* Your assessment is very important for improving the workof artificial intelligence, which forms the content of this project
Download Temeyer 2016 tick salivary cholinesterase
Plant disease resistance wikipedia , lookup
Adoptive cell transfer wikipedia , lookup
Social immunity wikipedia , lookup
Complement system wikipedia , lookup
Sociality and disease transmission wikipedia , lookup
DNA vaccination wikipedia , lookup
Transmission (medicine) wikipedia , lookup
Immunosuppressive drug wikipedia , lookup
Adaptive immune system wikipedia , lookup
Cancer immunotherapy wikipedia , lookup
Molecular mimicry wikipedia , lookup
Immune system wikipedia , lookup
Hygiene hypothesis wikipedia , lookup
Myasthenia gravis wikipedia , lookup
Polyclonal B cell response wikipedia , lookup
Schistosoma mansoni wikipedia , lookup
Innate immune system wikipedia , lookup
Journal of Medical Entomology Advance Access published January 21, 2016 Journal of Medical Entomology, 2016, 1–5 doi: 10.1093/jme/tjv252 Research article Arthropod/Host Interaction, Immunity Tick Salivary Cholinesterase: A Probable Immunomodulator of Host–parasite Interactions Kevin B. Temeyer1 and Alexander P. Tuckow Knipling-Bushland U.S. Livestock Insects Research Laboratory, U.S. Department of Agriculture-Agricultural Research Service, 2700 Fredericksburg Road, Kerrville, Texas 78028 ([email protected]; [email protected]) and 1Corresponding author, e-mail: [email protected] Received 21 September 2015; Accepted 23 December 2015 Abstract Key words: cholinesterase, acetylcholine, inflammation, parasite–host interaction, parasite immune regulation The southern cattle tick, Rhipicephalus (Boophilus) microplus (Canestrini), is the most economically important ectoparasite affecting cattle in the world (Bellgard et al. 2012, Guerrero et al. 2012). Rhipicephalus annulatus (Say) and R. microplus were eradicated from the United States through the Cattle Fever Tick Eradication Program in a protracted effort that began in 1906 and continues with ongoing inspection and treatment of imported cattle as well as quarantine and eradication of outbreak infestations within the United States (Graham and Hourrigan 1977). Rhipicephalus microplus and R. annulatus remain endemic in Mexico and other countries, and reintroduction of the ticks by importation or incursion constitutes a continuing threat to U.S. cattle producers (Temeyer et al. 2004b, Giles et al. 2014). Cattle dipping in coumaphos (an organophosphorus acaricide) is the preferred method for cattle treatment at importation inspection stations and for treatment of cattle before movement within or from quarantined premises (Davey et al. 2003). Organophosphate (OP) pesticides function by inhibition of acetylcholinesterase (AChE), an enzyme essential to the function of central nervous systems for both invertebrate and vertebrate organisms. OP resistance in insects is often conferred by point mutations in a gene encoding AChE, resulting in production of an altered AChE enzyme that is insensitive to inhibition (Lee and Bantham 1966, Fournier and Mutero 1994). Initial discovery of genes encoding AChE in ticks and searches for mutations conferring OP resistance failed to identify mutations responsible for production of AChE insensitive to inhibition by OPs. Subsequent studies revealed that ticks possess at least three genes encoding AChEs that differ substantially in amino acid sequence and biochemical properties, with BmAChE1, BmAChE2, and BmAChE3 exhibiting calculated Km values of approximately 5–10, 35–40, and 90–100 mM, respectively (Temeyer et al. 2004a, 2010). Quantitative reverse transcription polymerase chain reaction and gene silencing studies indicated that all three tick AChEs were expressed in the tick synganglion and that they were capable of functionally complementing one another (Temeyer et al. 2011, 2012a, 2013a). Further, all three tick AChEs were present at amplified copy number in genomic DNA and multiple transcripts were simultaneously expressed for each of the AChEs, providing an explanation for why searches for mutations conferring resistance had initially been unsuccessful (Temeyer et