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Article

Detection of Babesia odocoilei in Ixodes scapularis Ticks Collected from Songbirds in Ontario and Quebec, Canada

by
John D. Scott
*,
Emily L. Pascoe
,
Muhammad S. Sajid
and
Janet E. Foley
Department of Medicine and Epidemiology, School of Veterinary Medicine, University of California Davis, Davis, CA 95616, USA
*
Author to whom correspondence should be addressed.
Pathogens 2020, 9(10), 781; https://doi.org/10.3390/pathogens9100781
Submission received: 19 August 2020 / Revised: 15 September 2020 / Accepted: 16 September 2020 / Published: 24 September 2020
(This article belongs to the Section Human Pathogens)
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Abstract

:
Songbirds widely disperse ticks that carry a diversity of pathogens, some of which are pathogenic to humans. Among ticks commonly removed from songbirds, the blacklegged tick, Ixodes scapularis, can harbor any combination of nine zoonotic pathogens, including Babesia species. From May through September 2019, a total 157 ticks were collected from 93 songbirds of 29 species in the Canadian provinces of Ontario and Québec. PCR testing for the 18S gene of Babesia species detected Babesia odocoilei in 12.63% of I. scapularis nymphs parasitizing songbirds in Ontario and Québec; none of the relatively small numbers of Ixodes muris, Ixodes brunneus, or Haemaphysalis leporispalustris were PCR-positive. For ticks at each site, the prevalence of B. odocoilei was 16.67% in Ontario and 8.89% and 5.26% in Québec. Of 31 live, engorged I. scapularis larvae and nymphs held to molt, 25 ticks completed the molt; five of these molted ticks were positive for B. odocoilei. PCR-positive ticks were collected from six bird species—namely, Common Yellowthroat, Swainson’s Thrush, Veery, House Wren, Baltimore Oriole, and American Robin. Phylogenetic analysis documented the close relationship of B. odocoilei to Babesia canis canis and Babesia divergens, the latter a known pathogen to humans. For the first time in Canada, we confirm the transstadial passage of B. odocoilei in I. scapularis molting from larvae to nymphs. A novel host record reveals I. scapularis on a Palm Warbler. Our findings show that B. odocoilei is present in all mobile life stages of I. scapularis, and it is widely dispersed by songbirds in Ontario and Québec.

1. Introduction

Ticks carry a wide spectrum of disease-causing microorganisms that cycle between vectors and hosts, including humans. Some of these ectoparasites are laden with tick-borne zoonotic pathogens, including Babesia spp. (Apicomplexa: Piroplasmida: Babesiidae). These malaria-like piroplasms, which invade red blood cells, were first discovered by the Romanian researcher Victor Babes in 1888 [1,2,3]. The first description of human babesiosis was a fatal case in a splenectomized farmer in Croatia [4]. Although ticks were identified as vectors shortly after the discovery of the pathogen [5], more recently, this apicomplexan microorganism has also been found to be transmitted to humans by blood transfusion [6,7], by organ transplantation [8], and by maternal–fetal transmission [9,10]. Babesia species are typically host-specific and, globally, they infect a wide range of vertebrate hosts. These Babesia spp. often result in reduced fitness and mortality in wildlife and domestic animals, producing economic losses with low productivity and added mortality. Epidemiologically, they also cause morbidity and mortality in humans worldwide [2,3,4,11,12,13,14,15,16]. Human babesiosis is reported in Canada and the United States, sometimes with fatal outcomes [11,17]. Babesia species that bring about pathogenicity in humans include B. microti, B. crassa, B. duncani, B. venatorum, B. divergens, Babesia divergens-like MO-1, Babesia sp. KO-1, Babesia sp. XXB/HangZhou, and Babesia spp. CA1, CA3, and CA4 [11,17,18,19].
Migratory songbirds (Passeriformes) disperse ticks and tick-borne pathogens across regional and transcontinental areas. These migrants occasionally support the establishment of ticks and pathogens in new foci [20,21]. Some songbirds, such as the American Robin, are reservoirs of the Lyme disease bacterium, Borrelia burgdorferi sensu lato [22]; however, passerine species are not known to be reservoir-competent hosts of Babesia spp. Even if birds are refractory to infection with a tick-borne pathogen, they can host ticks that are already infected with disease-producing microbes. For example, the blacklegged tick, Ixodes scapularis (Acari: Ixodidae), an important human-biting tick in eastern and central North America, can harbor any combination of nine different zoonotic pathogens, including Babesia species [23]. A nymphal I. scapularis, which parasitized a spring-migrating Veery in southeastern New York state, was triple co-infected with B. burgdorferi sensu lato, Babesia microti, and Anaplasma phagocytophilum [24].
Certain cervids (i.e., caribou, deer, elk) are reservoirs of Babesia odocoilei, while I. scapularis ticks are vectors of this babesial infection. In many parts of eastern and central North America, I. scapularis ticks and cervine hosts co-habitat in nature to maintain B. odocoilei. Passerine birds are common incidental hosts of I. scapularis larvae and nymphs, and occasionally, these ticks are infected with B. odocoilei. Based on current knowledge, cervids and I. scapularis form a collective hub for the enzootic transmission cycle of B. odocoilei. Although B. odocoilei has been investigated as a pathogen of cervids, it has not been examined closely as a potential source of human babesiosis.
The aim of this study was to detect and identify, to species, any Babesia DNA in ticks collected from migratory songbirds in two provinces in Canada.

