 ±1 9 ±0 9. 8 ±1 9 ±0 24. 7 ±1 8 ±1 10. 8 ±0 11 ±0 25. 7 ±0 10 ±0 11. 7 ±1 10 ±1 26. 7 ±1.7 11 ±0 12. 8 ±1 10 ±0 27. 6 ±1 10 ±1 13. 7 ±0 9 ±1.7 28. 7 ±0 10 ±0 14. 6 ±1 7 ±1 29. 8 ±1 10 ±1 15. * 9 ±1.7 11 ±1 30. 8 ±0 11 ±0 Mean MIC ± SD (n) 7.17 ± 0.7 (30) Mean MBC ± SD (n) 9.2 ± 1.3 (30) (*)The least susceptible strain to manuka honey (n) number of isolates tested, this expirement was done in triplicate 130 The MIC range of 30 Acinetobacter isolates was between 6% (w/v) and 9% (w/v) manuka honey and the MBC range was between 7% (w/v) and 11% (w/v) (Table 3.12). Considering that MICs are normally performed by doubling dilutions, these differences are not large. Five clinical isolates (4, 14, 16, 17 & 27) have the lowest MIC at 6% (w/v), whereas the lowest MBC at 7% (w/v) was also found in five clinical isolates (1, 14, 16, 17 & 22). Hence isolates 14, 16 and 17 were the most susceptible cultures to manuka honey. However, the highest MIC and, MBC was observed in clinical isolate fifteen (15*) at 9% (w/v) and 11% (w/v) respectively (Table 3.12). The difference between MIC and MBC was < 4 for all isolates which means Acinetobacter exhibited bactericidal mode of inhibition with manuka honey. The mode MIC was 7% (w/v) with almost half of isolates inhibited at this concentration and the mode MBC was 10% (w/v) with eleven isolates killed at this concentration. The overall mean average of MIC and MBC were 7.17±0.7 (%w/v) and 9.2± 1.3 (%w/v) respectively (Table 3.12). This finding correlates with the study published by Blair et al., (2009) who reported the MIC of Acinetobacter with 8.1±1.5 (%w/v) using Medihoney. In addition similar potency against Acinetobacter (6-8 %v/v) has been reported by George & Cutting 2007. The inhibition of 10 ESBLs Klebsiella isolates were also determined with manuka honey and the mean MIC, MBC values were derived from duplicate expirements with standard deviation (SD) obtained (Table 3.13) 131 Table 3.13: Sensitivity of 10 Klebsiella isolates to manuka honey tested by the broth dilution method Klebsiella Isolate Mean MIC Mean MBC %(w/v) ±SD(2) %(w/v) ±SD(2) Kleb-1 12 ±0 12 ±0 Kleb-2 8 ±1.4 Kleb-3 Klebsiella Isolate Mean MIC Mean MBC %(w/v) ±SD(2) %(w/v) ±SD(2) Kleb-7 12 ±1.4 15 ±1.4 10 ±0 Kleb-8 12 ±2.8 12 ±2.8 12 ±1.4 13 ±1.4 Kleb-9 12 ±0 13 ±0 Kleb-4 12 ±0 13 ±1.4 Kleb-10 12 ±0 12 ±1.4 Kleb-5* 13 ±0 16 ±0 Kleb-6 12 ±0 13 ±0 Mean ± SD (n) 11.7± 1.3 (10) 12.9± 1.7 (10) (*) The least susceptible isolate (n) number of isolates tested, this expirement was repeated twice. The MICs of 10 Klebsiella isolates were found to range between 8% & 13% (w/v) manuka honey and between 10% & 16% (w/v) for MBC (Table 3.13). Although these values extended over a slightly wider range than the values obtained with Acinetobacter isolates, the variation was not large. Clinical isolate two demonstrated the lowest MIC where 8% (w/v) manuka honey were required to inhibit this bacterium and the highest MIC and MBC values were found in clinical isolate five at 13% (w/v) and 16% (w/v), respectively in the Klebsiella cohort. The mode MIC was 12% (w/v) manuka honey with eight isolates inhibited at this concentration and the mode MBC was 13% (w/v) with four isolates killed at this concentration. The MIC/MBC ratio was less than 4 for all Klebsiella isolates tested which proved the bactericidal mode of manuka honey on this species. The overall mean average of MIC and MBC were 11.7±1.3 & 12.9±1.7 (%w/v) respectively which also fairly correlate with Blair et al., (2009) finding with MIC of Klebsiella 13±2.4 (%w/v). 132 Mean MIC and MBC (%w/v) values of manuka honey were determined for eight ESBLs strains of Serratia and E.coli and the standard deviations (SD) were calculated from duplicate expirements (Table 3.14) Table 3.14: Sensitivity of 8 Serratia and 8 E.coli isolates to manuka honey using a broth dilution method SERRATIA ISOLATES Mean MIC %(w/v) ±SD(2) Mean MBC %(w/v) Serratia-1 10 ±0 12 ±0 Serratia -2 15 ±0 Serratia -3 E.COLI ISOLATES Mean MIC %(w/v) Mean MBC %(w/v) ±SD(2) ±SD(2) E.coli-1 10 ±1.4 12 ±1.4 18 ±0 E.coli-2 10 ±0 10 ±1.4 13 ±1.4 22 ±1.4 E.coli-3 10 ±0 10 ±0 Serratia -4* 15 ±1.4 20 ±0 E.coli -4 10 ±0 10 ±0 Serratia -5 15 ±0 16 ±0 E.coli -5 10 ±0 12 ±0 Serratia -6 14 ±0 16 ±0 E.coli -6 12 ±0 12 ±0 Serratia -7 13 ±0 14 ±0 E.coli -7* 13 ±0 13 ±0 Serratia -8 14 ±0 18 ±1.4 E.coli -8 8 ±0 8 ±0 Mean ± SD (n) 13.3 ± 1.7 (8) 17 ± 3.2 (8) Mean ± SD (n) 10.4 ± 1.5 (8) 10.9 ± 1.6 (8) ±SD(2) (*) Least susceptible isolates (n) number of isolates tested, this expirement was repeated twice The MIC values of 8 Serratia isolates ranged between 10% & 15% (w/v) and MBCs were between 12% & 22% (w/v) for manuka honey. Although there were large variations in the MIC and MBC ranges noted, manuka honey still demonstrated bactericidal action (Table 3.14). Concentrations of 13.3 ± 1.7 % (w/v) were required to inhibit test isolate. Serratia was considered to be the least susceptible isolates against manuka honey among the other species tested. Susceptibility of the E. coli isolates tested was similar to that of Klebsiella with MICs against manuka honey varying between 8% & 13% (w/v) (Table 3.14). The bactericidal action of honey also observed on E.coli where the MIC/MBC ratio was 133 very close (2 or less). It indicates that E.coli was inhibited and killed at the same concentration. There are several reports documenting the sensitivity of different honeys including manuka honey against E.coli (Blair et al., 2009; George & Cutting 2007; Tan et al., 2009; Sherlock et al., 2010). Some of them have an almost similar MIC value that was determined in this project with 10 % (w/v) (Lusby et al., 2005). Unlike E.coli, limited studies documented the sensitivity of honey against Serratia. 134 Table 3.15: Susceptibility of 15 Enterobacter isolates to manuka honey determined by broth dilution method and the SD were determined from the duplicate expirements. Mean MIC Mean MBC Mean MIC Mean MBC %(w/v) ±SD(2) %(w/v) ±SD(2) %(w/v) ±SD(2) %(w/v) ±SD(2) Enterobacter-1 9 ±0 15 ±1.4 Enterobacter-9* 13 ±0 14 ±0 Enterobacter-2 9 ±0 13 ±0 Enterobacter-10 11 ±0 14 ±0 Enterobacter-3 9 ±0 13 ±0 Enterobacter-11 11 ±0 14 ±0 Enterobacter-4 13 ±0 14 ±0 Enterobacter-12 8 ±1.4 12 ±0 Enterobacter-5 11 ±0 14 ±0 Enterobacter-13 11 ±0 14 ±0 Enterobacter-6 9 ±0 11 ±1.4 Enterobacter-14 12 ±0 13 ±0 Enterobacter-7 8 ±0 12 ±0 Enterobacter-15 10 ±0 13 ±0 Enterobacter-8 8 ±0 11 ±0 Mean ± SD (n) 10.1± 1.7 (15) 13.1± 1.2 (15) ISOLATES ISOLATES (*) least susceptible isolate (n) number of isolates tested, this expirement was repeated twice The MICs of 15 Enterobacter isolates ranged between 8% & 13% (w/v) manuka honey and MBCs were between 11% & 14% (w/v) (Table 3.15). The mode MIC & MBC was 9% & 14% respectively. The sensitivity of Enterobacter was similar to that of E.coli. The closest MIC, MBC ranges indicates the bactericidal mode of manuka honey. These results were corresponded with a previous report (Lusby et al., 2005), where the inhibitory concentration of Enterobacter was 10% (w/v). However, this contrast with Tan et al., (2009) finding where manuka honey also used at concentration of 20% (w/v) compared to our finding with 10.1± 1.7 (%w/v). 135 Table 3.16: Susceptibility of 12 Citrobacter isolates to manuka honey using broth dilution method and the SD were determined from the duplicate expirements. ISOLATES Mean MIC Mean MBC ISOLATES Mean MIC Mean MBC %(w/v) %(w/v) %(w/v) %(w/v) ±SD(2) ±SD(2) ±SD(2) ±SD(2) Citrobacter 1 9 ±0 12 ±0 Citrobacter 8 9 ±0 11 ±1.4 Citrobacter 2 10 ±1.4 15 ±0 Citrobacter 9 10 ±0 13 ±0 Citrobacter 3 10 ±0 14 ±0 Citrobacter 10 10 ±0 15 ±0 Citrobacter 4 10 ±0 15 ±0 Citrobacter 11 8 ±1.4 11 ±0 Citrobacter 5* 11 ±0 15 ±0 Citrobacter12 10 ±0 14 ±0 Citrobacter 6 10 ±0 14 ±0 Mean ± SD (n) 9.7± 0.8 (12) 13.3± 1.7 (12) Citrobacter 7 9 ±1.4 11 ±0 (*) least honey-susceptible isolate. (n) number of isolates tested, this expirement was repeated twice The inhibition ranges of 12 Citrobacter isolates between 8% & 11% (w/v) for MIC and between 11% & 15% (w/v) for MBC. This indicates a medium variation of 3% & 4% (w/v) for MIC and MBC respectively. The overall average MIC of Citrobacter was similar to that reported by Lusby et al., 2005 with 10 % (w/v) using manuka honey and Blair et al., 2009 with 9.1±3 % (w/v) using medihoney. 136 3.3.2 Sensitivity of MDR and ESBLs to Omani honey: The sensitivity of all of the clinical isolates was determined against the four Omani honey samples with the highest total antibacterial activity detected (Table 3.7) using the broth dilution method. MICs and MBCs % (w/v) was performed at once for all 85 MDR/ESBLs isolates, mean and SD was calculated (Tables 3.17 to 3.22). Similar to manuka honey, it was deduced that Omani honey had a bactericidal mode of action against test isolates because it was found that OH-B, OH-C and OH-F exhibited relatively similar values for MIC and MBC for each species. (The highlighted box indicates the lowest MIC mean± SD (highest susceptibility) observed of that isolate among the other type of honey). Table 3.17: Susceptibility of 30 MDR Acinetobacter isolates against 4 types of Omani honey using broth dilution method. Isolate No. OH-B OH-C OH-G OH-F MIC MBC MIC MBC MIC MBC MIC MBC (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) 1. 18 18 14 14 16 16 14 14 2. 14 14 16 18 18 20 18 18 3. 20 20 18 18 20 20 14 14 4. 41 18 18 20 20 22 16 16 5. 41 18 18 20 16 18 20 20 6. 41 16 18 18 22 24 14 14 7. 41 16 20 20 20 22 14 14 8. 18 20 16 22 20 22 16 16 9. 20 20 18 18 24 24 18 22 10. 20 20 18 18 18 18 18 18 11. 41 18 20 20 20 22 18 18 12. 41 16 18 22 20 22 20 20 137 13. 41 18 20 20 16 16 14 14 14. 41 18 16 16 24 24 20 20 15. 41 20 16 16 20 22 18 18 16. 41 20 20 20 22 24 18 18 17. 41 20 20 20 18 22 20 20 18. 41 20 18 20 18 22 18 18 19. 41 20 20 20 20 22 18 18 20. 41 18 20 20 22 >24 18 18 21. 20 20 20 20 24 >24 18 18 22. 16 18 18 22 24 >24 18 20 23. 14 14 18 22 20 22 20 20 24. 18 20 20 20 22 24 18 20 25. 18 20 18 18 24 24 20 20 26. 18 18 18 20 24 >24 18 18 27. 18 18 16 16 22 22 18 18 28. 18 18 18 20 20 20 18 18 29. 18 18 16 20 20 22 18 18 30. 18 20 20 20 22 22 18 18 16.6± 18.4± 18.1± 19.2± 20.5± 21.8± 17.6± 17.8± 2 1.7 1.6 1.9 2.4 2.3 1.9 2.1 Mean ± SD (30) (n) number of isolates tested, this expirement was done once 138 Table 3.18: Susceptibility of 11 Klebsiella isolates against 4 types of Omani honey using broth dilution method. Isolate No. OH-B OH-C OH-G OH-F MIC MBC MIC MBC MIC MBC MIC MBC (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) 1. 12 14 14 14 20 24 14 18 2. 18 18 18 20 22 26 18 20 3. 20 20 20 20 24 28 20 24 4. 20 22 20 20 26 28 20 22 5. 20 22 20 20 24 26 18 22 6. 16 16 18 18 22 24 18 20 7. 20 24 20 22 24 28 20 22 8. 16 20 18 18 20 24 16 18 9. 14 16 18 20 20 22 18 20 10. 14 16 18 18 20 24 16 20 11. 16 16 18 18 22 24 18 22 12. 20 22 20 22 24 26 20 22 17.2±3 18.8± 3.2 18.5± 1.7 19± 2 22± 2 25± 1.9 18± 1.9 20.8± 1.8 Mean ± SD (11) (n) number of isolates tested, this expirement was done once 139 Table 3.19: Susceptibility of 10 E.coli isolates against 4 types of Omani honey using broth dilution method. Isolate No. OH-B OH-C OH-G OH-F MIC MBC MIC MBC MIC MBC MIC MBC (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) 1. 18 20 20 20 22 24 20 20 2. 20 20 20 20 24 24 22 22 3. 20 22 20 20 26 26 22 24 4. 16 18 18 20 20 22 18 18 5. 20 22 20 20 26 28 22 22 6. 20 20 20 20 24 24 18 20 7. 18 18 18 18 22 24 18 20 8. 18 20 18 22 22 24 18 20 9. 