al. Published by Oxford University Press on behalf of Entomological Society of America 2016. This work is written by US Government employees and is in the public domain in the US. 1 Downloaded from http://jme.oxfordjournals.org/ by guest on August 10, 2016 The southern cattle tick, Rhipicephalus (Boophilus) microplus (Canestrini), is the most economically important cattle ectoparasite in the world. Rhipicephalus microplus and Rhipicephalus annulatus (Say) continue to threaten U.S. cattle producers despite eradication and an importation barrier based on inspection, dipping of imported cattle in organophosphate (OP) acaricide, and quarantine of infested premises. OP acaricides inhibit acetylcholinesterase (AChE), essential to tick central nervous system function. Unlike vertebrates, ticks possess at least three genes encoding AChEs, differing in amino acid sequence and biochemical properties. Genomic analyses of R. microplus and the related tick, Ixodes scapularis, suggest that ticks contain many genes encoding different AChEs. This work is the first report of a salivary cholinesterase (ChE) activity in R. microplus, and discusses complexity of the cholinergic system in ticks and significance of tick salivary ChE at the tick–host interface. It further provides three hypotheses that the salivary ChE plausibly functions 1) to reduce presence of potentially toxic acetylcholine present in the large bloodmeal imbibed during rapid engorgement, 2) to modulate the immune response (innate and/or acquired) of the host to tick antigens, and 3) to influence transmission and establishment of pathogens within the host animal. Ticks are vectors for a greater number and variety of pathogens than any other parasite, and are second only to mosquitoes (owing to malaria) as vectors of serious human disease. Saliva-assisted transmission (SAT) of pathogens is well-known; however, the salivary components participating in the SAT process remain to be elucidated. 2 Materials and Methods Tick Strains and Tissues The R. microplus susceptible strain Deutch was maintained at the Cattle Fever Tick Research Laboratory (Edinburg, TX) as described previously (Temeyer et al. 2007). Tick nymphs were collected using forceps from a patch enclosing the ticks on an infested animal approximately 2 weeks following infestation. Nymphs that molted into unfed adults were separated by sex. Unfed adult females were dissected to remove salivary glands and synganglia or microinjected with acetylthiocholine for toxicity studies and for collection of saliva. Excised salivary glands were placed in isotonic phosphatebuffered saline (PBS), pH 7.5, and stored on ice before salivary extract preparation. Salivary extract was prepared by grinding 20 pairs of tick salivary glands in 250 ml final volume of PBS and collection of supernatant after centrifugation (3 min, 20,800 g) to remove particulate material. Microinjection of Unfed Adult Ticks and Collection of Saliva Glass needles were pulled from 25-ml glass micropipettes using a Narishige PC-10 micropipette puller (Narishige Group USA, East Meadow, NY), according to the manufacturer’s instructions. Needles were broken from the glass capillary, inspected under a dissecting microscope, and epoxied onto blunt needles of gas-tight 10-ml Hamilton syringes (model 1702SN 26/0.5/PT3, Hamilton Company, Reno, NV), taking care to avoid any air pockets at the joint between the glass and metal needle. Unfed adult female ticks were placed ventral side up onto double-sided sticky pads mounted on a micromanipulator, and injected with 0.005–0.500 ml acetylthiocholine (various dilutions in isotonic PBS, pH 7.5) by positive displacement (no air in system) using a calibrated timer-activated screw-driven solenoid (Model M, ISCO Inc., Lincoln NE), as shown in Fig. 1. Saliva was collected from microinjected ticks by placement of a glass capillary over the hypostome. Acetylthiocholine Toxicity Toxicity of acetylthiocholine to unfed adult female R. microplus (average weight 2.5 mg) was investigated by microinjection (with minimal tissue damage) of dilutions of acetylthiocholine (81 mM stock solution) at the lateral axilla