Prevalence of tick-borne pathogens in the South Okanagan, British Columbia: Active surveillance in ticks (Dermacentor andersoni) and deer mice (Peromyscus maniculatus)

Background: Tick-borne pathogens are rare in the South Okanagan re­gion of British Columbia, but there is still public concern about the diseases they can cause. 
Methods: Ticks (Dermacentor an­dersoni) and deer mice (Peromyscus maniculatus) were collected and tested to determine the prevalence of tick-borne pathogens and hantavirus.
Results: No ticks contained evidence of Borrelia burgdorferi senso strictoAnaplasma phagocytophilumBartonella henselae, or Rickettsia rickettsiiR. peacockii (nonpathogenic) was present in 32.5% of ticks tested anad R. rhipicephali (unknown pathogenicity) was present in 12.5%. Deer mice tested had no antibodies to B. burgdorferi s.s. or B. henselae; one mouse was seropositive for A. phago­cytophilum; 12.3% were positive for R. rickettsii, but this might represent cross-reactivity to R. rhipicephali; 4.1% had significant antibody titres to Sin Nombre virus, a species of hantavirus. 
Conclusions: Given the low prevalence of tick-borne pathogens, health professionals should focus on im­proving public understanding of the true risk of tick-borne zoonoses in the area studied, and raise awareness of the personal protective practices (e.g., tucking pants into socks; regular self checks after being in tick habitat) that can further reduce the already low risk of infection.

Although results from testing ticks and mice in the South Okanagan suggest the risk is low for contracting Lyme disease and other zoonoses in the area, the public should be informed of protective personal practices that reduce tick bites.

Concerns about zoonoses
Several species of ticks—arthropod ectoparasites such as Ixodes pacificus—transmit pathogens that cause the most frequently contracted zoono­ses in North America.[1] Human cases of these diseases (e.g., Lyme disease, anaplasmosis, human babesiosis) are rare in the South Okanagan region of British Columbia.[2]

Indeed, Lyme disease, caused by the pathogen Borrelia burgdorferi sensu stricto, has a human incidence rate of less than 0.1/100000 in all of BC.[3] However, there is in­creasing public concern and controversy about the risk of contracting diseases from wildlife or domestic animals, particularly Lyme disease.[4]

The low risk of contracting tick-borne zoonoses in the South Okanagan region is supported by passive surveys for tick-borne pathogens. Between 1993 and 2006 health practitioners and private citizens sent ticks collected from humans for analysis at the British Columbia Centre for Disease Control (BCCDC), resulting in the identifi­cation of 5801 I. pacificus and 1151 I. angustus samples. 

Of the ticks collected, approximately 80 were found to harbor B. burgdorferi s.s.[2] How­ever, while passive surveys can provide an idea of the distribution of tick-borne pathogens (i.e., presence or absence), they do not constitute a representative sample of ticks in a given region. 

Passive surveys are indirect methods that do not reveal the prevalence of patho­gens within tick populations—that is, the likelihood of being exposed to a pathogen after being bitten by a tick.

Active surveys needed
Active surveys can help clarify the prevalence of tick-borne pathogens by directly examining ticks and their main disease host for the presence of pathogens. In BC, tick-borne patho­gens are maintained in the environment by the interaction between ticks and the main disease host, deer mice (Peromyscus maniculatus).[5

Examining ticks allows us to estimate the current prevalence of pathogens, while examining the antibodies in the serum of deer mice can allow us to confirm the prevalence found in ticks, as well as identify past exposures to patho­gens. As well, different species of ticks transmit different pathogens (e.g., Der­macentor andersoni transmit Rick­ettsia rickettsiiI. pacificus transmit B. burgdorferi s.s. and Anaplasma phagocytophilum).[6

Thus, active surveillance not only helps determine the prevalence of the pathogens, but also the tick species present and the patho­gens they are likely to transmit.

