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Abstract Previous studies have investigated the relationship between blood type and pancreatic cancer, but little research has been done to determine how blood type correlates with the development of colon cancer. The fucosyltransferase2 (FUT2) gene is involved in the production and secretion of ABH blood group antigens along with mucin into the lumen of the colorectal tract. These antigens serve as carbon sources and anchoring sites for bacteria that are normally present in our gut and aid with digestion. However, a mutation in the FUT2 gene inhibits secretion of the ABH blood group antigens. The absence of these antigens could lead to a decrease in the number of normal bacteria in the gut, in turn allowing pathogenic, potentially cancer-causing, bacteria to colonize the colorectal tract. Therefore, we examined the relationship between the rs516246 SNP in the FUT2 gene, the microbial composition of the gut and the presence of colorectal adenomas (CRAs), which are precursors to colorectal cancer. We hypothesized that individuals with the variant allele (T) of the rs516246 SNP would be more likely to have CRAs and would have different bacterial profiles than those with the wildtype allele (C). We genotyped the rs516246 SNP and sequenced bacterial DNA in over 600 cases and controls using genomic DNA extracted from blood and biopsies respectively. We found no significant overall correlation between the variant genotype and the risk of developing CRAs, but that the variant genotype does affect the bacterial profile. Genotype was also linked to the level of expression of inflammation and mucin genes. It was expected that a change in the mucin secreted would increase inflammation in epithelial cells of the colorectal tract, because the mucus layer covering epithelial cells may be less capable of preventing pathogenic bacteria from penetrating the cells. While the presence of a T allele was significantly associated with increased expression of TLR4, which activates the immune system, it was also significantly associated 1 with decreased expression of the inflammation marker IL-10. Our findings suggested that the rs516246 FUT2 variant alters bacterial composition and inflammation of the colorectal tract. Further studies are needed in order to analyze additional FUT2 SNPs and confirm their role in colorectal adenomas and cancer. Introduction Colorectal cancer is one of the leading causes of cancer death worldwide (Torre et al., 2015) and the third leading cause of cancer death in the United States, in both females and males (American Cancer Society, 2014). This disease usually progresses slowly, and the transition from normal epithelium to adenocarcinoma (Figure 1) can sometimes take 20 years (American Cancer Society, 2014). One of the stages of colorectal cancer is the adenoma (Lao et al., 2011), which was the focus of this study. Figure 1. The progression of colorectal cancer from normal gut epithelium to polyps/adenomas, to cancer. Source: (Lao et al., 2011) Colorectal cancer can be hereditary, but it can also affect individuals with no family history of the disease, as in sporadic colorectal cancer (Haghighi et al., 2009). Risk factors for sporadic colorectal cancer include lifestyle choices such as physical inactivity, smoking (Torre et al., 2015) and high meat intake (Roberts-Thomson et al., 1999). The impact that these environmental factors have on an individual can vary depending on the genetic polymorphisms 2 that are present (Roberts-Thomson et al., 1999). One genetic polymorphism that could affect the impact of environmental factors is the rs516246 SNP in the fucosyltransferase 2 (FUT2) gene, which is involved in the production of ABH blood group antigens (Jaff, 2010). It has been suggested that blood type in humans is associated with the risk of developing various types of cancer. Wolpin et al. (2009) reported that non-O blood group is related to an increased risk of pancreatic cancer. A later study found that the overall risk of developing cancer is lower in those with blood group O, while the greatest risk of developing cancer is associated with blood group A (Zhang et al., 2014). Blood type data from individuals with various types of cancer, including pancreatic, breast, colorectal, ovarian and nasopharyngeal, was used in this study (Zhang et al., 2014). Two genes that are involved in the production of ABH blood group antigens are fucosyltransferase 