20 20 20 20 26 28 20 22 10. 18 18 20 20 24 26 18 20 18.8± 1.3 19.8± 1.4 19.4±1 20± 0.9 23.6±2 25± 1.9 19.6± 1.8 20.8± 1.6 Mean ± SD (10) (n) number of isolates tested, this expirement was done once 140 Table 3.20: Susceptibility of 15 Enterobacter isolates against 4 types of Omani honey using broth dilution method. Isolate No. OH-B1 OH-C OH-G OH-F MIC MBC MIC MBC MIC MBC MIC MBC (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) 1. 22 22 18 24 22 26 18 22 2. 20 20 20 22 26 30 20 24 3. 22 >24 20 22 30 >30 20 24 4. 22 24 20 22 26 28 20 24 5. 22 >24 20 20 26 30 20 22 6. 22 22 18 20 24 24 18 22 7. 22 22 20 22 26 >30 18 20 8. 24 24 22 22 30 30 24 24 9. >24 >24 24 24 30 >30 22 24 10. 22 24 22 24 30 >30 22 28 11. 22 >24 20 24 26 30 20 22 12. 22 22 22 22 30 >30 20 20 13. 22 >24 20 22 22 24 22 24 14. 22 >24 18 22 24 24 18 18 15. 20 20 18 22 24 24 18 20 21.6± 22.9± 20.1± 22.2± 26.4± 28± 20± 22.5± 0.9 1.5 1.7 1.3 2.9 2.7 1.8 2.4 Mean ±SD (15) (n) number of isolates tested, this expirement was done once 141 Table 3.21: Susceptibility of 12 Citrobacter isolates against 4 types of Omani honey using broth dilution method. Isolate No. OH-B OH-C OH-G OH-F MIC MBC MIC MBC MIC MBC MIC MBC (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) 1. 22 >24 20 22 28 >28 18 18 2. 24 24 20 22 >28 >28 22 24 3. 18 22 16 18 28 >28 16 18 4. 16 16 14 16 28 >28 16 16 5. 20 24 16 18 >28 >28 16 16 6. 18 18 16 18 >28 >28 16 18 7. 16 18 14 18 28 >28 14 16 8. 18 18 16 20 26 >28 14 18 9. 16 16 14 16 28 >28 14 16 10. 18 18 16 18 22 24 14 16 11. 16 16 14 16 28 >28 16 18 12. 16 16 14 18 24 26 18 20 18.1± 2.6 18.5 ± 3.2 15.8± 2.1 18.3 ±2 26 ± 2.5 27.5± 1.4 16.1± 2.3 17.8± 2.3 Mean ± SD (12) (n) number of isolates tested, this expirement was done once 142 Table 3.22: Susceptibility of 8 Serratia isolates against 4 types of Omani honey using broth dilution method. Isolate No. OH-B OH-C OH-G OH-F MIC MBC MIC MBC MIC MBC MIC MBC (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) (%w/v) 1. 24 >24 18 20 >28 >28 18 20 2. 20 22 20 24 >28 >28 20 24 3. 22 24 20 24 >28 >28 20 24 4. 20 22 20 26 >28 >28 14 26 5. 20 22 20 24 >28 >28 14 28 6. 20 24 22 24 >28 >28 14 28 7. 18 20 20 22 >28 >28 20 24 8. 18 18 22 26 >28 >28 16 16 20.2± 1.9 21.7± 2.1 20.2± 1.2 23.7± 1.9 >28 >28 17± 2.8 23.7± 4 Mean ± SD (8) (n) number of isolates tested, this expirement was done once According to the above tables Acinetobacter and Citrobacter were the most sensitive (low MIC recorded) isolates to Omani honeys and to manuka honey as well (lowest MIC recorded). Acinetobacter were inhibited with Omani honeys B with MIC 16.6 (%w/v) (Table 3.17). The remaining two Omani honeys C & F with MIC 15.8 & 16.6 (%w/v) respectively were more inhibitory to Citrobacter (Table 3.21). Serratia were less susceptible to most honeys tested with MIC ranged between 17 - >28 (%w/v) (Table 3.22). Thus it was difficult to state which is the most effective honey because each species responded in a different way. However, OH-G had the highest MIC/MBC ratio among the other types of honey. But OH-B had lowest MIC values reported for Acinetobacter, E.coli and Klebsiella so can be considered to be the most effective 143 (Table 3.17-3.19), whereas OH-C and OH-F were more effective against Citrobacter, Enterobacter and Serratia (Table 3.20-3.22). The susceptibility of isolates tested was recorded against manuka honey and 4 types of Omani honey tested according to above tables were: Acinetobacter > Citrobacter > Klesiella > E.coli > Enterobacter > Serratia 144 3.4 Time Kill Curves One representative isolate from each of the different cohorts of clinical test species (the least susceptible one) was selected to investigate the kinetics of inhibition with manuka honey. Bactericidal concentrations of manuka honey were required in each experiment for each isolate. Approximately doubled MIC values of honey concentration were therefore utilised (Table 3.23). Table 3.23: Cultures and honey concentrations used in the time-kill curves assay Test organism Strain No. MIC (%w/v) Test conc. used 2x MIC (%w/v) Acinetobacter 15 9 20 E.coli 7 13 30 Klebsiella 5 13 30 Enterobacteria 9 13 30 Citrobacter 2 10 20 Serratia 4 15 30 3.4.1 Inhibition of test organisms by manuka honey monitored by optical density: Initially the optical density of each isolate incubated in isosensitest broth for 24 hours with and without a bactericidal concentration of manuka honey was plotted against time (Fig 3.4 to 3.9). As shown in Figures 3.4 to 3.9, no increase in optical density observed over the 24 h exposure to honey thus was interpreted as complete inhibition of growth of these six isolates at test concentration of manuka honey used. A steady increase in optical density was observed during 24 h for all six isolates without the addition of honey was expected. 145 Figure 3.4: The effect of manuka honey (%w/v) on the growth of Acinetobacter The growth curve of Acinetobacter 2.2 Optical density at 550 nm 2 1.8 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 200 400 600 800 1000 1200 1400 1600 Time (minutes) Acinetobacter without honey Acinetobacter with 20% (w/v) manuka honey Figure 3.5: The effect of manuka honey (%w/v) on the growth of E.coli The growth curve of E.coli 2 Optical density at 550nm 1.8 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 200 400 600 800 1000 1200 1400 Time (minutes) E.coli without honey E.coli with 30% (w/v) manuka honey 146 1600 Figure 3.6: The effect of manuka honey (%w/v) on the growth of Klebsiella The growth curve of Klebsiella 2 Optical density at 550nm 1.8 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 200 400 600 800 1000 1200 1400 1600 Time (minutes) Klebsiella without honey Klebsiella with 30% manuka honey Figure 3.7: The effect of manuka honey (%w/v) on the growth of Citrobacter The growth curve of Citrobacter 1.8 Optical density at 550 nm 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 200 400 600 800 1000 1200 1400 Time (minutes) Citrobacter without honey Citrobacter with 20% (w/v) manuka honey 147 1600 Figure 3.8: The effect of manuka honey (%w/v) on the growth of Enterobacter The growth curve of Enterobacter Optical density at 550 nm 3.5 3 2.5 2 1.5 1 0.5 0 0 200 400 600 800 1000 1200 1400 1600 Time (minutes) Enterobacter without honey Enterobacter with 30% (w/v) manuka honey Figure 3.9: The effect of manuka honey (%w/v) on the growth of Serratia The growth curve of Serratia 2.2 Optical density at 550 nm 2 1.8 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 200 400 600 800 1000 1200 1400 Time (minutes) Serratia without honey Serratia with 30% (w/v) manuka honey 148 1600 3.4.2 Inhibition of test organisms by manuka honey monitored by total viable count Time-kill curves were repeated for each representative test organism as above, except that viability was monitored by total viable count (TVC) using the surface drop method (Miles & Misra 1938). For total culturable counts decimal dilutions from 10-1 to 10-7 were determined. The lowest dilution that gives a reasonable count was selected and calculated the colony forming units (CFU) to determine the actual viable cells in 1 ml. The mean data (Log10 CFU/ml) against time were plotted for each isolate on the graph. A linear regression analysis for each set of data was performed. Time-kill curves were obtained for Acinetobacter (Fig 3.10), E.coli (Fig 3.11), Klebsiella (Fig 3.12), Enterobacter (Fig 3.13), Citrobacter (Fig 3.14) and Serratia (Fig 3.15). Each graph illustrated the difference in viability between the test (with honey treatment) and control (without honey treatment). The activity of manuka honey against all strains demonstrated by maximal bacterial killing and surviving bacteria were counted at 0, 30, 60, 90, 120, 180, 240 and 300 minutes incubated at 37oC. From figures bellow it was observed that manuka honey at 2 times the MIC (Table 3.23) was bactericidal for all strains tested up to 5 h. Log reduction (LD) were calculated for each isolate up to 5 h exposure to manuka honey (Table 3.24). T-test was applied to establish the statistical difference between untreated cells and honey treated cells in the selected 6 species (Table 3.25). 149 3.4.2.1 Acinetobacter Acinetobacter cultivated without honey demonstrated a typical growth curve and reached the stationary phase after 5 h incubation with broth only (Fig 3.10). However, the test organism incubated with 2x MIC demonstrated rapid loss of viability. Therefore, 20% manuka honey resulted in 1.44-log10 reduction in CFU/ml compared to the starting inoculum (≈99% killing of Acinetobacter) at 5 h incubation (Table 3.24). Although honey treated Acinetobacter cells demonstrated the slowest killing rate among the selected isolates, there was a marked difference in viable cell count between Acinetobacter with and without honey (Table 3.25). 150 Figure 3.10: The effect of manuka honey on the viability of Acinetobacter. Time -to-kill curve of Acinetobacter Number of bacterial cells Log 10 CFU/ml 12 10 8 6 4 2 0 0 200 400 600 Acinetobacter without honey 800 1000 1200 1400 Time/Minutes Acinetobacter with 20% (w/v) manuka honey This data was done in triplicate 151 1600 3.4.2.2 E.coli The time-kill curve clearly shows an increase in number of E.coli cells without honey treatment (Fig 3.11). However in honey treated cells a reduction in the number of E.coli survivors were observed over time by 1.97-log10 reduction in CFU/ml at 5 h incubation with 30% (w/v) manuka honey (Table 3.24). In other words, 30% manuka honey was expected to be capable of almost killing 99% (equivalent 2-log10 reduction) of the population of E.coli within 5 h and to yield an undetectable bacterial count (<500 cfu /ml) at 24 h incubation. The variations between non honey and honey treated were highly significant P= 0.00 (Table 3.25) using T-test analysis. 152 Figure 3.11: The effect of manuka honey on the viability of E.coli. Time -to-kill curve of E.coli Number of bacterial cells log10 CFU/ml 12 10 8 6 4 2 0 0 200 400 600 800 1000 1200 Time (minutes) E.coli without honey E.coli with 30% (w/v) manuka honey This data was done in triplicate 153 1400 1600 3.4.2.3 Klebsiella Klebsiella cultivated without honey demonstrated a typical growth curve as the isolates presented above (Fig 3.12). However, the test organism incubated with 2xMIC manuka honey demonstrated a marked decrease with 5 x105 cfu/ml after 24 hours exposure. Hence 30% manuka honey achieved a 1.7-log10 reduction (≈99% killing) in Klebsiella population at 5 h. The cells continued to decrease till it reached < 500 CFU in 1 ml at 24 h (Fig 3.12). Addition of 30% manuka honey therefore caused significant difference in the viability of Klebsiella population (Table 3.25). 154 Figure 3.12: The effect of manuka honey on the viability of Klebsiella Time -to-kill curve of Klebsiella Number of bacterial cells log10 CFU/ml 12 10 8 6 4 2 0 0 200 400 600 800 1000 1200 Time (minutes) Klebsiella without honey This data was done in triplicate 155 Klebsiella with 30% (w/v) manuka honey 1400 1600 3.4.2.4 Citrobacter Citrobacter incubated with broth alone only showed increase in cell number for the first 120 minutes then there were no significant change in colony counts in each time ponit with incubation beyond 24 h. Viable counts of Citrobacter with 20% (w/v) manuka honey showed markedly declined of colony forming unit from 1x108 cfu/ml (eight Log CFU) to below 5.5x104 cfu/ml (five Log CFU). A time of exposure to honey from 4 to 5 h was enough to reduce 99.9% (3-log10 reduction) of the population of Citrobacter (Fig 3.13). Citrobacter incubated with 20% (w/v) manuka honey demostrated the greatested bactericidal activity at 5 h incubation with >3-log10 killing unit (Table 3.24). The change in cell count in Citrobacter between non honey and honey treatment was statistically significant (Table 3.25). 