To address public concern and clarify the risk of contracting tick-borne zoonoses, active surveillance was conducted in an area within the South Okanagan to determine the prevalence of tick-borne pathogens. 

From 2007 to 2009, ticks and deer mice serum samples were collected and analyzed for the following pathogens (ticks only) or antibodies to the pathogens (deer mice serum): B. burgdorferi s.s.R. rickettsiiA. phagocytophilum; and Bartonella henselae

As we were concerned with the human exposure to pathogens during daily wilderness activities, our focus was on hard ticks (e.g., Dermacentor spp., Ixodes spp.), which are diurnal, and not soft ticks (e.g., Ornithodoros spp.), which are nocturnal. 

Deer mice serum samples were opportunistically tested for antibodies against Sin Nombre virus (SNV), a species of hantavirus that is transmitted by deer mice; human ex­posure to SNV can lead to respiratory failure.[7,8]

Collection of ticks and deer mice
Ticks were collected once a week from 1 April to 30 April 2008 and 1 April to 30 June 2009 at 11 sites in the study area (Figure). Ticks were collected by “flagging”[9] for 1 hour (from 6 to 10 a.m.) in suitable tick habitat at each site, and all collected ticks were identified by species and life stage.[10

Deer mice were collected every 2 weeks using 36 Longworth live traps[11] placed in suitable habitat for deer mice and ticks (i.e., areas with mixed vegetational structure)[12] at 10 sites in the study area from 1 May to 30 May and 1 August to 31 August 2007 and 1 April to 30 April 2008. 

Blood samples were collected from captured deer mice and all animals were examined for attached ticks. Animal handling and manipulations were approved under the University of British Columbia animal care protocol (approval number A08-0711).

Testing for pathogens in host-seeking ticks
In total, 330 adult D. andersoni ticks collected from the different sampling sites in 2008 and 2009 were tested for infection with B. burgdorferi s.s.A. phagocytophilumB. henselae, and spotted fever rickettsial species. 

Testing of B. burgdorferi s.s. was conducted at the BCCDC on 110 ticks collected in 2008, while the remaining 220 ticks collected in 2008 and 2009 were tested at the National Microbiology Laboratory (NML) in Winnipeg. Ticks were tested individually at BCCDC, while at the NML they were tested in pools of five ticks. DNA was extracted from ticks using QIAGEN commercial extraction kits.[13]

At the BCCDC, tick samples were screened for B burgdorferi s.s. DNA as previously described.[14] Briefly, polymerase chain reaction (PCR) was used to target amplicons of borrelial DNA and amplify a portion of the variable spacer region between two conserved structures, the 3' end of the 5S rRNA (rrf) and the 5' end of the 23S rRNA. The PCR was performed using a GE illustra PuReTaq Ready-To-Go PCR Beads on Stratagene Robocycler. 

At the NML, DNA from ticks was screened for A. phagocytophilumB. henselae, and spotted fever rickettsial species using real-time PCR. The prim­ers and probes were directed toward the msp2 gene,[15] 321s and H495as segments,[16] and gltA gene, respectively.[17

All reactions were performed using Taqman Fast Universal PCR Master Mix (Applied Biosystems) with a final concentration of 0.3 mM of each pri­mer and 0.1 mM of the probe. Determination of the rickettsial species in positive ticks was perform­ed by am­plification of DNA in a semi-nested PCR.[18

All amplicons were purified using the QIAquick PCR Purification kit (QIAGEN) and sequenced by the NML Genomics Core Facility in Winnipeg. The sequences were analyzed using DNASTAR Lasergene 7 software. Homologous sequences were detected using the National Center for Biotechnology Information search engine.

Serological assays on deer mouse sera
Serological assays were performed at the NML to detect antibodies against B. burgdorferi s.s.A. phagocyto­philumR. rickettsii, and SNV in deer mouse serum samples. 