2. Materials and Methods

2.1. Collection of Ticks from Songbirds

Bird banders and wildlife rehabilitators collected ixodid ticks from songbirds captured at five locations (Figure 1) between 23 April and 30 September 2019. They removed ticks using fine-pointed hardened stainless steel, #5, superfine-tipped forceps (BioQuip Products, Rancho Dominguez, CA, USA). There were three collection sites in Ontario (Ruthven Park, Long Point, and Toronto) and two in Québec (Ste-Anne-de-Bellevue and Montée Biggar). These technicians and collectors placed live ticks into transparent 8.5 mL, 15.7 mm × 75 mm, round-bottomed polypropylene tubes (Sarstedt, Montréal, Québec, Canada); each tube contained ticks from a single host. In order to prevent ticks from escaping and provide ventilation, a 3 cm piece of tulle netting was placed over the mouth of the tube, and a push cap, which had a 7 mm hole, was inserted into the tube opening. All ticks were promptly mailed in a double-zipper plastic bag with a moistened paper towel to the laboratory (JDS) for identification. Partially and fully engorged larval and nymphal ticks were held to molt to the next developmental life stage at a long-day photoperiod of 16:8 (L:D) h at room temperature in humidity from 90% to 95%. For the statistical analyses, molted ticks were designated the life stage at the time of collection. Taxonomic keys and descriptions were utilized for identification [25,26,27,28,29].

2.2. DNA Extraction and PCR

Unfed ticks were subjected to an ammonium hydroxide DNA extraction protocol as described previously [30], whereas DNA from fed ticks was extracted using the Qiagen DNeasy Blood and Tissue Kit (Qiagen, Valencia, CA, USA) following the manufacturer’s protocol for animal tissue. Ticks were initially pooled according to bird host; however, upon discovering the relatively high prevalence, we decided to process ticks individually. DNA was stored at −20 °C until PCR was performed. Conventional PCR was used to detect the 18S ribosomal RNA (rRNA) gene of the genus Babesia, with 25 µL reaction mixes containing 2.5 µL each of 5 µM primers BJ1 (5′-GTC-TTG-TAA-TTG-GAA-TGA-TGG-3′) and BN2 (5′-TAG-TTT-ATG-GTT-AGG-ACT-ACG-3′) [31], 5 µL nuclease-free water, 12.5 µL Green Go Taq (Promega, Madison, WI, USA), and 2.5 µL of DNA at 8–10 ng/µL. PCR was performed under thermal cycling conditions of initial denaturation at 94 °C for 10 min, 35 cycles of 94 °C for 1 min, 55 °C for 1 min, and 72 °C for 2 min with a final extension at 72 °C for 5 min, and then held at 4 °C. Amplified DNA was visualized with UV transillumination of a 1% agarose gel containing GelStar nucleic acid stain (Lonza, Rockland, ME, USA). Amplicons of 400–500 base pairs (bp) were excised from the gel and prepared for DNA sequencing using a gel extraction kit (QIAamp DNA Kit, Qiagen, Valencia, CA, USA).

2.3. DNA Sequencing and Phylogenetic Analysis

DNA sequencing was performed at UC Davis DNA Sequencing (College of Biological Sciences at University of California Davis, CA, USA) using the Big Dye Terminator cycle sequencing kit (Applied Biosystems, Foster City, CA, USA) and PCR primers. Sequences were compared to those published in GenBank using the BLAST database search program (https://blast.ncbi.nlm.nih.gov/Blast.cgi#_blank). In addition, sequences were manually corrected for ambiguous base calls and to remove end-reading errors. All sequences were trimmed to the same length, and the MUSCLE algorithm performed the sequence alignments [32]. DNA sequences from many Babesia species comprised B. odocoilei, B. bovis, B. conradae, B. divergens, B. duncani, B. canis canis, B. gibsoni, B. microti, and B. vulpes from GenBank for inclusion in the phylogenetic tree. Phylogeny was resolved using the maximum likelihood method in MEGA 10.0.5 [33] using the Hasegawa-Kishino-Yano with gamma distribution as determined by jModeltest 2.1.10 [34]. Bootstrapping was performed based on 1000 pseudoreplicate datasets generated from the original sequence alignments.