1 (FUT1) and FUT2 (Jaff, 2010). FUT1 is an enzyme that is responsible for producing ABH antigens that are presented on the surfaces of red blood cells, while FUT2 is an enzyme that is responsible for the production and secretion of ABH antigens into bodily fluids, such as the mucus of the gut (Wacklin et al., 2011). The H antigens produced by the FUT1 and FUT2 enzymes are precursors for the A and B antigens (Jaff, 2010). These blood group antigens that are secreted, along with mucin, into the lumen of the colon are oligosaccharides that serve as carbon sources and anchoring sites for gut bacteria (Mäkivuokko et al., 2012). Non-secretors, or those with a genetic mutation in the FUT2 gene, do not secrete ABH blood group antigens, so these antigens would not be present in the colorectal tract (Jaff, 2010). It has been found that beneficial bacteria, such as Bifidobacteria, are more abundant in the colorectal tracts of secretors than non-secretors (Wacklin et al., 2011), which suggests that other, pathogenic bacteria may colonize the gut of non-secretors. These pathogenic bacteria may also be better able to infect epithelial cells of the colorectal tract in non-secretors because a lack 3 of secretion of ABH antigens would change the composition of the protective mucus layer that lines the lumen of the gut (Tong et al., 2014). Therefore, non-secretors may be at a higher risk for colorectal cancer, as research has indicated that the gut microbiome may play a highly significant role in the development of this disease (Louis et al., 2014). The rs516246 SNP in the FUT2 gene is a good indicator of the secretor status of an individual. It can be inferred that those with the wildtype cytosine (C) at the site of this SNP in both alleles have the secretor status, while those with the variant thymine (T) at this same site in both alleles have the non-secretor status (Okunola et al., 2015). Those who are heterozygous and have a C at the rs516246 SNP in one allele and a T at this SNP in the other allele most likely experience some secretion of blood group antigens. We hypothesized that the rs516246 SNP is associated with the risk of developing colorectal adenomas and that this association may be modified by bacteria, which utilize the antigens produced by FUT2. In addition, the differences in the levels of secretion of these antigens into the mucin of the gut may affect levels of inflammation caused by pathogenic bacteria in the gut. In this study we examined the relationship between the FUT2 C>T polymorphism (rs516246), microbial gut composition, levels of gene expression of inflammatory markers (Interleukin 10, Toll-Like Receptor 4, Mucin 2) and the presence of colorectal adenomas. Methods Study Population The study population consisted of 628 consenting subjects between the ages of 50 and 80 who were undergoing screening colonoscopy at UNC Hospitals as part of the Diet and Health 4 Study V (DHSV). The study was approved by the UNC School of Medicine IRB. Rectal biopsies and blood samples used in this study were obtained during the procedure. After collection, blood was centrifuged in order to separate the plasma, buffy coat and red blood cells. The buffy coat containing the white blood cells was collected and stored at -80°C until use in the current study. DNA Extraction from Buffy Coat DNA Extraction was performed using the Gentra Puregene Blood Kit (Qiagen) according to the kit protocol. Buffy coat samples were thawed at 37 °C, after which residual red blood cells were lysed with Red Blood Cell Lysis solution. The white blood cells were then pelleted by centrifugation and lysed with Cell Lysis solution in order to isolate genomic DNA. The solution was treated with RNase A Solution to achieve RNA-free DNA. Proteins were separated from the DNA with Protein Precipitation Solution, and isopropanol was added to each sample to coalesce the DNA strands. The DNA was then pelleted, dried and later resuspended in DNA Hydration Solution. The concentration of DNA obtained from each sample was measured using a NanoDrop Spectrophotometer, and the DNA was stored at -4 °C. Allelic Discrimination Assay Individual samples were genotyped using a TaqMan SNP Genotyping Assay (ThermoFisher Scientific). A total of 10 ng of DNA from each sample were added to an individual well of a 384-well plate and combined with TaqMan Genotyping Master Mix (ThermoFisher Scientific) and FUT2-specific primers and probes to target the rs516246 SNP. The plate was