between the first and second or between the second and third legs. Injections of 30 or 300 nI of 100fold dilution series of acetylthiocholine stock solutions (810 nM to 81 mM) were performed to give final concentrations (based on 2.5 mg wt of uninjected ticks) of from 1 nM to 10 mM. Injected ticks were placed in packets and incubated at 28 C and 92% humidity, as described for the larval packet assay (Miller et al. 2002), and packets were monitored at 1, 2, 3, 4, and 8 h. Mortality was recorded after 24 h. Control injections with water alone resulted in no mortality. AChE Microplate Assay AChE activity and biochemical characterization in tick saliva or extracts of salivary glands or synganglia were determined in microplate assays using triplicate samples as described previously (Temeyer et al. 2010), except that data for calculation of Km and Vmax were analyzed and plotted by nonlinear regression using GraphPad Prism ver. 5.0 (GraphPad Prism, Inc., La Jolla, CA). Comparison of salivary gland extract with recombinant BmAChE1 utilized 5 ll per well of either salivary gland extract or 500-fold dilution (in PBS) of BmAChE1 baculoviral supernatant (Temeyer et al. 2010). Substrate preference for acetylthiocholine versus butyrylthiocholine in tick salivary gland extracts was tested at a final substrate concentration of 100 lM. Results Acetylthiocholine delivered to unfed female ticks by microinjection resulted in rapid tick paralysis at final equivalent concentrations of 1–10 mM, while lesser concentrations resulted in slowed movement and rapid onset of copious salivation. After 3 h, approximately 50% of ticks exposed at calculated internal concentrations of 1 mM acetylthiocholine exhibited normal movement and 50% moved very slowly with progression to 20% mortality at 4 h, 30% mortality by 8 h, and 60% mortality at 24 h. Acetylthiocholine at final equivalent concentrations of 100 mM or less resulted in minimal (5%) mortality at 24 h post-injection, while 100% mortality occurred at 10 mM. At 24 h post-injection, dead ticks appeared desiccated and were frequently “cemented” to the packet by their mouthparts in similar fashion as ticks killed by exposure to coumaphos at the IC50 concentration (data not shown). AChE assay of tick saliva, or extracts prepared from excised synganglia or salivary glands all exhibited cholinesterase activity using acetylthiocholine as substrate. The available sample of tick saliva was very limited, but yielded an apparent Km for acetylthiocholine of 10-12 mM. AChE activity was verified in salivary gland extracts by substrate preference for acetylthiocholine (AcSCh) over butyrylthiocholine, exhibiting 44-fold preference for AcSCh. Total AChE activity was approximately 2.4-fold higher in synganglial extract compared with extract from an equivalent number of paired salivary glands. AChE activity in tick salivary gland extract was compared with that of recombinant BmAChE1 expressed in baculoviral supernatant. As shown in Fig. 2, the relative response to increasing substrate concentrations was very similar for recombinant BmAChE1 and salivary gland extract. Calculated Km values for acetylthiocholine were 8.755 mM and 13.62 mM for recombinant BmAChE1 and salivary gland extract, respectively; however, the 95% confidence Downloaded from http://jme.oxfordjournals.org/ by guest on August 10, 2016 2011). Genotyping surveys identified multiple mutations associated with resistance for each of the three tick AChEs, and baculoviral expression and biochemical characterization of recombinant AChEs have to date confirmed OP-resistance mutations in at least two of the three tick AChEs (Temeyer et al. 2007, 2009, 2012b, 2013b). The genome of the related hard tick, Ixodes scapularis, is available, and appears to contain many genes that putatively encode AChEs (Temeyer et al. 2013a). In addition, the R. microplus genome also appears to contain many genes that putatively encode AChEs (Bellgard et al. 2012). The present work reports a salivary cholinesterase (ChE) activity in R. microplus, and discusses the complexity of the cholinergic system in ticks and the functional significance of tick