Antibodies to B. burgdorferi s.s. were detected by enzyme-linked immunosorbent assay (ELISA) and Western blot assay as previously described.[19

Serum samples were screened for antibodies to A. phagocytophilum in an immunofluorescence assay (IFA) similar to that described by Nieto and Foley in 2008.[20] Modifications in­cluded using FTA Hemagglutination Buffer as sample diluent, Evan’s Blue for conjugate dilution, and commercially prepared slides (Fuller Laboratories, CA). 

Reactive samples were confirmed by an IgG Western blot assay similar to that described by Walder and colleagues in 2006,[21] but using a conjugate specific to Peromyscus antibodies. 

Serum samples were screened for antibodies to R. rickettsii using an IFA protocol similar to that described in a National Center for Infectious Diseases-CDC publication,[22] though modified for use with rodent sera. 

Briefly, serum samples diluted 1:64 were applied to slides pre-coated with R. rickettsii and performed as per the A. phagocytophilum IFA above. Re­active samples were further titrated and samples with titres equal to or greater than 1:64 were considered positive for this study.  

Lastly, serum samples were tested for evidence of infection with SNV using the protocol as previously des­cribed,[7] but with Black Creek Canal virus used as the coating antigen in the initial screening ELISA.

Tick and small mammal collection
A total of 5557 ticks were collected. Although other species are known to be present in the area (e.g., I. angustus),[23D. andersoni was the only species collected and more than 99% of these ticks were adult males and females. 

No larvae and only 37 D. andersoni nymphs were collected, of which 17 were collected from the small mammals. A total of 276 deer mice were captured, and serum samples were collected from 219 animals.

The deer mice collected were mainly adults (more than 80%), while the rest were juveniles. Other types of rodents were collected: 22 chipmunks, Tamias townsendii; 17 Great Basin pocket mice, Perognathus parvus; and 5 Mon­tane voles, Microtus montanus. These rodents were examined for ticks and released without further processing as per animal care guidelines.

Pathogens detected in ticks 
DNA of B. burgdorferi s.sA. phagocytophilumB. henselae, and R. rickettsii was not detected in any of the ticks tested by PCR. R. peacockii was present in all the pooled tick samples except for 2, and confirmed in 13 of 40 ticks tested; R. rhipicephali was present in 8 of the pooled samples, and confirmed in 5 of 40 ticks tested; an unknown rickettsial agent was detected in 3 of 40 ticks.

Antibodies in deer mouse sera
The deer mouse sera results were as follows: 0% (0/219) positive for B. burgdorferi s.s., 0.46% (1/219) positive for A. phagocytophilum, and 12.3% (27/219) positive for R. rickettsii. The single positive for A. phago­cytophi­lum suggests that the pathogen is present, but given the absence of Ixodes spp. collected, it is at a low prevalence in the environment. 

Similarly, the positive results for R. rickettsii confirm the low prevalence found among the ticks. However, because R. rhipicephali was present in the ticks at our study sites, but not R. rickettsii, the seropositivity may be due to cross-reactions in the IFA.[24] Finally, 4.1% of the deer mice had evidence of in­fection with SNV.

Low prevalence of pathogens confirmed
The prevalence of tick-borne patho­gens was low in the study area, suggesting there is little risk that humans will be exposed to the pathogens and contract the diseases they can cause. The ticks tested showed no evidence of B. burgdorferi s.s.A. phagocyto­philumB. henselae, or R. rickettsii

R. peacockii was present in nearly all tick pools tested, but this is not surprising as it is an endosymbiont of D. andersoni; notably, it is nonpathogenic. R. rhipicephali was found in 12.5% of ticks tested, but is of unknown pathogenicity. 