loaded onto a Bio-Rad CFX Real-Time PCR machine for one cycle of 95 °C for 10 minutes, followed by 40 cycles of 95 °C for 10 seconds and 60 °C for 60 seconds. A plate 5 read was performed upon completion of the run. Each of the two alleles in the FUT2 gene of each DNA sample were determined by Bio-Rad CFX Manager software. One possible allele contained a C at the rs516246 SNP, and the other possible allele contained a T at the position of this SNP. The two different alleles were distinguished through the use of probes, which were small strands of nucleotides attached to a fluorescent reporter dye molecule and a quencher dye molecule (Livak 1999). While attached to the probe, the level of fluorescence of the fluorescent reporter dye molecule was kept low by the quencher dye molecule (Livak 1999). Only when the fluorescent reporter dye molecule was detached from the probe and separated from the quencher dye molecule was it able to emit a high level of fluorescence (Figure 2) (Livak 1999). VIC reporter dye was attached to probe one, which was complementary to the C allele. FAM reporter dye was attached to probe two, which was complementary to the T allele. During PCR, these probes attached to the site of the rs512646 SNP in their complementary allele. Forward and reverse primers then attached to either end of the region of DNA containing the SNP of interest, and Taq polymerase added on nucleotides to the primers (Figure 2). When the Taq polymerase reached the probe, the fluorescent reporter dye molecule was cleaved, causing the fluorescence emitted by this molecule to increase in intensity. In cases where the complementary sequence to one of the probes was not present, such as in homozygotes for the rs516246 SNP, that particular probe did not bind to the DNA. Its reporter dye molecule remained attached to the probe, and it did not fluoresce at a high level. The amount of fluorescence reported by each of the two dye molecules in each individual well was measured during PCR. The level of fluorescence of each dye molecule corresponded to the frequency of each allele. In this way the genotype of each individual sample was determined to be either homozygous for the wildtype nucleotide, homozygous for the variant nucleotide or heterozygous at the location of the rs516246 SNP. 6 Figure 2. Cleavage of the fluorescent reporter dye during an allelic discrimination assay. Source: (Livak, 1999) Bacterial DNA Extraction and Illumina Sequencing Both human and bacterial DNA were extracted from colorectal biopsy samples using a Qiagen DNeasy Blood and Tissue Kit with a modified kit protocol that included lysozyme and bead-beating (McCoy et al., 2013). The Illumina library was then created using two different PCR reactions. First-step PCR (PCR1) was performed using primers designed to amplify the V2 region of the 16S bacterial rRNA gene. For PCR1, one reaction was performed for each sample using Phusion HighFidelity Master Mix (Life Technologies, Carlsbad, CA. PCR1 product was diluted 20-fold for use as a template for second-step PCR (PCR2). PCR2 primers contained an Illumina index barcode sequence, Illumina adapter sequence and a tag sequence. There were two sets of PCR2 primers, and each PCR2 reaction received one 7 of each, resulting in a dual-indexed product. One reaction was performed for each sample using Phusion High-Fidelity Master Mix. PCR product was visualized on an E-Gel 96 (Life Technologies, Carlsbad, CA) to check all samples for amplification. All samples with positive amplification were included in the library. All samples were normalized to 25 ng/µl using the SequalPrep Normalization Kit (Life Technologies, Carlsbad, CA). The library was cleaned using AxyPrep Mag Beads (Fadrosh, 2014). Bacterial sequences were filtered for quality control and processed in Qiime (Caporaso, 2010). Expression of Inflammatory Markers Human RNA was extracted from colorectal biopsy samples using a Qiagen RNeasy Mini Kit. The RNA was loaded into a chip and run on the Agilent 2100 bioanalyzer using the Agilent 6000 Nano Kit, in order to determine the concentration and fragment size of the RNA in each sample. The RNA for each sample was then diluted to a concentration of 500 ng per 10 ΞΌl. A Promega RQ1 RNase-Free DNase Kit was used to digest any DNA contaminants in the RNA samples. Reverse transcription PCR was performed using an Invitrogen Cloned AMV FirstStrand cDNA Synthesis Kit in order to create cDNA from the RNA samples. The cDNA