156 Figure 3.13: The effect of manuka honey on the viability of Citrobacter Time-to-kill curve of Citrobacter Number of bacterial cells Log10 CFU/ml 12 10 8 6 4 2 0 0 200 400 600 800 1000 1200 Time (minutes) Citrobacter without honey This data was done in triplicate 157 Citrobacter with 20% (w/v) manuka honey 1400 1600 3.4.2.5 Enterobacter The number of untreated cells increased with time as shown below (Fig 3.14). The total number of live Enterobacter cells significantly decreased when exposed to 30% manuka honey (Table 3.25). These differences were statistically significant (Table 3.25). A slow drop in numbers can be observed over time from 55 x106 just below (eight Log CFU) to 1.5 x106 just below (six Log CFU). Manuka honey with twice MIC concentration produced 1.57-log10 decrease in viable counts at 5 h (Fig 3.14). 158 Figure 3.14: The effect of manuka honey on the viability of Enterobacter Time -to- kill curve of Enterobacter Number of bacterial cells Log 10 CFU/ml 12 10 8 6 4 2 0 0 200 400 600 800 1000 1200 Time (minutes) Enterobacter without honey This data was done in triplicate 159 Enterobacter with 30% manuka honey 1400 1600 3.4.2.6 Serratia An increased number of colony forming units of Serratia was observed as shown by the trend line in the growth curve without honey, while number of cells decreased with time after exposure to 30% manuka honey with 1.87-log10 reduction in CFU/ml (≈99% killing). There was marked bacterial killing at 5 h incubation with honey. The cells continued to decrease till <500 colonies in 1 ml up to 24 hrs were found (Fig 3.15). The mean difference in number of colony forming units between non honey and honey treated Serratia were statistically significant (P <0.05) (Table 3.25). 160 Figure 3.15: The effect of manuka honey on the viability of Serratia Time-to-kill curve of Serratia Number of bacterial cell Log 10 CFU/ml 12 10 8 6 4 2 0 0 200 400 600 800 1000 1200 Time (minutes) Serratia without honey Serratia with 30% (w/v) manuk honey This data was done in triplicate 161 1400 1600 The Log Reduction (LR) was calculated for each isolate by subtracting the Log CFU at zero time and the Log CFU at 5 h incubation with 2x respective MICs of manuka honey. The higher LR, the faster was the killing rate (Table 3.24). Acinetobacter was the most susceptible MDR when tested with MIC, but Citrobacter were inhibited at a faster rate (Table 3.24). Table 3.24: Log reduction (LR) for each isolate after 5 h exposure to 2x respective MICs of manuka honey Isolate LogCFU/ml + honey LR At 0 h At 5 h Acinetobacter 7.04 5.6 1.44 E.coli 7.97 6 1.97 Klebsiella 7.39 5.69 1.7 Enterobacter 7.74 6.17 1.57 Citrobacter 8 4.74 3.26 Serratia 7.87 6 1.87 Sensitivity profile of six tested strains against honey at each concentration according to the table above is: Citrobacter > E.coli > Serratia > Klebsiella > Enterobacter > Acinetobacter 162 All isolates showed statistically significant differences in the mean of cell count between honey treated and untreated cells P <0.05 using T-test analysis (Table 3.25). Serratia determined the higher differences in cell count between non-honey and honey treated cells. Table 3.25: Comparison of the mean viable cell count between non honey and honey treated cells using paired sample test (T-test). Isolate ID Paired mean difference (Non honey-honey) P- value Acinetobacter 11.57 <0.005 E.coli 8.86 <0.005 Klebsiella 8.90 0.001 Enterobacter 10.33 <0.005 Citrobacter 9.10 <0.005 Serratia 12.19 <0.005 163 3.5 Effect of honey on bacterial structure: Electron microscopy is an essential tool to observe the ultrastructural and physical changes that occur to cells after adding certain agents. Details of surface structures and bacterial morphology aid an understanding of the action of various drugs on bacteria. In this project both scanning and transmission electron microscopy was used to determine membrane integrity, morphological changes of cells, electron density of the cytoplasm and evidence of cell division before and after exposure to honey. 3.5.1 Growth Curves: The exponential cells were collected after 3 h incubation at 37°C in ISB as indicated by the arrows in each of the growth curves for Acinetobacter (Fig 3.16), E.coli (Fig 3.17), Klebsiella (Fig 3.18), Enterobacter (Fig 3.19), Citrobacter (Fig 3.20), and Serratia (Fig 3.21). The exponential phase was selected because of active growth of cells was expected to result in many proteins and enzymes being synthesized. These molecules are considered to be the main target site for various inhibitors and thereby help in identifying the action of an antimicrobial agent. Biosynthetic pathways in stationary phase bacteria are more likely to reflect secondary metabolism, rather than central pathways. Exponential phase cultures were treated with and without approximately twice MIC concentrations of honey and monitored for 180 minutes. 164 Figure 3.16: Growth curve of Acinetobacter in ISB Growth Curve of Acinetobacter Optical Density at 550 nm 0.7 0.6 0.5 0.4 0.3 0.2 0.1 0 0 100 200 300 400 500 600 700 600 700 Time (minutes) Figure 3.17: Growth curve of E.coli in ISB Growth Curve of E.coli Optical Density at 550 nm 1.2 1 0.8 0.6 0.4 0.2 0 0 100 200 300 400 Time/minutes 165 500 Figure 3.18: Growth curve of Klebsiella in ISB Growth curve for Klebsiella 2 Optical Density at 550 nm 1.8 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 100 200 300 400 500 600 700 Time (minutes) Figure 3.19: Growth curve of Enterobacter in ISB Growth curve for Enterobacter Optical Density at 550 nm 1.2 1 0.8 0.6 0.4 0.2 0 0 100 200 300 400 Time (minutes) 166 500 600 700 Figure 3.20: Growth curve of Citrobacter in ISB Growth curve for Citrobacter Optical Density at 550 nm 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 100 200 300 400 500 600 700 Time (minutes) Figure 3.21: Growth curve of Serratia in ISB Growth curve for Serratia 1.8 Optical Density at 550 nm 1.6 1.4 1.2 1 0.8 0.6 0.4 0.2 0 0 100 200 300 400 Time(minutes) 167 500 600 700 3.5.2 Scanning Electron Microscopy (SEM): 3.5.2.1 SEM of Acinetobacter For Acinetobacter an average of ten SEM micrographs with a magnification of 5,000 (for cell count) and two micrographs with a magnification of 20,000 (for cellular details) were taken for each time point. In total 30 SEM micrographs were taken for untreated honey samples (control) and 50 micrographs for treated honey samples. However only representative images for 0, 60, 90, 150 and 180 time points are shown here. SEM micrographs of untreated cells of Acinetobacter incubated with broth only at time 0 were observed to have a regular rod shaped cell with a smooth surface for 95% of the cells and cell length was 3 µm (Fig. 3.22); normal cell size is between 1.5 to 2.5 µm (Gillespie and Hawkey 2006). However, after 3 h incubation in liquid media this bacterium became enlarged and appeared as long bacilli (Fig. 3.24, 3.26, 3.28) with mean cell size increased to 5.5 µm. This bacterium normally tends to be a bacillus in shape when it incubated for long time in liquid media and/or if collected in exponential growth phase (Murray et al., 2007). Septated cells were also observed with no surface changes and no debris. In the honey treated sample, the majority of cells (94%) appeared unchanged for the first 30 minutes exposure to manuka honey (Fig 3.23). From 60 minutes onwards lots of debris was observed, suggesting that some leakage of cellular material or lysis had taken place. Also clumping and cell aggregation increased (Fig. 3.25, 3.27 & 3.29). There were significant changes in the cell length of Acinetobacter after 1 h exposed to 20% (w/v) manuka honey compared to untreated honey (p = 0.0216) 168 (Table 3.26). The length of individual cells treated with honey appeared to be shorter than those without honey, which in turn resulted in decreased cellular volume. In addition an increased number of septa were seen after 150 minutes incubation with 20% (w/v) manuka honey (Fig 3.29). Formation of elongated cells seemed to be decreased (P = 0.025) (Table 3.26) which again would lead to decrease in cellular volume. An interesting effect seen in this stage was that multiple cell division constriction sites were apparent on some filaments of cells, suggesting that cell separation had not been completed (Fig 3.29 b, c & d). Also more fragments of debris were present in honey- treated cells than in untreated cells incubated for the same time (Fig 3.28 b). A significant change occurred after 3 hrs incubation where marked damage observed in cell surface. It appeared that treated cells entirely diffused and lysed (Fig 3.31) compared to control cells. The statistical analysis of morphological changes in untreated and treated honey cells are shown in Table (3.26) 169 Figure 3.22: SEM micrograph of untreated cells of Acinetobacter after 0 minutes at x5,000 magnification Figure 3.23: SEM micrograph of Acinetobacter cells exposed to 20% (w/v) manuka honey after 0 minutes at x5,000 magnification 170 Figure 3.24: SEM micrograph of untreated cells of Acinetobacter after 60 minutes at x5,000 magnification Figure 3.25: SEM micrograph of Acinetobacter cells exposed to 20% (w/v) manuka honey after 60 minutes at x5,000 magnification Clumps Debris 171 Figure 3.26: SEM micrograph of untreated cells of Acinetobacter after 90 minutes at x5,000 magnification Figure 3.27: SEM micrograph of Acinetobacter cells exposed to 20% manuka honey after 90 minutes at x5,000 magnification Debris Clumps 172 (w/v) Figure 3.28: SEM micrographs of untreated cells of Acinetobacter after 150 minutes at x5,000 A & x20,000 B magnification respectively A Single division B 173 Figure 3.29: SEM micrographs of Acinetobacter cells exposed to 20% (w/v) manuka honey after 150 minutes at x5,000A, x10,000B, x20,000C & x25,000D magnification respectively Debris A Multiple division sites B 174 Cell division C Multiple septa in each cell D 175 Figure 3.30: SEM micrographs of untreated cells of Acinetobacter after 180 minutes at x5,000 A & x10,000 B magnification respectively A B 176 Figure 3.31: SEM micrographs of Acinetobacter cells exposed to 20% (w/v) manuka honey after 180 minutes at x 5,000 (A) & (B) magnification respectively Cell lysis A B 177 3.5.2.2 SEM of E.coli For E.coli an average of four SEM micrographs with a magnification of 5,000 (for cell count) and one micrograph with a magnification of 20,000 (for cellular details) were taken for each time point. In total 20 SEM micrographs were taken for untreated honey samples and 30 micrographs for treated honey samples. However, due to small variation in cell morphology between each time point, only representative images collected at 30 and 180 time points were shown here. SEM micrographs of control cells of E.coli incubated with broth only were shown to have rods with regular structure and normal size after 3 h incubation in liquid media (Fig 3.32 & 3.34) In honey treated cells there was no change in shape and size at 0 min (not shown) (P >0.05). There was no significant difference of cell length between treated honey sample and untreated one at most of the time point (P> 0.05) (Table 3.26). However, deformation of cells was observed after 3 hrs incubation with 30% manuka honey (P= 0.025) (Fig 3.35, white arrows). Also it was observed that the cells exposed to honey aggregated together by forming extended strand materials (filament) shape around each cell probably cytoplasmic consistuent (Fig 3.33 & 3.35). Septated cells were not observed in this stage. 