salivary ChE at the tick–host interface. It is the first report of tick salivary ChE and provides three hypotheses that tick salivary ChE may plausibly function 1) to reduce presence of potentially toxic acetylcholine present in the extremely large bloodmeal imbibed during rapid engorgement, 2) to potentially modulate the immune response (innate and/or acquired) of the host to tick antigens and subsequent exposures, and 3) to influence tick transmission and establishment of pathogens to the host. The last hypothesis is significant because ticks are vectors for a greater number and variety of pathogens than any other parasite, and are second only to mosquitoes (owing to malaria) as vectors of serious human disease. Journal of Medical Entomology, 2016, Vol. 0, No. 0 Journal of Medical Entomology, 2016, Vol. 0, No. 0 3 Fig. 2. Comparison of R. microplus acetylcholinesterase activity in salivary gland extract with recombinant BmAChE1. The plot shows increasing substrate (acetylthiocholine) concentration on the X-axis versus initial velocity (DOD/min) on the Y-axis. Solid lines are best fit curves. intervals were 7.1–17.1 and 12–20.1, indicating that the Km values were not significantly different from one another. The previously reported Km values for BmAChE2 and BmAChE3 are quite different from that of BmAChE1 (Temeyer et al. 2011). These results suggest that although of unknown identity, the ChE activity present in tick saliva exhibits kinetic properties similar to BmAChE1. Discussion Acaricidal activity of organophosphate is attributed to inhibition of AChE and subsequent accumulation of the neurotransmitter acetylcholine causing overstimulation and failure of the tick nervous system resulting in death. This paradigm would predict that parenteral administration of acetylcholine in sufficient concentration to overwhelm the available AChE should exhibit toxic effects on ticks. Microinjection of acetylthiocholine appeared to produce an equivalent toxicological profile as that observed to result from organophosphate intoxication (i.e., dose-dependent response, with dead ticks exhibiting apparent desiccation and attachment to packets resulting from excessive salivation). The reported Km values for bovine erythrocyte AChE (140 mM acetylthiocholine, Mendelson et al. 1998; 220 mM acetylthiocholine, Montenegro et al. 2009) are 1020-fold higher than that of tick ChE present in saliva or salivary extract of R. microplus (10–14 mM acetylthiocholine). During rapid engorgement, ticks ingest several hundred times their unengorged body weight in host blood in a 3-5-d period, with most of the blood intake occurring in the final day of rapid engorgement, suggesting that one function of tick salivary AChE may be to detoxify the host bloodmeal by hydrolyzing potentially toxic levels of acetylcholine (Fujii et al. 1995) imbibed during rapid engorgement. Interestingly, bedbugs have also been reported to contain AChE as a significant component of their saliva (Francischetti et al. 2010, Seong et al. 2011). In addition to a plausible role of tick salivary ChE for detoxification of the bloodmeal, the prolonged attachment of ticks to the host may suggest another potentially significant role for tick salivary ChE. Tissue damage and introduction of “foreign” material into the host during and subsequent to tick attachment would be expected to activate an innate immune and inflammatory response by the host (Francischetti et al. 2009). Phospholipids and other materials released from damaged tissues would be converted to proinflammatory eicosanoids, arachidonic acid, and prostaglandins. Dendritic cells and other immune sentinel cells would initiate an inflammatory response, including release of cytokines and other immunostimulatory molecules to increase blood flow (vasodilation) and recruit various cellular components of the immune system to the wound site and to guide appropriate generation of subsequent innate and acquired components of the immune response (Saeed et al. 2005). Tick saliva contains a myriad of immunomodulatory components (Mathias et al. 2011, Kot al et al. 2015) that work together to modify innate and adaptive host immune response to allow Downloaded from http://jme.oxfordjournals.org/ by guest on August 10, 2016 Fig. 1. Photographic depiction of microinjection setup for R. microplus. Upper left, complete setup with microinjector module, Hamilton syringe, dissecting microscope, ticks on micromanipulator. Upper right, ticks on micromanipulator. Lower left, size of unfed adult ticks. Lower right, microscopic view of microinjection. 