was used as a template for real time PCR, along with a Qiagen RT² qPCR Primer Assay, which included primers specific to the genes of interest. The Primer Assay was mixed with template cDNA and ππππ ππ Universal SYBR® Green and run on a Bio-Rad CFX384 Real Time PCR Detection System (Kang et al., 2013). Statistical Analysis Comparisons of general characteristics of the study population, genotype distribution, 8 bacterial abundance and gene expression between adenoma cases and controls with no adenomas were assessed by t-tests for continuous variables and chi squared test for categorical variables. Multivariate analysis of bacteria data such as cluster analysis and non-multidimensional scaling was performed using PRIMER-7 software as previously described (Shen et al., 2010). Multivariate analysis permits the examination of relationships among multiple variables at the same time. P-values <0.05 were deemed significant after adjustment for multiple comparisons. Results The purpose of the experiments described above was to determine if there is a correlation between the rs516246 SNP, the types of bacteria present in the gut, the level of inflammation in the gut and the presence of colorectal adenomas. The bacterial profile of the gut was determined through the use of Illumina sequencing of extracted bacterial DNA, and the level of inflammation of the gut was determined by measuring the level of expression of certain genes involved in inflammation. The results of these experiments, along with the general characteristics of the study population are given below. The characteristics of subjects according to case/control status are given in Table 1. Race, body mass index (BMI) and calories were evenly distributed among cases and controls, however, age, sex and waist-hip ratio differed significantly between these two groups. There was a higher proportion of males among subjects with colorectal adenomas, and these subjects were also older and had a higher waist-hip ratio than those who did not present with colorectal adenomas. 9 Table 1. Descriptive Characteristics of Study Participants General Characteristics Case (n=190) Control (n=438) P-value Age (mean, SE) 56.5 (0.5) 54.9 (0.3) 0.005 Sex (% Male) 110 (58) 188 (43) 0.0006 Race (% White) 164 (86) 377 (86) 0.94 Waist-Hip Ratio 0.937 (0.006) 0.906 (0.004) <0.0001 27.7 (0.4) 27.0 (0.3) 0.11 2,045 (66) 1,949 (39) 0.21 (mean, SE) Body Mass Index (mean, SE) Calories (mean, SE) The genotype distributions of FUT2 were in Hardy-Weinberg equilibrium, as determined by the equation p² + 2pq + q² = 1, but there was no significant overall association between FUT2 genotype and presence of colorectal adenomas. The distribution of the CC, CT and TT genotypes was 29%, 49% and 22% respectively for cases and 28%, 51% and 21% respectively for controls. However, there were differences in bacterial profiles between those with the CC genotype and those with the TT genotype that were borderline significant (P=0.07). As shown in Figures 3a and 3b, the TT genotype is associated with reduced abundance of Ruminococcus (P=0.02) and Dialister (P=0.04) and increased abundance of Eggerthella (P=0.06) compared to the CC genotype. The genera of bacteria analyzed are divided into two graphs based on the scale of the axis that best fits the data. 10 Bacterial Abundance by Genotype 4.5 4 Percent Abundance 3.5 3 2.5 2 1.5 1 0.5 0 Bacteria CC CT TT Figure 3a. The distribution of six genera of bacteria by FUT2 genotype. There was a significant reduction in Dialister (p=0.04) and a borderline significant increase in Eggerthella (p=0.06) from CC to TT. 11 Bacterial Abundance by Genotype 25 Percent Abundance 20 15 10 5 0 Ruminococcus Blautia Bacteria CC CT TT Figure 3b. The distribution of two genera of bacteria by FUT2 genotype. There was a significant reduction in Ruminococcus (p=0.02) from CC to TT. Table 2 displays the relationship between three inflammatory markers, FUT2 genotype at the rs516246 SNP and the presence of colorectal adenomas. In cases, compared to controls, the carriage of the T allele, compared to the CC genotype, was associated with reduced expression levels of Interleukin-10 gene (IL-10), which produces an anti-inflammatory cytokine (Iyer et al., 2012), and increased expression of Toll-Like Receptor 4 gene (TLR4), which produces a protein that activates the innate immune system when bound to a pathogen (Chaudhuri et al., 2013). 