178 Figure 3.32: SEM micrograph of untreated cells of E.coli after 30 minutes at x5,000 magnification Normal cells Figure 3.33: SEM micrograph of E.coli cells exposed to 30% (w/v) manuka honey after 30 minutes at x5,000 magnification Cells with clumps 179 Figure 3.34 : SEM micrograph of untreated cells of E.coli after 180 minutes at x5,000 magnification Figure 3.35 : SEM micrograph of E.coli cells exposed to 30% (w/v) manuka honey after 180 minutes at x5,000 magnification Filament shapes 180 3.5.2.3 SEM of Klebsiella Klebsiella was treated with 30% manuka honey and 40% Omani honey (OH-B). An average of eight SEM micrographs with a magnification of 5,000 (for cell count) and two micrographs with a magnification of 15,000 and 20,000 (for cellular details) were collected for analysis of both types of honey at each time point. In total 20 SEM micrographs were taken for untreated honey samples and 60 micrographs for treated honey samples. However, only 30 and 180 time points were shown here. SEM micrographs of Klebsiella incubated with broth alone (no honey) were found to have a conventional rod shape after 3 h incubation in liquid media with approximate size of 0.6 to 6 µm long (Fig 3.36 & 3.37). In SEM micrographs of honey treated cells cell size and shape did not appear to be significantly different to untreated cells after 30 min (Fig 3.38 & 3.40) for both honeys (P = > 0.05). However, cell size significantly increased between 1 to 3 hours exposure for both honeys (P = < 0.05) (Table 3.26). In addition rough cell surfaces were observed at the same time points (Fig 3.39 b,c,d manuka honey) and (Fig 3.41 b,c,d Omani honey). There few septa present with no debris observed. 181 Figure 3.36: SEM micrographs of untreated cells of Klebsiella after 30 minutes at x5,000 (A) & 15,000 (B) magnification respectively Normal cells A B 182 Figure 3.37: SEM micrographs of untreated cells of Klebsiella after 180 minutes at x5,000 (A) & 15,000 (B) magnification respectively A Normal cells B 183 Figure 3.38 : SEM micrographs of Klebsiella cells exposed to 30% manuka honey after 30 minutes at x5,000 (A) & 15,000 (B) magnification respectively A B 184 Figure 3.39: SEM micrographs of Klebsiella cells exposed to 30% (w/v) manuka honey after 180 minutes at x5,000A, x15,000B,C & x20,000D magnification A Rough surfaces B 185 Rough surface C D 186 Figure 3.40: SEM micrographs of Klebsiella cells exposed to 40% (w/v) Omani honey after 30 minutes at x5,000 A & x15,000 B magnification respectively A B 187 Figure 3.41 : SEM micrographs of Klebsiella cells exposed to 40% (w/v) Omani honey after 180 minutes at x5,000 A & x 20,000 B,C & D magnification respectively A Rough surface B 188 C D 189 3.5.2.4 SEM of Enterobacter Similarly for Enterobacter an average of four SEM micrographs with a magnification of 5,000 (to do cell counts or cell sizes) and one micrograph with a magnification of 20,000 (for examination of cellular surface details) were taken for each time point. In total 20 SEM micrographs were taken for untreated honey samples and 30 micrographs for treated honey samples. However, only 30 and 180 time points were shown here. Again, regular bacilli shaped cells with no surface irregularities were observed in untreated sample (Fig. 3.42). After exposure to 30% (w/v) manuka honey lots of mesh like material between cells was obvious as a result of cells aggregation (Fig. 3.43 & 3.45). There were no significant difference in cell size between untreated and treated honey samples at any time point (P = > 0.05) (Table 3.26). 190 Figure 3.42: SEM micrographs of untreated cells of Enterobacter after 30 minutes at x5,000 A & x15,000 B magnification respectively Normal cells A B 191 Figure 3.43: SEM micrographs of Enterobacter cells exposed to 30% manuka honey after 30 minutes at x5,000 A & B magnification respectively Cells with clumps A B 192 (w/v) Figure 3.44: SEM micrographs of untreated Enterobacter cells after 180 minutes at x5,000 A & x20,000 B magnification respectively Filter membrane Normal cells A B 193 Figure 3.45: SEM micrographs of Enterobacter cells exposed to 30% (w/v) manuka honey after 180 minutes at x5,000 (A & B) magnification respectively Mesh like structure A B 194 3.5.2.5 SEM of Citrobacter For Citrobacter an average of four SEM micrographs with a magnification of 5,000 (for cell count) and one micrograph with a magnification of 20,000 (for cellular details) were taken at each time point. In total 20 SEM micrographs were taken for untreated honey samples and 30 micrographs for treated honey samples. However, only 30 and 180 time points are shown here. Regular bacilli shaped cells with approximate size 2 to 6 µm long with smooth surfaces were observed in untreated cells (Fig. 3.46). After exposure to 20% (w/v) manuka honey, the surface of bacterial cells seemed to be rougher, maybe as a result of outer membrane damage (Fig. 3.47 & 3.49). Also, at higher magnification black areas were present on the surface of some cells (Fig. 3.49 b) which was suggestive of pore formation. There were significant difference in cell size between untreated and treated honey samples at 30, 90 and 180 minutes time point (P ≤ 0.05) (Table 3.26). 195 Figure 3.46: SEM micrographs of untreated cells of Citrobacter after 30 minutes at x5,000 A & x15,000 B magnification respectively A Normal cells B 196 Figure 3.47: SEM micrographs of Citrobacter cells exposed to 20% (w/v) manuka honey after 30 minutes at x10,000 A & x15,000 B magnification respectively A B 197 Figure 3.48: SEM micrographs of untreated Citrobacter cells after 180 minutes at x5,000 (A & B) magnification respectively A B 198 Figure 3.49: SEM micrographs of Citrobacter cells exposed to 20% (w/v) manuka honey after 180 minutes at x5,000 A & x15,000 B magnification respectively Filter membrane A Pore formation B 199 3.5.2.6 SEM of Serratia For Serratia an average of four SEM micrographs with a magnification of 5,000 (for cell count) and one micrograph with a magnification of 20,000 (for cellular details) were taken at each time point. In total 20 SEM micrographs were taken for untreated honey samples and 30 micrographs for treated honey samples. However, only 30 and 180 time points are shown here. Regular bacilli shaped cells with approximate size 0.9 to 2 µm long with smooth surfaces were observed in untreated sample (Fig. 3.50). After exposure to 30% (w/v) manuka honey for 30 minutes cells surfaces were noticeably uneven and cell debris seemed to be present, suggesting that some cells had lysed. Blebs were also seen on some honey treated cells (Fig 3.51). After 180 minutes exposure to 30 % (w/v) manuka honey, elongated cells were significantly present (p = 0.0002) with cells aggregation (Table 3.26). Extracellular material was observed, suggesting that biofilm formation had been initiated (Fig. 3.53). Septated cells were not observed at this stage. 200 Figure 3.50: SEM micrograph of untreated cells of Serratia after 30 minutes at x5,000 magnification Figure 3.51: SEM micrograph of Serratia cells exposed to 30% (w/v) manuka honey for 30 minutes at x 5,000 magnification Filter membrane 201 Figure 3.52: SEM micrograph of untreated cells of Serratia after 180 minutes at x5,000 magnification Figure 3.53: SEM micrograph of Serratia cells exposed to 30% (w/v) manuka honey after 180 minutes at x5,000 magnification 202 Table 3.26: Comparison of changes in cell length (μm) of isolates observed in scanning electron microscopy between untreated and honey treated cells, respectively, after 240 min. (P value <0.05) (Mann-Whitney Test) Time point Acinetobacter (n=20) E.coli (n=20) Manuka honey Klebsiella (n=20) Manuka Omani Manuka honey Citrobacter (n=20) Enterobacter (n=20) Serratia (n=20) Manuka honey Manuka honey Manuka honey 0 0.85 0.85 NT NT 0.41 NT NT 30 NT NT 0.104 0.38 0.0046 0.79 0.623 60 0.0216 NT NT NT 0.733 NT NT 90 NT NT 0.140 0.037 0.064 NT 0.049 120 NT 0.82 0.037 0.0091 NT NT NT 180 0.025 0.025 NT NT 0.053 0.67 0.0002 240 NT 0.909 0.0173 0.0046 1.00 NT NT n= number of cells observed P value = <0.05 expressed in bold NT = Not tested 203 3.5.2 Transmission Electron Microscopy (TEM): 3.5.2.1 TEM for Acinetobacter: TEM micrographs of untreated cells of Acinetobacter revealed regularly shaped cocco-bacilli with entire margins after 60 minutes incubation in ISB (blue arrows) with a few elongated cells were also seen (Fig 3.54). After 3 hrs cells did not appear to have major change in cell shape or size (Fig 3.56). However, distinct morphological changes had occurred in honey treated cells after 60 minutes incubation with 20% (w/v) manuka honey in ISB. These changes took place in the cell membrane, which was observed to be incomplete and indistinct in some cells (Fig 3.55, red arrows) compared to the well defined cell membrane seen in untreated cells (Fig 3.54, blue arrows). Moreover, some cells presented with black deposit possibly mineral and some with empty vacuoles inside some cells (Fig. 3.55). The presence of cellular debris indicated lysis of cells (Fig. 3.55 & 3.57). The number of cells with septa was increased following treatment with 20% (w/v) manuka honey (Fig 3.57 black arrows). 204 Figure 3.54: Transmission micrographs of untreated cells of Acinetobacter after 1 h incubation with isosensitest broth (ISB) at 16,000x magnification (A, B, C) Cocco-bacilli shape A 300 nm x16,000 Define cell wall B 300 nm x16,000 C 300 nm x16,000 205 Figure 3.55: Transmission micrographs of Acinetobacter incubated with isosensitest borth (ISB) containing 20% (w/v) manuka honey for 1 h at 16,000x magnification. Debri s Hole s 300 nm x16,000 A Black deposit B 300nm x16,000 C 300nm x16,000 206 Figure 3.56: Transmission micrographs of untreated cells of Acinetobacter incubated with isosensitest broth (ISB) after 3 h at 16,000x(A,B) & 32,000x(C) A 300nm x16,000 B 300nm C 300nm 207 x16,000 x32,000 Figure 3.57: Transmission micrographs of Acinetobacter incubated with isosensitest broth (ISB) containing 20% (w/v) manuka honey after 3 h at 16,000x magnification A 300nm x16,000 Debris B 300nm x16,000 Septa C 300nm 208 x32,000 3.5.2.2. TEM for E.coli: TEM images of untreated cells of E.coli did not appear to show obviously damaged or abnormal shaped and sized cells. Nevertheless empty spaces or holes were observed in some cells (Fig 3.58 & 3.60). Honey-treated cells of E.coli with 30% (w/v) manuka honey demonstrated gaps between the cell membrane and the cytoplasm which seemed to have caused the membranes to shrink away from the cytoplasm (Fig 3.59). Also deformed cell membrane could be seen in some images. Very interestingly, due to membrane rupture the intracellular components had leaked out from the cells after honey treatment and formed empty cells with black deposit inside (Fig 3.59). After 3 hrs incubation with 30% (w/v) manuka honey these samples also demonstrated cells with irregular shapes with relatively less electron dense material compared to untreated cells (Fig 3.61). Septated cells were not observed in this stage. Unfortunately it was not possible to process all of the ESBL organisms for structural changes induced by honey. 