4 In addition, chronic inflammation is a key component of many serious diseases, including Alzheimer’s disease, amyotrophic lateral sclerosis, multiple sclerosis, Parkinson’s disease, myasthenia gravis, arthritis, asthma, as well as cardiovascular disease (Shytle et al. 2004, Nizri and Brenner 2013). Parasitic cholinergic capitalization on complexities of vertebrate neural-immune integration may provide a “Rosetta Stone” for further deciphering regulatory pathways and mechanisms controlling vertebrate immune response and regulation of inflammation. In summary, this is the first report of tick salivary ChE and provides three hypotheses that the salivary ChE plausibly functions 1) to reduce presence of potentially toxic acetylcholine present in the extremely large bloodmeal imbibed during rapid engorgement, 2) to potentially modulate the immune response (innate and/or acquired) of the host to tick antigens and subsequent exposures, and 3) to influence tick transmission and establishment of pathogens to the host. The last hypothesis is significant because ticks are vectors for a greater number and variety of pathogens than any other parasite, and are second only to mosquitoes (owing to malaria) as vectors of serious human disease. Elucidation of the effects of tick cholinesterase in altering the responses of specific immune cell populations to various activating factors is suggested as a promising area for further study. We would welcome immunological collaboration to further investigate the hypotheses presented in this study. Acknowledgments We thank Kristie Schlechte, Dave Krska, and Jason Tidwell for technical support and help with tick dissection. USDA is an equal opportunity provider and employer. This work was funded by USDA appropriated funds (CRIS # 6205-32000-031-00D and 3094-32000-036-00). A.P. Tuckow was supported by a USDA, ARS, Postdoctoral Research Program award to K.B. Temeyer. References Cited Bellgard, M. I., P. M. Moolhuijzen, F. D. Guerrero, D. Schibeci, M. Rodriguez-Valle, D. G. Peterson, S. E. Dowd, R. Barrero, A. Hunter, R. J. Miller, et al. 2012. CattleTickBase: An integrated internet-based bioinformatics resource for Rhipicephalus (Boophilus) microplus. Int. J. Parasitol. 42: 161–169. Davey, R. B., J. E. George, and R. J. Miller. 2003. Efficacy of various concentrations of coumaphos to control adult, nymphal, and larval stages of an organophosphate-resistant strain of Boophilus microplus on infested cattle. Am. J. Vet. Res. 64: 684–689. Fournier, D., and A. Mutero. 1994. Modification of acetylcholinesterase as a mechanism of resistance to insecticides. Comp. Biochem. Physiol. 108C: 19–31. Francischetti, I. M., A. Sa-Nunes, B. J. Mans, I. M. Santos, and J. M. Ribeiro. 2009. The role of saliva in tick feeding. Front. Biosci. 14: 2051–2088. Francischetti, I. M., E. Calvo, J. F. Andersen, V. M. Pham, A. J. Favreau, K. D. Barbian, A. Romero, J. G. Valenzuela, and J. M. Ribeiro. 2010. Insight into the sialome of the bed bug, Cimex lectularius. J. Proteome Res. 9: 3820–3831. Fujii, T., S. Yamada, N. Yamaguchi, K. Fujimoto, T. Suzuki, and K. Kawashima. 1995. Species differences in the concentration of acetylcholine, a neurotransmitter, in whole blood and plasma. Neurosci. Lett. 201: 207–210. Fujii, T., T. Tsuchiya, S. Yamada, K. Fujimoto, T. Suzuki, T. Kasahara, and K. Kawashima. 1996. Localization and synthesis of acetylcholine in human leukemic T cell lines. J. Neurosci. Res. 44: 66–72. Fujii, T., Y. Watanabe, T. Inoue, and K. Kawashima. 