12 There was no statistically significant relationship between the Mucin 2 gene (MUC2) and FUT2 genotype. Table 2. Gene Expression Levels of Inflammatory Markers in Relation to FUT2 Genotype Inflammatory Marker IL-10 Genotype Case Control P-Value CC (wildtype) CT TT T allele 0.79 0.64 0.46 0.55 0.63 0.70 0.55 0.66 0.27 0.10 0.46 0.06 MUC2 CC (wildtype) CT TT T allele 1.24 1.02 1.02 1.02 1.20 1.19 1.16 1.19 0.67 0.49 0.40 0.45 TLR4 CC (wildtype) CT TT T allele 1.03 1.19 1.03 1.13 1.0 1.03 0.87 0.95 0.65 0.15 0.05 0.03 Discussion In this study we determined the relationship between a FUT2 polymorphism (rs516246), risk of colorectal adenomas, bacterial composition of the colorectal tract and inflammatory markers. Although previous studies had found a correlation between blood type and pancreatic cancer (Wolpin et al., 2009) and non-secretor status and oral cancer (Ensinck et al., 2013), we did not find any overall association between the rs516246 FUT2 SNP and the risk of developing colorectal adenomas. However, we found that the homozygous variant genotype (TT) is associated with reduced abundance of Ruminococcus and Dialister and increased abundance of Eggerthella compared to the homozygous wildtype genotype (CC). We also found a correlation between the variant T allele, increased expression of TLR4 and decreased expression of IL-10 among cases, compared to controls. 13 Previous studies reported significantly lower levels of Ruminococcus and Dialister in the stool of patients with colorectal cancer compared to healthy individuals (Weir et al., 2013) and high levels of Eggerthella in the gut of colorectal cancer patients (Wang et al., 2012). Therefore, the association between the reduced abundance of the two former genera, the increased abundance of Eggerthella and the variant FUT2 genotype could imply that the rs516246 FUT2 SNP affects the risk of developing colorectal cancer by way of altering the bacterial profile of the gut. Although it is not completely understood how bacteria in the colorectal tract interact with their human host, it is known that variations in the composition of the gut microbiome are present in many diseases (Wu et al., 2015). Not only does FUT2 affect the composition of the gut microbiome, but it also seems to affect the function of these bacteria in the mucosal layer of the colorectal tract (Tong et al., 2014). These functional changes have been shown to be accompanied by inflammation of the intestinal walls (Tong et al., 2014). In this study we found a link between inflammation and the presence of colorectal adenomas. Compared to controls, cases with the variant T allele displayed lower expression levels of the anti-inflammatory gene IL-10 and higher expression levels of the TLR4 gene, which produces a receptor that triggers the innate immunity response when it is bound to a pathogen, than those with the homozygous wildtype genotype (CC). This may suggest that a complex relationship exists between the gut microbiota, intestinal inflammation, FUT2 and colorectal adenomas. Although no overall association was found in this study between the rs516246 FUT2 SNP and the risk of developing colorectal adenomas, that does not discount FUT2 as being an important factor in the progression of colorectal cancer, because this SNP is one of many polymorphisms in the FUT2 gene. Sample size was not an issue in this study (n=628), but if we 14 were not under time constraints, we would have liked to genotype more SNPs within the FUT2 gene. In summary, our findings suggest that the rs516246 FUT2 variant alters bacterial composition and inflammation of the colorectal tract. Further studies are needed in order to analyze additional FUT2 SNPs and confirm their role in colorectal adenomas and cancer. Acknowledgements I would like to thank Dr. Temitope Keku for giving me the opportunity to complete this study, for developing the hypothesis and for her continued support and input throughout the process. I would like to thank Amber McCoy for teaching me all protocols and for completing the bacterial DNA extractions and Illumina sequencing. I would like to thank Winifred Okunlola for extracting and genotyping DNA from almost a third of the samples used in this study. I would like to thank Dr. Joe Galanko for completing the data analysis for this study. I would like to thank Félix Araújo-Pérez and the University of Maryland Institute for Genome Sciences for determining cytokine gene expression in this study. I would like to thank Dr. Blaire Steinwand for serving as my Biology Faculty Sponsor. I wish to acknowledge the Center of Gastrointestinal Biology and Disease in the UNC School of Medicine for providing the research laboratory for this study. This project was supported by the Tom and Elizabeth Long Excellence Fund for Honors administered by Honors Carolina and by grants from the National Institutes of Health NIH R01 CA04468, R01 CA136887 and P30 DK 034987. 