209 Figure 3.58: Transmission micrographs of untreated cells of E.coli after 1 h incubation with isosensitest borth (ISB) at 16,000x magnification Hole A 300nm x16,000 B 300nm 300nm C 210 x16,000 x16,000 Figure 3.59: Transmission micrographs of E.coli incubated with isosensitest borth (ISB) containing 20% (w/v) manuka honey after 1 h at 16,000x magnification Empty cell with deposit A 300nm x16,000 Lysed cell Empty cell with deposit B 300nm x16,000 Empty cell with deposit C Deformed cells 300nm 211 x16,000 Figure 3.60: Transmission micrographs of untreated cells of E.coli after 3 h incubation with isosensitest broth (ISB) at 16,000x(A) & 32,000x (B,C). Holes A 300nm x16,000 B 300nm x32,000 Define cell wall C 300nm x32,000 212 Figure 3.61: Transmission micrographs of E.coli incubated with isosensitest broth (ISB) containing 20% (w/v) manuka honey after 3 h at 16,000x magnification Irregular cells A 300nm x16,000 Less electron dense B 300nm x16,000 C 300nm x16,000 213 3.6 Effect of honey on bacterial proteins: 3.6.1 Two Dimensional Gel Electrophoresis: This technique is able to separate proteins using two distinct steps: the isoelectric focusing (IEF) separates proteins according to their isoelectric point (pI) and SDSpolyacrylamide gel electrophoresis (SDS-PAGE) separates proteins according to their molecular weight (MW). Each resulting spot from a 2-D gel can be matched to a single protein in the sample. Then it can be analysed using PDQuest Basic 8.0 software to determine the number and position of spots. Besides obtaining protein the pI and molecular weight identification, this method detects the amount of each protein present. The proteome analysis of Acinetobacter using 2-D electrophoresis was carried out to establish the differences in protein expression between treated and untreated honey cells. This test was performed in Acinetobacter only because the electron microscopy results of this bacterium were shown more physiological damage. The software that was mention previously was able to detect the number of spots present in each test gel (honey treatment) (Fig 3.63) and compared it to control gel (no honey) (Fig 3.62). This allows for identifying those spots whether up or down regulated by comparing their expression between these gels. A total of 10 gels (control & test) were run successfully according to the method described above, but despite repeated attempts, unfortunately the effect on protein expression within this bacterium after exposure to 20% manuka honey was not possible at this stage. This techniques offers promise in investigating the effects of honey on ESBLs, but further work in optimising the conditions is needed. It has proved valuable in UWIC in investigating the effect of manuka honey on MRSA (Jenkins et al., 2011). 214 Figure 3.62: 2-D protein electrophoresis gel of Acinetobacter cells without honey treatment Protein spots Figure 3.63: 2-D protein electrophoresis gel of Acinetobacter cells exposed to 20% (w/v) manuka honey 215 Chapter 4 Discussion 216 “The therapeutic potential of uncontaminated, pure honey is grossly underutilized. It is widely available in most communities and although the mechanism of action of several of its properties remain obscure and needs further investigation, the time has now come for conventional medicine to lift the blinds off this „traditional remedy‟ and give it its due recognition” (Zumla and Lulat 1989). This study was carried out to investigate the efficacy of Omani honey and manuka honey in the inhibition of Gram negative multi-drug resistant organisms implicated in wound infections. The antibacterial potency of each honey was determined by bioassay method, MIC and MBC, time-kill study and electron microscopy. Each experiment provided some insight into possible inhibitory mechanisms of honey on microorganisms. 4.1 Antibacterial activity of honey samples: For many years local, natural and untreated honey was previously used in different countries for their antibacterial activity against different types of bacteria (Alandejani et al., 2009; Al-Jabri et al., 2003; Al-Waili, 2004; Basson and Grobler 2008; Wadi et al., 1987). In order to quantify the antibacterial activity of a honey using the agar well diffusion method, a bioassay in which activity was compared to phenol as a reference was developed in New Zealand (Allen et al., 1991). Phenol is a chemical that was used as an antiseptic in surgical procedures in the nineteenth century. It has been used as a reference for the evaluation of the potency of many antiseptics, but it is not usually used for wound treatment because of its hazardous effect in damaging cells and tissues. It could be therefore argued that it is not a suitable standard to measure the 217 activity of honey, because topical treatments for wounds must be non-cytotoxic, as well as antibacterial. Nevertheless it has been used in several studies. A New Zealand study of 345 honey samples found that non-peroxide activity presented only in 25 honey samples which were identified as either manuka or viper‟s bugloss (Allen et al., 1991). The same bioassay was used to survey antibacterial activity in 139 Welsh honeys and it was found that not all honeys had a detectable amount of total activity, and non-peroxide activity was not detected (Wheat 2004). Also, a study of 30 Portuguese honeys showed only 7 honeys possessed non-peroxide activity with 11.5 % (w/v) phenol equivalent (Henriques et al., 2005). Twenty years from Allen et al., another New Zealand survey on the antibacterial activity of 477 Australian honey samples found that 80 samples (16.8%) exhibited non-peroxide activity (Irish et al., 2011) From the bioassay most Omani honey tested in this project had a certain amount of antibacterial activity (total activity) which ranged between < 2% and 22.8% (w/v) phenol equivalent where 2% (w/v) is the lowest phenol standard able to cause a zone of inhibition. However, none of them demonstrated detectable activity when tested for non-peroxide activity, ie incubation with catalase. All the antibacterial activity of Omani honey on dilution was therefore related to the formation of H2O2 and they can be called peroxide honeys. Manuka honey used in this study possessed an equal amount of antibacterial activity both total activity with 21.3±0.85 and non-peroxide activity with 21.4± 0.8 (% w/v) phenol equivalent. Manuka honey therefore had nonperoxide type activity and this confirmed the deduction of Allen, Molan and Reid (1991). 218 Non-peroxide honey shown to be effective in wound management. According to many studies on the antibacterial activity of different types of honey, manuka honey has been shown to be the most effective honey and because anti-bacterial activity on dilution was entirely due to the non-peroxide components that are found in this honey, this gives manuka honey an advantage over peroxide honeys (Al Somal et al., 1994; Molan and Russell 1988; Snow and Manley-Harris 2003). There are several rating systems recently developed to describe the quality and effectiveness of non-peroxide honey as an anti-microbial agent for wound treatment. Unique Manuka Factors (UMF) was the first rating system identified to denote the potency of honey. Manuka honey with UMF activity of ten or above (10 +) (same potency of 10% phenol equivalent) is the most acceptable for therapeutic use. Methylglyoxal (MGO) and the Molan Gold Standard are new registered trademark from different organizations to rate the potency of manuka honey (http://www.molangoldstandard.co.nz/article). 4.2. Chemical & physical analysis of honey samples Different types of local honey from different origins were studied for chemical compositions and antioxidant activity (Aljadi and Kamaruddin 2004; Al-Mamary et al., 2002; Beretta et al.,2005; Estevinho et al., 2008). However, the physicochemical analysis of Omani honey including the phenolic acid and anti-radical activity was not well studied. Determination of honey compositions and its source of origin aid in identifying its biochemical properties. Omani honey was traditionally assessed by sensory tests such as taste, colour, aroma and texture which make the detection of honey quality more difficult. Generally natural honey is variable in its composition mainly in pH value, ash, water and sugar content. 219 The selected Omani honeys were analysed for their sugar, water, pH, HMF, colour, protein, antioxidant and pollen. The values were compared to the reference National Honey Board (NHB) (Table 4.1) and most parameters were found to be within the NHB range. Table 4.1: The physicochemical analysis of selected honeys tested Honey Sample pH Water content %(w/v) Sugar content % (w/v) Protein (mg/g) HMF (mg/kg) Antiradical activity% Phenol content (eq/kg) NHB 3.5-5.5 17.2 82.4 0.7 15 N/A N/A Mean ± 4.7± 15.8± 81± 4.7± 11.1± 64.6± 89.7± SD (n) of Omani honey 0.9 1.9 2.8 1.5 11.9 4.1 64.8 Manuka honey 3.5 20 78 0.3 3 61.1 65.4 N/A (not available) To date there has been only one research study that was conducted in Sultan Qaboos University in Oman in which two parameters (sugar fractions and protein content) in 51 Omani honeys were analysed. These honeys collected from Muscat and Al-Batina regions during summer and winter seasons between 1999- 2002. The mean sugar was recorded as 67.41% and the mean protein was as low as 2 ± 1 mg/g. The same study also compared the level of these two factors in summer and winter honeys, and in multifloral and unifloral honeys. It was found the level of sugars in honeys collected in summer was higher than winter honey whereas no difference in sugar between multifloral and unifloral honeys was found. However the protein content was not affected by either season or the type of flora (Sajwani et al., 2007b). This study, therefore, has provided detailed information about selected Omani honeys. 220 Sugars are the major content of honey, however when these sugars (glucose and fructose) broken down, the HMF released. An increase level of HMF in honey samples occur when honey is stored for long periods at high temperature. Using improper storage temperature or breakdown of sugars by acid hydrolase, therefore releases high amount of HMF which could be used an indicator of honey quality (Badawy et al., 2004; Sanz et al., 2003). Honey is known to possess antioxidant activity which is one of main therapeutic benefits of honey in trapping the free radicals and promoting wound healing (Molan 1992b). At an injury or wound site the activity of free radicals is increased. Topical application of honey to the injury site is expected to mop up the free radicals and so promote rapid healing (Subrahmanyam et al., 2003; Henriques et al., 2005). Omani honey exhibited high levels of anti-radical activity (64.6± 4.1%) compared to tualang honey (41.3±0.78%) (Mohammed et al., 2010). Phenolic compounds in honey have been considered as possible indicators of the botanical origin of honey (Al-Mamary et al., 2002; Yao et al., 2003). Honey acts a natural antioxidant and it is known that the colour of honey is related to antioxidants. Dark honey has been determined to contain more phenolic components and so more antioxidant potency than the lighter ones (Bogdanov et al., 2004; Estevinho et al., 2008; Pyrzynska & Biesaga 2009). There are more than 500 polyphenolic compounds already known in honey where phenolic acid and flavonoids are most predominant (Anklam 1998). These compounds are identified by high performance liquid chromatography and electrophoresis (Pyrzynska & Biesaga 2009). 