2003. Upregulation of mRNA encoding the M5 muscarinic acetylcholine receptor in human T- and B-lymphocytes during immunological responses. Neurochem. Res. 28: 423–429. Downloaded from http://jme.oxfordjournals.org/ by guest on August 10, 2016 prolonged tick feeding through inhibition of blood clotting and maintenance of blood availability (maintain vasodilation), and inhibition of wound closure and healing. The anti-inflammatory nature of systemic release of acetylcholine resulting from vagal nerve stimulation has long been known; however, the extent and nature of cholinergic involvement in immune regulation has only recently become apparent (Tracey 2007, Nizri and Brenner 2013). Many cellular components of the immune system are cholinergically competent, including presence of choline acetyltransferase and various nicotinic and muscarinic acetylcholine receptors enabling synthesis, release, and response to acetylcholine (Fujii et al. 1996, 2003; Nizri et al. 2009). Activated dendritic cells, T-cells, B-cells, and macrophages have been shown to synthesize and release acetylcholine under complex regulation (Reardon et al. 2013). Lymphocytes may be a likely source of measurable levels of acetylcholine in circulating blood (Rosas-Ballina et al. 2011, Olofsson et al. 2012). Although the cholinergic control of immune cells is not completely understood, in general, activation of nicotinic acetylcholine receptors produces an anti-inflammatory response by reducing production of pro-inflammatory cytokines, interferons, and TNF (tumor necrosis factor) without inhibiting production of IL-10 (interleukin10), while activation of muscarinic acetylcholine receptors generally results in production of a pro-inflammatory response (Nizri et al. 2006, 2008). The injection of tick salivary cholinesterase at the tick attachment site would be expected to substantially reduce local concentrations of acetylcholine, thereby altering the relative activity of nicotinic and muscarinic acetylcholine receptors, hypothetically affecting production and release of various cytokines, interferons, interleukins, TNF, etc., from activated immune cells. There is substantial evidence supporting the integration of cellular cholinergic signaling systems with other cellular pathways controlling immune system function (Razani-Boroujerdi et al. 2007, Rosas-Ballina et al. 2009, Nizri and Brenner 2013, Munyaka et al. 2014). Cholinergic competence of many immune component cell populations suggests that these cells have the capacity to maintain homeostatic local concentration of acetylcholine, thereby providing a limitation on response to changes in acetylcholine receptor activation and preventing runaway immune responses to temporal immune stimulation. Localized presence of tick salivary ChE possessing a significantly lower Km than mammalian AChE would therefore be expected to prevent return to homeostatic balance as long as the tick ChE remained present, suggesting an experimental protocol for future experiments, although choice and separation of immune cell subsets may be critical to identify regulatory changes in production of cytokines, interferons, TNFs, or other immunoregulatory products. It is therefore reasonable to conclude that tick salivary cholinesterase likely works together with other immunomodulatory components of tick saliva to modify the resulting immune response of the host. In particular, the reduced local concentration of acetylcholine might be expected to support the pro-inflammatory vasodilation response, helping to maintain availability of host blood to the feeding tick. Parasite saliva has also been shown to be an important factor in transmission and establishment of pathogens, a process referred to as saliva-assisted transmission (SAT; Hanneier et al. 2003, Nuttall and Labuda 2004, Titus et al. 2006, Kazimı́rov a and Štibr aniov a 2013, Liu and Bonnet 2014), for which the responsible salivary components have not yet been identified. Therefore, a possible additional consequence of the proposed immunomodulation by tick salivary ChE may be the enhancement of pathogen transmission and establishment within the host. Journal of Medical Entomology, 2016, Vol. 0, No. 0 Journal of Medical Entomology, 2016, Vol. 0, No. 0 Lymphocyte-derived ACh regulates local innate but not adaptive immunity. Proc. Natl. Acad. Sci. U.S.A. 110: 1410–1415. Rosas-Ballina, M., R. S. Goldstein, M. Gallowitsch-Puerta, L. Yang, S. I. Valdés-Ferrer, N. B. Patel, S. Chavan, Y. Al-Abed, H. Yang, and K. J. Tracey. 