3. Results

3.1. Tick Collection

Overall, 157 ixodid ticks were collected from 93 songbirds of 29 bird species in 2019 at five sites in Ontario (ON) and Québec (QC) (Table 1). Species of ticks included Haemaphysalis leporispalustris (rabbit tick) (n = 6), Ixodes brunneus (bird tick) (n = 4), Ixodes muris (mouse tick) (n = 21), and I. scapularis (n = 126). The majority of ticks were nymphs (n = 134), followed by larvae (n = 19), and only four adults. Of 31 engorged ticks that were held to molt, nine successfully molted from larvae to nymphs (six I. muris and three I. scapularis), eight I. scapularis molted from nymph to adult female, seven I. scapularis molted from nymph to adult male, and one female I. muris laid a clutch of eggs, which hatched to larvae. Two I. scapularis larvae were collected from a Swainson’s Thrush on 31 May 2019 at Long Point, ON. These larvae molted to nymphs and tested positive for B. odocoilei; they constitute the first transstadial passage of B. odocoilei-positive larvae molting to nymphs in Canada.
The highest tick burden occurred at Montée Biggar, QC, with an average of 2.44 ticks per individual bird, followed by Ruthven Park, ON (1.84), Sainte-Anne-de-Bellevue, QC (1.36), Long Point, ON (1.33), and Toronto, ON (1.0). Ixodes scapularis was the only tick species found at all sampled locations, and all four tick species were present at Ruthven Park and Sainte-Anne-de-Bellevue.
The mean tick burden across all bird species was 1.69 ticks per individual with American Robins having the greatest tick burden with an average of 4.0 ticks (Table 1). Veeries, House Wrens, Winter Wrens, Hermit Thrushes, and Swainson’s Thrushes each had an average burden of 2.0–2.7 ticks per individual. Tick burdens in all other tick species were lower. Of note, I. scapularis was collected from a Palm Warbler at Long Point, Ontario on 14 May 2019, and it denotes the first report of this host record. Ixodes muris were recorded on 12 bird species, and I. brunneus and H. leporispalustris were found on three bird species each.

3.2. Babesia Detection

At least 12 ticks, all of which were I. scapularis, tested positive for Babesia, including a pool of four ticks collected from a Common Yellowthroat, a pool of five from a Common Yellowthroat, and a pool of seven from an American Robin. In general, the prevalence of Babesia in ticks was at least 8.89% (12/135), and it was highest at Ruthven Park (16.67%), followed by 8.89% at Sainte-Anne-de-Bellevue, and 5.26% at Montée Biggar (Table 2). There were no positive samples from the other two locations. The highest prevalence of Babesia in bird-feeding ticks was Swainson’s Thrush (30.00%, 3/10 tested pools), Baltimore Oriole (25.0%), American Robin (16.67%, 1/6 tested pools), Common Yellowthroat (15.63%, 5/32 tested pools), and House Wren (14.29%). DNA sequencing confirmed all positive samples as B. odocoilei; sequences were 99.18–100% similar, and all samples were confirmed as B. odocoilei. With the exception of four nymphs pooled from a Common Yellowthroat (99.59%) and a single nymph from a Common Yellowthroat both from Ruthven Park, amplicons were 100% similar to three published B. odocoilei. The closest related species was B. canis canis (93.33–93.82% similarity to reference samples), which differed from B. odocoilei by 18 base pairs. Upon further analysis, we noticed a 92.88% similarity between sequences of B. divergens and B. odocoilei in the phylogenic tree (Figure 2).
The prevalence for both larvae and nymphs combined revealed that 12 (11.54%) of 104 I. scapularis ticks were positive for B. odocoilei. PCR-positive nymphs were collected between 5 May and 20 August, and the larvae were collected on 31 May. These larval and nymphal ticks included two larvae that were held to molt, and were tested as nymphs. The GenBank accession numbers for B. odocoilei, and their bird-tick-pathogen associations are listed in Table 3.
The sequences from tick DNA samples were all identical, except for CN19-33B and pool CN19-47B, which differed each by a single nucleotide from the other sequences. Therefore, these two sequences were on separate branches within the same clade of B. odocoilei sequences.