221 The colour of honey is the most obvious physical parameter that is observed directly by users. It varies with botanical origins, age, storage condition and the amount of pollen present. The colour can vary from water white, amber brown shade to almost black. There are two common classification systems used for colour grading, the Pfund and Townsend classifications. These systems depend on optical assessment to obtain the intensity of colour (Bogdanov et al., 2004). A new method has been introduced using reflectance spectroscopy for colour classification (Terrab et al., 2002a) The colour of each Omani honey was estimated initially by visual assessment, then it was tested by determining the optical density of 50% (w/v) honey at 560 nm and the colour was classified according to Townsend system (Townsend 1969). The results obtained from visual assessment completely matched the Townsend system. The colour of most honey samples ranged from extra light amber to dark amber even black. This means that Omani honeys exhibited a dark colour, which is also visually obvious in all honeys sold in Oman. Elevated level of anti-radical activity with phenolic content and antioxidant in Omani honeys highlight the important of these compounds in human health to fight infections and in nutrition as a deitery supplement of vitamins. Eight honey samples collected for this project were produced in four different regions of Oman. An estimated flora source for each honey sample was provided by the beekeepers. Pollen grains were analysed and full identification of flora source was kindly provided from National Pollen And Research Unit (NPARU) at Worcester University (Table 3.9). Five honey samples showed that nectar sources came from mixed flora sources (multi-flora). These are Graminae (the grasses), 222 Acacia (thorn trees), Myrtacae eucalyptus and Brassica types. However, the remaining three honeys were not identified because of little pollen present in the slides and may have been honeydew honeys. This demonstrated that the beekeepers were not always correct in their assumptions about floral origin of honey due to lack materials that could used in identifying pollen. The quality of honey is based on their flora source which is determined by pollen analysis, and chemical composition. The latter is more accurate and specific in analysis of various components that present in honey and it involves identifying the flora origin of honey. The price of honey is depended on its quality. 4.3 Effect of honey samples against test cultures: Several reports have been published regarding the antimicrobial activity of different types of honey against variety of organisms including Staphylococcus (MRSA & MSSA), Pseudomonas aeruginosa, Streptococcus and anaerobes (Cooper et al., 1999; Maedaa et al., 2008; Mullai and Menon 2005, 2007) but little was documented for Gram negative Enterobacteriaceae especially MDR and ESBL producing organisms before this study. Here the antibacterial activity of five types of selected honey was tested against six species of MDR organisms that usually cause wound infections. These were Acinetobacter, E.coli, Klebsiella, Citrobacter, Enterobacter and Serratia. Eighty seven isolates in total were tested for MIC and MBC against these five types of honey including manuka honey. MIC is a measurement of the quantity of honey required for bacterial inhibition. To determine the MIC of honey samples against selected bacteria two methods were 223 used: agar incorporation method and broth dilution method using 96 well microtiter plates. The results in latter method are determined by visual inspection of turbidity and confirmed by using spectrophotometric assay. Initially agar incorporation was used for 10 Acinetobacter isolates against manuka honey. The mean MIC results showed 7.18 (%w/v) compared to 7.17 (%w/v) using broth dilution methods. The nature of agar incorporation method is basic but it has some limitations in the results as it does not report MBC values and limits the number of test replicates. Also it is time consuming, required large amount of samples and extensive plate preparation was also needed. There were no differences in the results between two techniques though the broth dilution technique presents many advantages including: smaller volume of samples used, rapid and cheaper, allows more replicates in the same plate, produce large amount of statistical data and determines the MBC value (Patton et al., 2006). Recently, a microtiter plate assay has been widely used in antibiotic testing and bioactivity (Casey et al., 2004; Kuda et al., 2004). Thus because of these advantages, the broth dilution method was used for all other isolates instead. The bactericidal activity of any antimicrobial agent is usually more desirable than agents with bacteriostatic activity. The antimicrobial agent considered to have a bactericidal action is when MIC/MBC ratio < 4 while the bacteriostatic action is when this ratio become >4 (Levison 2004). From the MIC and MBC results it was observed that all honeys exhibit bactericidal mode of action against all isolates tested in this project. Different honey reacts differently on each isolate and at different concentrations. It is therefore difficult to determine which honey has a more potent activity than others. However, manuka honey remained the most effective against 224 major wound pathogens, consistently giving lower MIC values for all of the test organisms. According to the summarized charts below (Fig. 4.1- 4.6) Acinetobacter isolates were more sensitive (low MIC recorded) to 3 types of honey (manuka honey, and Omani honeys B & G) with MICs of 7.17, 16.6 and 20.5 (%w/v) respectively. The remaining two Omani honeys (C & F) with MICs of 15.8 and 16.6 (%w/v) respectively were more active against Citrobacter. Serratia cultures were less susceptible to most of the honeys tested with MICs ranging between 13.3-28 (%w/v). As previously mentioned the antimicrobial activity of honey against MDR Gram negative bacilli was not well documented in the medical literature. However, in some circumstances the MIC values determined from this study were comparable to the MICs reported earlier (Table 4.2). However, comparisons were limited by variations in methodology and the honeys utilised. In Oman honey has been used for thousand of years in the treatment of many diseases. In this study only small number of honey samples were tested and this does not account for all of the types present in Oman. Few studies of Omani honey were reported on their antibacterial activity. It was documented that Omani honey has a broad spectrum activity against Staphylococcus aureus, E. coli and P. aeruginosa (Al-Jabri et al., 2003, 2005b). In addition the combination between honey and antibiotics was first initiated by Al-Jabri et al., (2005a) who found that Omani honey had a synergistic effect with aminoglycosides. However, analysis of Omani honeys needs to be more extended by collecting larger number of samples, and determing the effect of honey on other antimicrobial groups. 225 Table 4.2: Comparison between previous studies and current study on MIC of different honeys including manuka honey against six bacteria species. MIC % (w/v) previous studies Manuka honey Acinetobacter E.coli Klebsiella Other honey Authors N/A 8.1±1.5 (Blair et al., 2009) 12.5 11.25 (Tan et al., 2009) N/A 6-8 (George & Cutting 2007)* N/A 7.5±0.8 (Blair et al., 2009) 17.5 22.5 (Tan et al., 2009) 10 20 (Lusby et al., 2005) 12.5 12.5 (Sherlock et al., 2010)* N/A 6-8 (George & Cutting 2007)* N/A 13±2.4 (Blair et al., 2009) <20 <20 (Lusby et al., 2005) N/A 6-8 (George & Cutting 2007)* Comments MIC % (w/v) this study Manuka honey Omani honey (OH) OH-B OH-C OH-D OH-F 7.17± 0.7 16.6± 2 18.1± 1.6 20.5± 2.4 17.6± 1.9 Omani honey has higher MIC than medihoney, tualang and some Australian honey 10.4± 1.5 18.8± 1.3 19.4±1 23.6±2 19.6±1.8 OH has lower MIC than tualang and some Australian honey 11.7±1 .3 17.2±3 18.5±1.7 22± 2 18± 1.9 OH has lower MIC than some Australian honey Continue from Table 4.1 226 MIC % (w/v) Previous studies Manuka honey Citrobacter Enterobacter Serratia Other honey Authors N/A 9.1±3 (Blair et al., 2009) 10 20 (Lusby et al., 2005) N/A 11.7±1.8 (Blair et al., 2009) 20 25 (Tan et al., 2009) 10 20 (Lusby et al., 2005) N/A 6 (George & Cutting 2007)* N/A 14.8±0.5 (Blair et al., 2009) 0 0 (Lusby et al., 2005) Comments MIC % (w/v) this study Manuka honey Omani honey (OH) OH-B OH-C OH-D OH-F 9.7± 0.8 18.1±2.6 15.8±2.1 26 ± 2.5 16.1± 2.3 OH has lower MIC than some Australian honey 10.1± 1.7 21.6±0.9 20.1±1.7 26.4±2.9 20±1.8 OH has same activity as Australian honey and lower MIC than tualang honey but higher than medihoney 13.3± 1.7 20.2± 1.9 20.2± 1.2 >28 17± 2.8 OH has higher MIC than medihoney N/A (not available) Blair et al., 2009 used medihoney (Australia) by agar incorporation method (%w/v), Tan et al., 2009 used local tualang honey (Malaysian) by broth dilution method (%w/v), Lusby et al., 2005 used some Australian honey by agar incorporation (%w/v), Sherlock et al., 2010 used manuka and ulmo honey by microtitire plate (% v/v). George & Cutting 2007 used medihoney (Australia) by agar incorporation method (%v/v). 227 Figure 4.1: Mean MIC and MBC (%w/v) for 30 Acinetobacter strain against 5 types of honey Susceptibility of 30 Acinetobacter strains against 5 types of honey % bacterial inhibition 25 20 18.4 15 18.1 16.6 10 19.2 20.5 21.8 17.6 17.8 11 7.17 5 0 MH-A OH-B OH-C OH-G OH-F Honey types Mean MIC (W/V%) Mean MBC (W/V%) Figure 4.2: Mean MIC and MBC (%w/v) for 12 Klebsiella strain against 5 types of honey Susceptibility of12 Klebsiella strains against 5 types of honey 30 % bacterial inhibition 25 25 22 20 17.2 15 10 11.7 18.5 19.2 18.8 20.8 18 12.9 5 0 MH- A OH-B OH-C OH-G Honey types Mean MIC (W/V%) 228 Mean MBC (W/V%) OH-F Figure 4.3: Mean MIC and MBC (%w/v) for 10 E.coli strain against 5 types of honey Susceptibility of 10 E.coli strains against 5 types of honey 30 % bacterial inhibition 25 23.6 20 18.8 19.8 25 19.4 20 19.6 20.8 15 10 10.4 10.9 5 0 MH- A OH-B OH-C OH-G OH-F Honey type Mean MIC (W/V%) Mean MBC (W/V%) Figure 4.4: Mean MIC and MBC (%w/v) for 12 Citrobacter strain against 5 types of honey % bacterial inhibition 30 Susceptibility of 12 Citrobacter strains against 5 types of honey 25 26 27.5 20 18.1 18.5 15 18.3 17.8 16.1 15.8 13.3 10 9.7 5 0 MH- A OH-B OH-C OH-G Honey type Mean MIC (W/V%) 229 Mean MBC (W/V%) OH-F Figure 4.5 Mean MIC and MBC (%w/v) for 15 Enterobacter strain against 5 types of honey Susceptibility of 15 Enterobacter strains against 5 types of honey % bacterial inhibition 30 25 26.4 20 21.6 22.9 28 22.5 22.2 20.1 20 15 13.1 10 10.1 5 0 MH- A OH-B OH-C OH-G OH-F Honey type Mean MIC (W/V%) Mean MBC (W/V%) Figure 4.6: Mean MIC and MBC (%w/v) for 8 Serratia strain against 5 types of honey Susceptibility of 8 Serratia strains against 5 types of honey % bacterial inhibition 30 28 28 25 23.75 20 20.2 23.7 20.2 17 15 10 21.7 17 13.3 5 0 MH- A OH-B OH-C OH-G Honey type Mean MIC (W/V%) 230 Mean MBC (W/V%) OH-F 4.4 Inhibition of test organisms by manuka honey using time kill curve assay Time-kill curve studies are used to measure the killing rate of organism by antibiotics using time and concentration. Total cell count is define as the total number of both dead and living cells in the a sample, whereas total viable count (TVC) is define as the number of living cells (Singleton 2004). A T test analysis was applied to establish the statistical difference in cell count between honey treated cells and untreated cells in the selected species under study. P values of less than 0.05 were considered to be statistically significant. A bactericidal activity is defined as in vitro activity of 3 log reduction in the cfu/ml or 99.9% killing over a specific period of time (Shrivastava et al., 2009). Killing measurement was made in this study by the actual decrease in viable counts at 5 h for each species. To maintain and minimize the impact of time- kill variables on test results several factors should be considered when performing time-kill studies. These variations affect the results of the assay and/or interpretation of the results. These factors are: first, the initial or starting inoculum of (104-106 cfu/ml) should be applied. Second, the samples should be incubated at 37°C in shaking water bath. Third, the assay should be continued up to 24 h (Klepser et al., 1998). In this study all these conditions were applied in the time-kill assays and there were significant differences between treated and untreated honey samples (P<0.05) (Table 3.25). 