The results from the ticks were confirmed with the deer mouse sera tested: 0% B. burgdorferi s.s., 0.4% A. phagocytophilum, and 12.3% possible positives for R. rickettsii. The evidence of positive R. rickettsii in the deer mouse sera is questionable, given that R. rickettsii was found at low titres (≥1:64) and this finding may be the result of a cross-reaction with R. rhipicephali or other rickettsial agents.[24

In addition, only D. andersoni ticks were collected, suggesting that patho­gens transmitted by those ticks (i.e., R. rickettsii) are more common in the region and of more concern than those transmitted by Ixodes spp. (i.e., B. burgdorferi s.s.). Finally, 3.1% of the samples were positive for hantavirus, confirming the presence of the disease as previously found in human cases in BC.[8]

The absence of B. burgdorferi s.s. in our results, in both the ticks and the deer mice, confirms the rarity of Ixo­des spp. in the region[25] and indicates that D. andersoni is not a competent vector for the pathogen, but is competent for rickettsial agents such as R. rhipicephali.[24

If B. burgdorferi s.s. was significantly present in the environment within Ixodes spp. ticks—which we did not collect (as further discussed below)—its presence would also have been indicated through the antibodies in the deer mouse sera tested. 

The prevalence of pathogens found is in accordance with reports of patient cases and passive surveys in the region.[24,26] Other BCCDC surveys of deer mice spurred by suspected human cases of Lyme disease have found that 3.66% (6/164) of deer mice caught tested positive for B. burgdorferi s.s. antibodies.[3

The presence of pathogens is due to the collection of deer mice in regions of BC that have populations of Ixodes spp. present rather than the D. andersoni collected in the South Okanagan. Indeed, recent predictive modeling of I. pacificus and I. angustus distributions based on habitat conditions in BC suggest they are mainly located along the coast of BC.[25]

Limitations of study
Clearly, this study had several limitations. First, a restricted area was examined—which is the trade-off of active surveys: though our sampling intensity allowed for an understanding of the prevalence of tick-borne pathogens in specific locations, other locations in the South Okanagan not sampled could harbor different patho­gens or even Ixodes spp. 

Also, as previously mentioned, other areas of BC have had human cases of Lyme disease and evidence of Ixodes spp., so the tick-borne pathogens in those areas are likely different. Our results can thus not be generalized to other parts of BC. 

Further, we were limited to examining only the main disease reservoir, deer mice, and did not ex­amine other species we collected (e.g., pocket mice) because they were deem­ed at-risk species or we lacked the permits to collect them. Previous work has shown that other species can be competent disease reservoirs,[27] so other tick-borne pathogens may have been overlooked. 

Importantly, our collection of only D. andersoni and no Ixodes spp. ticks was likely the result of our study design and our choice of sampling times and locations: although Ixodes spp. and nymph ticks are present in the region,[23] they are more active in cooler months and at earlier hours in the day. However, we selected our sampling times because they reflected the times and locations of human activity so that our results would be meaningful for evaluating the risk of human exposure to tick-borne patho­gens. 

The South Okanagan is an arid and hot region, where the temperatures can be in excess of 30°C. In these conditions, only the hardiest ticks will be active: Ixodes spp. are more sensitive to heat than D. andersoni;[28] similarly, being smaller, nymphs are more sensitive to heat and desiccation than adults. 

As well, Ixodes spp. and nymphs may prefer to quest for hosts on leaf litter rather than vegetation, thus making them unavailable for collection in this study.28 Although we were not able to survey all the ticks in the region for pathogens (i.e., patho­gens from Ixodes spp. and the noc­turnal soft ticks), our results suggest that, during daily activities in the wilderness, humans are most likely to encounter D. andersoni ticks and their associated pathogens.

While prevalence of tick-borne patho­gens is low and exposure to them is unlikely, the zoonoses they can cause remain a source of public concern.[4] Addressing tick-borne zoonoses in the South Okanagan may be primarily a communication challenge. 