2009. The selective alpha7 agonist GTS-21 attenuates cytokine production in human whole blood and human monocytes activated by ligands for TLR2, TLR3, TLR4, TLR9, and RAGE. Mol. Med. 15: 195–202. Rosas-Ballina, M., P. S. Olofsson, M. Ochani, S. I. Vades-Ferrer, Y. A. Levine, C. Reardon, M. W. Tusche, B. A. Pavlov, U. Andersson, S. Chavan, et al. 2011. Acetylcholine-synthesizing T cells relay neural signals in a vagus nerve circuit. Science 334: 98–101. Saeed, R. W., S. Varma, T. Peng-Nemeroff, B. Sherry, D. Balakhaneh, J. Huston, K. J. Tracey, Y. Al-Abed, and C. N. Metz. 2005. Cholinergic stimulation blocks endothelial cell activation and leukocyte recruitment during inflammation. J. Exp. Med. 201: 1113–1123. Seong, K. M., Y. H. Kim, D. H. Kwon, and S. H. Lee. 2011. Identification and characterization of three cholinesterases of the common bed bug, Cimex lectularius. Insect Mol. Biol. 21: 149–159. Shytle, R. D., T. Mori, K. Townsend, M. Vendrame, N. Sun, J. Zeng, J. Ehrhart, A. A. Silver, P. R. Sanberg, and J. Tan. 2004. Cholinergic modulation of microglial activation by a7 nicotinic receptors. J. Neurochem. 89: 337–341. Temeyer, K. B., R. B. Davey, and A. C. Chen. 2004a. Identification of a third Boophilus microplus (Acari: Ixodidae) cDNA presumptively encoding an acetylcholinesterase. J. Med. Entomol. 41: 259–268. Temeyer, K. B., J. M. Pound, J. A. Miller, A. C. Chen, J. H. Pruett, F. D. Guerrero, R. B. Davey, P. M. Untalan, K. H. Lohmeyer, A. Y. Li, et al. 2004b. Organophosphate resistance in Mexican strains of Boophilus microplus: a major threat to the U.S. cattle industry. SAAS Bull. Biochem. Biotech. 17: 43–51. Temeyer, K. B., J. H. Pruett, P. U. Olafson, and A. C. Chen. 2007. R86Q, a mutation in BmAChE3 yielding a Rhipicephalus microplus organophosphate-insensitive acetylcholinesterase. J. Med. Entomol. 44: 1013–1018. Temeyer, K. B., P. U. Olafson, and R. J. Miller. 2009. Genotyping mutations in BmAChE3: A survey of organophosphate-resistant and -susceptible strains of Rhipicephalus (Boophilus) microplus. J. Med. Entomol. 46: 1355–1360. Temeyer, K. B., J. H. Pruett, and P. U. Olafson. 2010. Baculovirus expression, biochemical characterization and organophosphate sensitivity of rBmAChE1, rBmAChE2, and rBmAChE3 of Rhipicephalus (Boophilus) microplus. Vet. Parasitol. 172: 114–121. Temeyer, K. B., M. Tijerina, R. B. Davey, and P. U. Olafson. 2011. Baculovirus expression, biochemical characterization and organophosphate sensitivity of rBmAChE1, rBmAChE2, and rBmAChE3 of Rhipicephalus (Boophilus) microplus. Zoosymposia 6: 260–266. Temeyer, K. B., A. C. Chen, R. B. Davey, F. Guerrero, J. M. Howell, D. Kammlah, A. Y. Li, K. H. Lohmeyer, P. U. Olafson, A. A. Pérez de Le on, et al. 2012a. Novel approaches for control of Rhipicephalus (Boophilus) microplus. Rev. Mex. Cienc. Pecu. 3: 25–40. Temeyer, K. B., P. U. Olafson, and J. H. Pruett. 2012b. Sequence polymorphism in acetylcholinesterase transcripts and genotyping survey of BmAChE1 in laboratory and Mexican strains of Rhipicephalus (Boophilus) microplus. J. Med. Entomol. 49: 555–562. Temeyer, K. B., P. U. Olafson, D. K. Brake, A. P. Tuckow, A. Y. Li, and A. A. Pérez de Le on. 2013a. Acetylcholinesterase of Rhipicephalus (Boophilus) microplus and Phlebotomus papatasi: Gene identification, expression, and biochemical properties of recombinant proteins. Pest. Biochem. Phys. 106: 118–123. Temeyer, K. B., A. P. Tuckow, D. K. Brake, A. Y. Li, and A. A. Pérez de Le on. 2013b. Acetylcholinesterases of blood-feeding flies and ticks. Chem. Biol. Interact. 203: 319–322. Titus, R. G., J. V. Bishop, and J. S. Mejia. 2006. The immunomodulatory factors of arthropod saliva and the potential for these factors to serve as vaccine targets to prevent pathogen transmission. Parasit. Immunol. 28: 131–141. Tracey, K. J. 2007. Physiology and immunology of the cholinergic antiinflammatory pathway. J. Clin. Invest. 