15 References American Cancer Society (2014). Colorectal Cancer Facts and Figures 2014-2016. Atlanta: American Cancer Society. Caporaso J, J Kuczynski, et al. (2010). QIIME allows analysis of high-throughput community sequencing data. Nature Methods, 7(5): 335-336. Chaudhuri A, N Wilson, et al. (2013) Host genetic background impacts modulation of the TLR4 pathway by RON in tissue-associated macrophages. Immunology and Cell Biology, 91(7): 451-460. Ensinck M, M Valles, et al. (2013). Expression of the FUT2 gene and CD44 marker in patients with oral lesions. Immunología, 32(4): 123-128. Fadrosh D, B Ma, et al. (2014). An improved dual-indexing approach for multiplexed 16S rRNA gene sequencing on the Illumina MiSeq platform. Microbiome, 2(1): 6. Haghighi MM, M Vahedi, et al. (2009). Comparison of survival between patients with hereditary non polyposis colorectal cancer (HNPCC) and sporadic colorectal cancer. Asian Pacific Journal of Cancer Prevention, 10(3): 497-500. Iyer S, G Cheng (2012). Role of Interleukin 10 Transcriptional Regulation in Inflammation and Autoimmune Disease. Critical Reviews in Immunology, 32(1): 23-63. Jaff MS (2010). Higher frequency of secretor phenotype in O blood group β its benefits in prevention and/or treatment of some diseases. International Journal of Nanomedicine, 5 (1):901-905. 16 Kang M, P Edmundson, et al. (2013). Association of plasma endotoxin, inflammatory cytokines and risk of colorectal adenomas. BMC Cancer, 13: 91. Lao V, W Grady (2011). Epigenetics and Colorectal Cancer. Nature Reviews Gastroenterology and Hepatology, 8(12): 686-700. Livak K (1999). Allelic discrimination using fluorogenic probes and the 5β nuclease assay. Genetic Analysis: Biomolecular Engineering, 14(5-6): 143-149. Louis P, G Hold, H Flint (2014). The gut microbiota, bacterial metabolites and colorectal cancer. Nature Reviews Microbiology, 12(10): 661-672. Mäkivuokko H, S Lahtinen, et al. (2012). Association between the ABO blood group and the human intestinal microbiota composition. BMC Microbiology, 12, 94. McCoy A, F Araújo-Pérez, et al. (2013). Fusobacterium Is Associated with Colorectal Adenomas. PLoS One, 8, e53653. Okunola W, A McCoy, et al. (2015). Association of FUT2 gene variant, gut bacteria and colorectal adenomas. Cancer Research, 75, 4586. Roberts-Thomson IC, WJ Butler, et al. (1999). Meat, metabolic genotypes and risk for colorectal cancer. European Journal of Cancer Prevention, 8(3): 207-211. Shen XJ, JF Rawls, et al. (2010). Molecular characterization of mucosal adherent bacteria and associations with colorectal adenomas. Gut Microbes,1(3):138-147. Torre LA, F Bray, et al. (2015). Global cancer statistics. CA: A Cancer Journal for Clinicians, 65(2): 87-108. 17 Tong M, I McHardy, et al. (2014). Reprogramming of gut microbiome energy metabolism by the FUT2 Crohnβs disease risk polymorphism. International Society for Microbial Ecology Journal, 8, 2193-206. Ürün Y, N Yildirim, et al. (2012). ABO and Rh blood groups and risk of colorectal adenocarcinoma. Asian Pacific Journal of Cancer Prevention, 13(12): 6097-6100. Wacklin P, Mäkivuokko H, et al. (2011). Secretor phenotype (FUT2 gene) is strongly associated with the composition of bifidobacteria in the human intestine. PLOS ONE, 6, e20113. Wang T, G Cai, et al. (2012). Structural segregation of gut microbiota between colorectal cancer patients and healthy volunteers. The International Society for Microbial Ecology Journal, 6, 320-329. Weir T, D Manter, et al. (2013). Stool Microbiome and Metabolome Differences between Colorectal Cancer Patients and Healthy Adults. PLOS ONE, 8, e70803. Wolpin BM, AT Chan, et al. (2009). ABO blood group and the risk of pancreatic cancer. Journal of the National Cancer Institute, 101(6): 424-431. Wu H, V Tremaroli, et al. (2015). Linking Microbiota to Human Diseases: A Systems Biology Perspective. Trends in Endocrinology & Metabolism, 26(12): 758-770. Zhang BL, N He, et al. (2014). ABO blood groups and risk of cancer: a systematic review and meta-analysis. Asian Pacific Journal of Cancer Prevention, 15(11): 4643-4650. 18