Members of the public need to know both the true risk of contracting a disease and the personal protective practices that can effectively reduce the likelihood of contact with pathogens (e.g., tucking pants into socks; regular self-checks after being in tick habitat).[29

Risk communication is particularly important in the South Okanagan, given the region’s expanding human population and economic growth. More people are recreating and working in the human-wildlife interface and many of these are new residents who are unfamiliar with local environmental hazards, such as ticks, and do not know how to protect themselves.[30]

In summary, the prevalence of tick-borne pathogens was found to be low in the South Okanagan, and there is little risk of contracting zoonoses when exposed to a tick in the region. Health professionals should thus fo­cus on improving public understanding of tick-borne zoonoses, and on promoting personal protective practices. 

Future research should continue to actively examine other sites in the South Okanagan as well as other locations in BC that are expected to have populations of Ixodes spp.[25]

This research was made possible by funding through the PHARE training program. We thank David Roth, Thomas Sullivan, and Sarah Gergel for help, comments, and advice.

Competing interests
None declared.

This article has been peer reviewed.


1. Walker DH. Tick-transmitted infectious diseases in the United States. Annu Rev Public Health 1998;19:237-269.
2. Ogden NH, Lindsay LR, Morshed M, et al. The rising challenge of Lyme borreliosis in Canada. Can Commun Dis Rep 2008;34:1-19.
3. Henry B, Morshed M. Prevention of bites is key to summer safety in BC. BCMJ 2007;49:303.
4. CBC News. Doctors failing to treat Lyme disease: B.C. victim’s family. 2008. Accessed 15 December 2009.
5. Piesman J, Eisen L. Prevention of tick-borne diseases. Annu Rev Entomol 2008;53:323-343.
6. Randolph SE. Tick ecology: Processes and patterns behind the epidemiological risk posed by ixodid ticks as vectors. Parasitology 2004;129:S37-S39.
7. Lindsay LR, Drebot MA, Weiss E, et al. Hantavirus pulmonary syndrome in Manitoba. Can J Infect Dis 2001;12:169-173.
8. MacDougall L, Fyfe M, Bowie WR, et al. Hantavirus infection in British Columbia: An atypical case history and epidemiological review. BCMJ 2005;47:234-240.
9. Daniels TJ, Falco RC, Fish D. Estimating population size and drag sampling efficiency for the blacklegged tick (Acari: Ixodidae). J Med Entomol 2000;37:357-363.
10. Furman DP, Loomis EC. The ticks of California (Acari: Ixodida). Berkeley, CA: University of California Press; 1984.
11. Mills JN, Childs JE, Ksiazek TG, et al. Methods for trapping and sampling small mammals for virologic testing. Atlanta, GA: US Department of Human Health Services, Public Health Service; 1995.
12. Sullivan TP, Sullivan DS. Plant and small mammal diversity in orchard versus non-crop habitats. Agriculture Ecosystems & Environment 2006;116:235-243.
13. Cockwill KR, Taylor SM, Snead ECR, et al. Granulocytic anaplasmosis in three dogs from Saskatoon, Saskatchewan. Can Vet J 2009;50:835-840.
14. Morshed MG, Scott JD, Fernando K, et al. Distribution and characterization of Borrelia burgdorferi isolates from Ixodes scapularis and presence in mammalian hosts in Ontario, Canada. J of Med Entomol 2006;43:762-773.
15. Courtney JW, Kostelnik LM, Zeidner NS, et al. Multiplex real-time PCR for detection of Anaplasma phagocytophilum and Borrelia burgdorferi. J Clin Microbiol 2004;42:3164-3168.
16. Maggi RG, Breitschwerdt EB. Potential limitations of the 16S-23S rRNA intergenic region for molecular detection of Bartonella species. J Clin Microbiol 2005;43:1171-1176.
17. Stenos J, Graves SR, Unsworth NB. A highly sensitive and specific real-time PCR assay for the detection of spotted fever and typhus group rickettsiae. Am J Trop Med Hyg 2005;73:1083-1085.
18. Rozental T, Eremeeva ME, Paddock CD, et al. Fatal case of Brazilian spotted fever confirmed by immunohistochemical staining and sequencing methods on fixed tissues. Ann N Y Acad Sci 2006;1078:257-259.
19. Ogden NH, Bouchard C, Kurtenbach K, et al. Active and passive surveillance and phylogenetic analysis of Borrelia burg­dorferi elucidate the process of Lyme disease risk emergence in Canada. Environ Health Perspect 2010;118:doi:10.1289/ehp.090176.
20. Nieto NC, Foley JE. Evaluation of squirrels (Rodentia: Sciuridae) as ecologically significant hosts for Anaplasma phagocytophilum in California. J Med Entomol 2008;45:763-769.
21. Walder G, Fuchs D, Sarcletti M, et al. Human granumocytic anaplasmosis in Austria: Epidemiologica, clinical and laboratory findings in five consecutive patients from Tyrol, Austria. Int J Med Microbiol 2006;S1:297-301.
22. NCID-CDC. Indirect fluorescent antibody technique for the detection of rickettsial antibodies. Atlanta GA: National Center for Infectious Diseases-CDC; 1991. p. 12.
23. Smith IM, Lindquist EE, Behan-Pelletier V. Mites (Acari). In: Smith IM, Scudder GGE, (eds). Assessment of species diversity in the Montane Cordillera Ecozone. Burlington, ON: Ecological Monitoring and Assessment Network; 1998.
24. Dergousoff SJ, Gajadhar AJ, Chilton NB. Prevalence of Rickettsia species in Canadian populations of Dermacentor andersoni and D. variabilis. Appl Environ Microbiol 2009;75:1786-1789.
25. Mak S, Morshed M, Henry B. Ecological niche modeling of Lyme disease in British Columbia, Canada. J Med Entomol 2010;47:99-105.
26. Banerjee S. Update on the status of Lyme borreliosis in British Columbia, Canada. Clin Infect Dis 1995;21:704-704.
27. Brisson D, Dykhuizen DE, Ostfeld RS. Conspicuous impacts of inconspicuous hosts on the Lyme disease epidemic. Proc Biol Sci 2008;275:227-235.
28. Needham GR, Teel PD. Off-host physiological ecology of ixodid ticks. Ann Rev Entomol 1991;36:659-681.
29. Wilson ME. Prevention of tick-borne diseases. Med Clin North Am 2002;86:219-230.
30. Patz JA, Daszak P, Tabor GM, et al. Unhealthy landscapes: Policy recommendations on land use change and infectious disease emergence. Environ Health Perspect 2004;112:1092-1098.