117: 289–296. Downloaded from http://jme.oxfordjournals.org/ by guest on August 10, 2016 Giles, J. R., A. T. Peterson, J. D. Busch, P. U. Olafson, G. A. Scoles, R. B. Davey, J. M. Pound, D. M. Kammlah, K. H. Lohmeyer, and D. M. Wagner. 2014. Invasive potential of cattle fever ticks in the southern United States. Parasit. Vectors 7: 189. Graham, O. H., and J. L. Hourrigan. 1977. Eradication programs for the arthropod parasites of livestock. J. Med. Entomol. 13: 629–658. Guerrero, F. D., R. J. Miller, and A. A. Pérez de Le on. 2012. Cattle tick vaccines: Many candidate antigens, but will a commercially viable product emerge? Int. J. Parasitol. 42: 421–427. Hanneier, S., J. Liversidge, J. M. Sternberg, and A. S. Bowman. 2003. Ixodes ricinus tick salivary gland extract inhibits IL-10 secretion and CD69 expression by mitogen-stimulated murine splenocytes and induces hyporesponsiveness in B lymphocytes. Parasit. Immunol. 25: 27–37. Kazimı́rova, M., and I. Štibr aniov a. 2013. Tick salivary compounds: their role in modulation of host defences and pathogen transmission. Front. Cell infect. Microbiol. 3: 43. Kotal, J., H. Langhansov a, J. Lieskovsk a, J. F. Andersen, I.M.B. Francischetti, T. Chavakis, J. Kopecký, J.H.F. Pedra, M. Kotsyfakis, and J. Chmelař. 2015. Modulation of host immunity by tick saliva. J. Proteomics 128: 58–68. Lee, R. M., and P. Bantham. 1966. The activity and organophosphate inhibition of cholinesterase from susceptible and resistant ticks (Acari). Entomol. Exp. Appl. 9: 13–24. Liu, X. Y., and S. I. Bonnet. 2014. Hard tick factors implicated in pathogen transmission. PLoS Negl. Trop. Dis. 8: e2566. Mathias, M.I.C., K.C.S. Furquim, and P. H. Nunes. 2011. Immunomodulatory effects of tick saliva. Invertebr. Survival J. 8: 231–240. Mendelson, I., C. Kronman, N. Ariel, A. Shafferman, and B. Velan. 1998. Bovine acetylcholinesterase: Cloning, expression and characterization. Biochem. J. 334: 251–259. Miller, R. J., R. B. Davey, and J. E. George. 2002. Modification of the food and agriculture organization larval packet test to measure amitraz-susceptibility against Ixodidae. J. Med. Entomol. 39: 645–651. Montenegro, M. F., M. T. Moral-Naranjo, E. Muñoz-Delgado, F. J. Campoy, and C. J. Vidal. 2009. Hydrolysis of acetylthiocoline, o-nitroacetanilide and o-nitrotrifluoroacetanilide by fetal bovine serum acetylcholinesterase. FEBS J. 276: 2074–2083. Munyaka, P., M. F. Rabbi, V. A. Pavlov, K. J. Tracey, E. Khafipou, and J.-E. Ghia. 2014. Central muscarinic cholinergic activation alters interaction between splenic dendritic cell and CD4þCD25- T cells in experimental colitis. PLoS ONE 9: e109272. Nizri, E., and T. Brenner. 2013. Modulation of inflammatory pathways by the immune cholinergic system. Amino Acids 45: 73–85. Nizri, E., Y. Hamra-Amitay, C. Sicsic, I. Lavon, and T. Brenner. 2006. Antiinflammatory properties of cholinergic up-regulation: a new role for acetylcholinesterase inhibitors. Neurophysiology 50: 540–547. Nizri, E., M. Irony-Tur-Sinai, N. Faranesh, I. Lavon, E. Lavi, M. Weinstock, and T. Brenner. 2008. Suppression of neuroinflammation and immunoregulation by the acetylcholinesterase inhibitor rivastigmine. J. Neuroimmunol. 203: 12–22. Nizri, E., M. Irony-Tur-Sinai, O. Lory, A. Orr-Urtreger, E. Lavi, and T. Brenner. 2009. Activation of the cholinergic anti-inflammatory system by nicotine attenuates neuroinflammation via suppression of Th1 and Th17 responses. J. Immunol. 183: 6681–6688. Nuttall, P. A., and M. Labuda. 2004. Tick-host interactions: saliva-activated transmission. Parasitology 129: S177–S189. Olofsson, P. S., M. Rosas-Ballina, Y. A. Levin, and K. J. Tracey. 2012. Rethinking inflammation: neural circuits in the regulation of immunity. Immunol. Rev. 248: 188–204. Razani-Boroujerdi, S., R. T. Boyd, M. I. D avila-Garcı́a, J. S. Nandi, N. C. Mishra, S. P. Singh, J. C. Pena-Philippides, R. Langley, and M. L. Sopori. 2007. T cells express a7-nicotinic acetylcholine receptor subunits that require a functional TCR and leukocyte-specific protein tyrosine kinase for nicotine-induced Ca2þ response. J. Immunol. 179: 2889–2898. Reardon, C., G. S. Duncan, A. Brüstle, D. Brenner, M. W. Tusche, P. S. Olofsson, M. Rosas-Ballina, K. J. Tracey, and T. W. Mak. 2013. 5