231 Addition of honey to an exponential phase culture leads to an obvious reduction for bactericidal population over a period of time (Fig. 3.10 to 3.15). E.coli and Serratia showed reductions in population of 1.97 and 1.87 log10 cfu/ml respectively (99% growth inhibition) within 5 h. However, Citrobacter was inhibited faster because it exhibited the highest reduction in population than other species tested within 5 h with > 99.9% killing rate (it exceeded 3 log10 cfu/ml reduction). The initial concentration of Acinetobacter and Enterobacter were 7 and 7.74 log10 cfu/ml and were reduced to 5.6 and 6.17 log10 cfu/ml respectively within 5 h exposure to manuka honey. These isolates were considered to be the least susceptible species among those tested here (Table 3.24). This study has therefore shown that manuka honey exhibited bactericidal activity within 5 hours. 4.5 Effect of honey on bacterial structure: Shapes of various bacteria can be observed by light microscopy, including cocci, rods, spiral or cubes. The development of electron microscopes provides new insights into bacterial ultrastructural studies and bacterial organisation. Scanning electron microscopy (SEM) provides a three-dimensional view of cellular structures and information about their surface topography. Transmission electron microscopy (TEM) examines the external and internal bacterial structures (Hobot 2002). Details of surface structures and bacterial morphology aid to study the action of various drugs on bacteria. The mechanism of antimicrobial effects of honey is not yet fully understood. The effects of honey on bacteria could be complicated because of the complexity of 232 honey chemistry. Nevertheless, observation of the bacterial structures and morphological variation present valuable knowledge of complete understanding of antimicrobial action of honey on bacteria. From the EM images of the selected isolates all species undergo morphological changes after exposure to honey, however the nature of changes seen was different in each species. Primary research on the action of manuka honey on Gram positive and negative bacteria using electron microscopy sequentially identifying the mode of action and the target site was initiated by research team at UWIC. Manuka honey with Staphylococcus aureus affected the cell division process by the production of septated cells which were unable to complete cell division (Henriques et al., 2009). However, cell destruction and lysis were observed in Pseudomonas aeruginosa which affected the structure of the cell wall (Henriques et al., 2009, 2010). It was therefore documented that both species responded differently to certain concentration of manuka honey. Typical prokaryotic bacterial structure consists of a cell wall, cytoplasmic membrane, ribosomes, inclusions, chromosome, plasmids, pili or fimbrie, and possibly a capsule. Each structure has a specific function in regulating nutrition and protection processes (Hobot 2002). Due to previous observations on Pseudomonas aeruginosa which demonstrated that the cell surface was markedly changed by exposure to honey (Henriques et al., 2010), it seemed logical to concentrate on the outer layer of the Gram negative bacteria studied here, especially the cell wall and cytoplasmic membrane. The cell wall of Gram negative bacteria is important for maintaining the bacterial shape. It allows for the passage of the macromolecules from the outside environment 233 to the cytoplasmic membrane to the cytoplasm. If the cell wall is ruptured or damaged, the cytoplasmic contents may be lost and eventually cause lysis of bacteria (Sussman 2002). The cell wall consists of an outer membrane layer and inner peptidoglycan layer. The important component of the outer membrane is a group of proteins referred to as porins that permit the passage of small macromolecules, such as glucose or maltose to the cell interior. These porins can open or close their pores under cellular control. The peptidoglycan (murein) is responsible for maintaining the cell shape and confers rigidity. It also prevents the osmotic pressure of the cytoplasm from bursting the cell and is involved in cell division (Konig et al., 2010). The structure of bacterial cells exposed to inhibitory concentrations of manuka honey (2x MIC values) was compared to untreated cells using scanning electron microscopy. The cells were collected in exponential growth phase where the cell growth are fast and most of the proteins and enzymes are produced in that phase (Madigan et al., 2009) which could be an indication of target site of the antimicrobial action of honey. Images of treated Acinetobacter suggested increased cellular debris which is an indication of cell lyses. However, the most remarkable change was increased formation of constrictions suggesting septa in the individual cell (four septa in each cell) (Fig 3.29). Instead of cells dividing by binary fission they seemed to undergo multiple fission without cell separation, which normally only occurs in eukaryotic cells. It could be the cells attempt to adapt to the high exposure of osmotic concentration as a kind of stress response. However, after 1 h exposure to honey onward the cells become significantly shorter compared to untreated cells which led to a decrease in cellular volume (p = 0.0216). 234 In TEM, the cell membrane was interrupted and septated cells were also observed with honey. The presence of dark areas in some cells that could be mineral deposit also evidences cells abnormalities (Fig 3.55). In hypertonic solution (in this case honey) water molecules move from low concentration (inside bacteria) to high concentration and this results in decreased internal pressure and shrinkage of cells. In this case the high sugar concentration which is believed to aid the antimicrobial effect of honey causes noticeable membrane damage. In addition the minimum pH limit for most organisms to be viable is pH 5. pH value below this level may inhibit the metabolism of most enzymes, alter fatty acids that responsible for cell wall synthesis and protein denaturation may also occur which consequently leads to cell damage (Booth 1985; Cotter and Hill 2003). This could reduce the size of bacterial cells and lead to decrease cell volume. This may have been the reason why a significant decrease in cells size of Acinetobacter from 1 to 3 h exposed to 20% (w/v) manuka honey compared to untreated honey (Table 3. 26) was noted. In normal division the size and volume of cells are increased before cell separate to form new daughter cells but the opposite appears to happen here. Acinetobacter cells in cultures exposed to honey were shortened and filamented, suggesting that incomplete cell division had occurred. The total number of culturable cells decreased immediately after exposure to honey. This was also confirmed by the data from time to kill curves experiments (Fig 3.10). In SEM images of E.coli treated cells, aggregation of cells is seen with strands of material extending from honey treated cells (Fig 3.35). The most noticeable change was seen in TEM images where the intracellular components leaked out from the honey treated cells (cell lysed) due to loss of membrane integrity and formed empty 235 cells (Fig 3.59). Some treated cells also demonstrated irregular shapes with relatively less electron dense material compared to untreated cells and the cytoplasmic material had contracted away from the cell boundaries. All of these changes support the suggestion of an effect of honey on bacterial cell membrane as a target site in E.coli. Lysis of cells due to alteration in membrane integrity prevents bacterial growth and multiplication and consequently inhibits normal cells division (Cotter and Hill 2003). Also, by supporting the results from time kill study, the total number of cells were decreased as shown by growth curve (Fig 3.5) and number of culturable cells were also decreased (Fig 3.11). Septated cells were not observed in either SEM or TEM images. However, it does not mean that it was not present, it was possible that it might have been failed to be spotted through the ultrathin sectioning or due to improper orientation of the section which reduce the chance of septum location. However, cells of Klebsiella treated with manuka and Omani honey had a noticeably rougher cell surface, compared to untreated cells (Fig 3.36). In addition, changes in cells size significantly increased for both types of honeys (p= < 0.05). This suggests that outer cell surfaces might have been affected by honey (Fig 3.39b,c,d, & Fig 3.41b,c,d) Using SEM with Citrobacter exposed to 20% manuka honey revealed a significant change in cell size between untreated and treated honey samples at 30, 90 and 180 minutes time point (p = ≤ 0.05). In addition, the surface of bacterial cells becomes rougher, perhaps as a result of outer membrane damage (Fig 3.47). The possibility of formation of pore was observed by black areas in the cell surface (Fig 3.49b). This indicates that honey could enter the cells though that pore and cause cell destruction. The total number of culturable cells showed marked decrease in colony forming unit 236 with more than (3-log10 reduction). This means 99.9% of the Citrobacter population were killed. Citrobacter therefore gave the greatest bactericidal response compared to the other species tested (Table 3.24). SEM images of Enterobacter showed increased formation of a net like structure in honey treated cells after 30 minutes of exposure compared to the background of the untreated cells (Fig 3.45). This could be formed from lysed cells or from leaked cellular products. Thus comparable to expectation from time- kill curve (Fig 3.14), the total number of culturable cell count decreased immediately with time after exposure to honey. There were no significant difference in cell size between untreated and treated honey samples at each time point tested (P > 0.05) (Table 3.25) Serratia treated with 30% manuka honey revealed some changes in cell surface and increased incidence of cellular debris as a result of cell lyses (Fig 3.51). Increased elongated cells was significant (P = 0.0002) (Fig 3.53). No septa were observed in this stage. 