Dr Teng is a postdoctoral fellow in the De­partment of Geography at the University of Victoria. Dr Lindsay is a research scientist for the Public Health Agency of Canada at the National Microbiology Laboratory in the Zoonotic Diseases and Special Pathogens section. Dr Bart­lett is an associate professor at the School of Environmental Health at the University of British Columbia. Dr Klinkenberg is an associate professor in the Department of Geography at UBC. Ms Dibernardo is a biologist for the Public Health Agency of Canada at the National Microbiology Laboratory in the Zoonotic Diseases and Special Pathogens section. Dr Wood is a biologist for the Public Health Agency of Canada at the National Microbiology Laboratory in the Zoonotic Diseases and Special Pathogens section. Dr Morshed is program head of Zoonotic and Emerging Pathogens at the British Columbia Centre for Disease Control, and a clinical professor in the Department of Pathology and Laboratory Medicine at UBC.

Jack Teng, PhD,, Robbin Lindsay, PhD,, Karen Bartlett, PhD,, Brian Klinkenberg, PhD,, Antonia Dibernardo, BSc, MLT,, Heidi Wood, PhD,, Muhammad Morshed, PhD, SCCM. Prevalence of tick-borne pathogens in the South Okanagan, British Columbia: Active surveillance in ticks (Dermacentor andersoni) and deer mice (Peromyscus maniculatus). BCMJ, Vol. 53, No. 3, April, 2011, Page(s) - Clinical Articles.

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