237 Table 4.3: Summary of the growth inhibition, killing rate and ultra-structure changes in EM for six species selected after exposure to 2x MIC (%w/v) of manuka honey: Honey Conc. 2xMIC Growth inhibition by MIC % (w/v) Killing rate by time-kill* Acinetobacter 20% 9 E.coli 30% Klebsiella SEM TEM Site of cell change Septa formation Debris (cell lysed) 6 Shorter cells with clumps High High loss of cell membrane, cellular debris, septated cells and black deposit 13 2 Extended strand materials around the cells Not seen Not seen Excess loss of membrane integrity, irregular shape, empty cells and less electron dense 30% 13 4 Cell size, rough surface Few Not seen Not done Citrobacter 20% 11 1 Cell size, rough surface, black deposit Not seen Not seen Not done Enterobacter 30% 13 5 No change Few High Not done Serratia 30% 15 3 Cell surface & size Not seen Moderate Not done Killing rate by time-kill curve* (1-6) = (1) killing at faster rate, (6) slowest killing rate 238 To date there is little research on the effect of honey on multidrug resistant Acinetobatcter and Enterobacteriaceae in general. However, no medical research was conducted up to electron microscope level to find out the ultra-structural change of these species against honey using EM in particular. It is difficult therefore to prove the mechanism of the inhibitory effects of honey on bacteria using this approach alone. A proteomic approach is likely to give more useful information on the proteins that are affected by honey, but there was insufficient time to develop the protocols in this study. However, in manuka honey cellular protein extraction of Gram positive cocci (Staph aureus) was recently studied using 2-D electrophoresis. The cells showed down regulation in protein synthesis after exposure to 10% (w/v) manuka honey. The protein spot was identified using MALDI-TOF-MS techniques as universal stress protein A (Jenkins et al., 2011). This will give an expectation on the different proteomic profile of honey treated Gram negative bacteria. That same research on the mechanisms of action of manuka honey on MRSA stated that the manuka honey affected the process of cell division during septa formation. It was recognised that decreased level of FtsZ enzyme, which is involved in cell division, leads to disruption of the cell cycle after honey treatment and caused cell death (Jenkins et al., 2011). Nonetheless, microarrays would also give valuable information on how gene expression in Gram negative bacteria is affected by honey. Some researchers suggested that the antimicrobial activity was due to the presence of high amount of tetracycline derivatives, peroxidases, phenols, amylases, ascorbic acid and fatty acid (Nzeako and Hamdi 2000). Nevertheless, this pilot project has clearly shown that even the most antibiotic-resistance bacteria succumb to relatively 239 low concentrations of honey in the laboratory and clinical studies are urgently needed. The most feasible suggestion on the action of honey on Gram negative bacteria is the alteration in cell wall or cell membrane integrity. The observation of cell lysis suggested that there were significant changes in cell wall and plasma membrane integrity (possibly by increased formation of pores) allowing honey to enter cells and cellular contents to escape (Table 4.3). Then the action of antioxidant, phenolic acid, MGO and other factors may be expected to contribute to the process of cell destruction, but the extent of each influence is as yet unknown. Another line of evidence to support this suggestion is that honey can act upon the structure of a biological membrane to disrupt it enough to allow the diffusion of protons into a liposome or bacterial cell (Grovell 2006). Very recently, Kwakman and his colleagues who identified the bee defensin-1 for the first time studied the antimicrobial activity of two important honeys (manuka and Revamil honeys) against different species. Also, the quantity of bee defensin-1, MGO and H2O2 were analysed for both honeys. It was found Revamil killed bacteria rapidly because of unique presence of bee defensin-1 and H2O2 which create ion channels in lipid bilayers and increase permeability of outer and inner biological membranes. Where as manuka honey retained its activity even with higher dilution, the presence of high sugar, low pH, high concentration of MGO (44 fold higher than Revamil) and other cationic and non- cationic bactericidal factors aid in the bactericidal activity of manuka honey (Kwakman et al., 2011). Defensins are small, cysteine rich broad spectrum antibacterial peptides found in human neutrophils. Their antimicrobial activity on Gram negative and Gram positive bacteria, Mycobacteria, fungi and enveloped virus was documented in-vitro (Kagan et al., 1994). 240 The effect of defensin peptide was first reported morphologically on Staph. aureus using TEM and caused major changes in the cytoplasmic membrane (Shimoda et al., 1995). It is known to increase permeability of the cell wall in Gram negative bacteria, causing cytoplasmic contents to leak out. Its effect on E.coli causes damage of outer and inner membranes by rapid permeabilization of the plasma membrane leading to cell death (Lichtenstein 1991). Defensin was therefore proven to cause destruction in the biological membrane. However its effect on human tumour cells revealed that the primary target is the plasma membrane. Generally, antibacterial peptides affect several target sites on bacteria such as binding to intracellular compounds (DNA, RNA and proteins) or by bacterial enzymes inhibition (Patrzykat et al., 2002). The evidence that the effect of bee defensin-1 is similar to human defensin will provide a good indication in the mechanism of action of honey containing that peptide on bacteria. Therefore, honey contains compounds that inhibit bacteria to develop resistance. Until now no report demonstrated that honey can develop resistance even in excessive use (Blair et al., 2009; Cooper et al., 2010) The statistics of war wound infection in wounded soldiers during military operations (2003-2005) in Iraq had increased compared to previous operation in Korea, Vietnam and the Persian Gulf. This has caused increase prevalence of MDR Acinetobacter calcoaceticus-baumannii complex isolated from wound and subsequently caused bacteraemia (Murray et al., 2008). Most investigations by medical military research suggested that this is a nosocomial infection but their source was not known. Despite careful procedure in the selection of antibiotic therapy in such outbreaks there will be limited options of drug therapy available to 241 treat this infection (Davis et al., 2005). In addition global increase in antibiotic resistant organisms causes major problems in controlling the emergence of resistance (Hawkey and Jones 2009). Currently an increase of aggressive situations worldwide i.e war in Libya and earthquake in Japan may cause increased prevalence of resistant strain of Acinetobacter. This highlights the necessirly to develop alternative treatments to eliminate such infections. As honey has several effective properties in wound healing including anti-inflammatory properties, providing moist environment around the wound, non toxic, reduce exudates and oedema, painless, debriding agent and ease of application (Molan 2006). In addition rapid wound healing due to honey treatment reduces hospital stays especially in chronic wound patients and reduces the time required for doctors and nurses until the wound heals. This results in a decrease in financial cost of the health care system. Thus it could be used as a perfect treatment. The main conclusion obtained from this study is that the antimicrobial effect of honey is most probably due to several factors controlling its activity. Thus the mechanisms of action of honey could have various target sites such as proteins, enzymes and DNA. 242 4.6 Further investigations: There is much evidence of antibacterial activity of using honey in the topical treatment of infected wounds, however further assumptions needs to be given to its systemic application and therapeutic properties in order to improve the use of this product in clinical and systemic infections especially with increase prevalence of multi drug resistant bacteria. This pilot study of the Omani honeys needs more comprehensive research with different types of honeys collected from different parts in Oman in order to establish whether all honeys possess both antibacterial and healing properties. This could improve the identification of the most appropriate type of honey to be used for wound care in Oman particularly after isolation of highly resistant NDM gene of Klebsiella pneumonia for the first time in Oman (Poirel et al., 2010). Also using an advanced method to identify and study the nature of other components in Omani honey could aid its antimicrobial effect such as, MGO, glucose oxidase enzyme, antioxidant and bee defensin-1. Further study on the idenfication of bee defensin-1 in other honey samples to determine its effect on Gram postive and negative bacteria and to prove its simillarity effect as human defensin is needed. Omani honeys could be tested for bee defensin. Further study on the action of different types of honey to identify the intracellular morphological changes using electron microscopy is required. Investigation of the molecules that leaked out from the cells after exposure to honey such as DNA, potassium ions or other cell organell using leakage study. Furthermore, extensive 243 study on the alteration of Gram negative bacterial cell wall structure after honey treatment by invistigating the synthesis and degradation of murien and/or expression of murein hydrolase and peptidoglycan hydrolase enzymes is needed. These enzymes are involved in cell cycle by controlling the breakdown of cell wall components before cytokinesis and cell separation occurs. However, in Gram positive (MRSA) these enzymes showed reduced activity after honey treatment (Jenkins et al., 2011). By investigating these effects, a better understanding of the effect of manuka honey on cell cycle of Gram negative bacterial will be achieved. Large scale analysis on proteome expression using 2-D electrophoresis and kinetics of RNA using radioactive isotopes in different organisms, provides important information about the mode of action. Another method using MALDI-TOF- MS techniques for the identity of protein after the detetcion of down regulated or upregulated protiens in the proteome analysis in 2-D electrophoresis. Microarray methods could be used to explain the reproducibility of gene expression on honey treated cells compared to non honey treated cells. To determine whether honey has simillar activity in vivo, further clinical trials on wounds infected with MDR Acinetobacter or other ESBLs and treated with different types of honey must be conducted. With the current difficulties in treating ESBL infections in wounds, honey does seem to offer real potential in eradicating these pathogens. 244 Chapter 5 References 245 Adams, C. J., Boult, C. H., Deadman, B. J., Farr, J. M., Grainger, M. N. C., Manley-Harris M., Snow, M. 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