4. Discussion

As vectors, I. scapularis ticks play an integral role in the enzootic transmission cycle of B. odocoilei. Of medical significance, these arthropod vectors, which are commonly infected with pathogenic microbes, bite humans. Since I. scapularis larvae and nymphs parasitize birds, they are transported continental distances during spring and fall migration. Geographically, avian hosts can transport B. odocoilei-infected I. scapularis larvae and nymphs hundreds of kilometers during the migratory flight. This study highlights the major role that songbirds play in the dispersal of bird-feeding ticks and their associated pathogens, especially B. odocoilei. We show that the prevalence of B. odocoilei transported by wild birds is significant.
At the northern extent of migratory avian flyways that cover most of the western hemisphere [35], Canada experiences ticks and tick-transmitted pathogens from birds each spring from as far south as equatorial South America [36,37,38,39,40]. While Canadians contend with numerous tick-borne diseases, recent bird–tick–pathogen evidence reveals I. scapularis nymphs as far north and as far west as northern Alberta [41], and some of these ticks were infected with B. burgdorferi sensu lato [41]. As well, in Atlantic Canada, researchers have reported songbird-transported I. scapularis nymphs infected with B. burgdorferi sensu lato as far north as the province of Newfoundland and Labrador [41]. Here, we show that at least 29 migrating and locally active bird species carry multiple tick species across a wide area of southern Canada [42], and at least 12.63% of the nymphal I. scapularis infesting these avian hosts bring with them the apicomplexan pathogen B. odocoilei.
Four species of ticks were removed from songbirds, including I. muris and H. leporispalustris, which commonly infest small mammals and birds. The bird tick, I. brunneus, is exclusively on birds [28], whereas H. leporispalustris, I. muris, and I. scapularis parasitize both avian and mammalian hosts. The latter two tick species bite humans, and I. scapularis is the predominant vector of pathogens associated with borreliosis, anaplasmosis, and babesiosis [23]. Biologically, I. scapularis has at least 150 vertebrate hosts (i.e., avian, mammalian, reptilian), and of these hosts, I. scapularis parasitize at least 82 different bird species [26,42,43]. The most commonly infested birds in our study were American Robins, Veeries, House Wrens, Winter Wrens, Hermit Thrushes, and Swainson’s Thrushes, all with an average of 2–4 ticks per individual bird. These ground-foraging species scratch and pick through the leaf litter, which facilitates bird parasitism by ectoparasites, especially host-seeking ticks. During fall migration, all ticks from short- and long-distance songbirds originated in Canada. Notably, we report a new host record of I. scapularis parasitizing a Palm Warbler.
With the exception of Blue Jays, all of the passerines captured are migratory and support the transportation of I. scapularis northward during spring migration. The bird species that carried ticks with the highest prevalence of B. odocoilei (Figure 3) were Common Yellowthroat, Swainson’s Thrush, Veery, House Wren, Baltimore Oriole, and American Robin. Our findings revealed that up to 25% of orioles were parasitized.
Babesia odocoilei is a recently described malaria-like microorganism that was originally reported as apathogenic in cervine hosts [44]. Now, it is known to cause death associated with high levels of parasitemia in cervids (Artiodactylia: Cervidae). This cervid family includes white-tailed deer (Odocoileus virginianus), American elk (Cervus elaphus canadensis), and caribou (Rangifer terandus caribou) [45,46]. Mortality has been noted in captive and wild cervids in various parts of North America.
Based on phylogenetic analysis of the 18S rRNA gene, B. divergens is the closest known genetic relative to B. odocoilei; the former is a human pathogen [11,19]. Even though the B. odocoilei amplicons in this study formed a close-knitted clade, they were widely distributed geographically. For instance, the direct flight path between Site 1 and Site 5 is 607 km. Since serological assays are not able to discriminate between certain babesial strains and species [31,47], DNA sequence analysis of PCR amplicons is needed to confirm the identity of any given Babesia species.
To date, I. scapularis is the only vector known to harbor and transmit B. odocoilei. This particular piroplasm has been detected in I. scapularis ticks in multiple states of the U.S.A., including Indiana [48,49], Maine [49], Wisconsin [49], Michigan [50], New York [51], and Pennsylvania [49,52]. Prior to the present study, B. odocoilei-positive I. scapularis have been reported parasitizing songbirds in southwestern Ontario [53,54]. In northeastern North America, a B. odocoilei-positive I. scapularis tick was reported feeding on a human [55]. Stateside, a B. divergens-like agent was linked to a case of human babesiosis in Missouri [20].
We provide the first documentation of transstadial passage of B. odocoilei in I. scapularis from larvae to nymphs in Canada. Overall, we observed 25 unique events of molt metamorphosis, of which five were positive for Babesia, including larvae to nymphs and nymphs to adults. From one particular dual infestation on a Swainson’s Thrush, two B. odocoilei-positive I. scapularis larvae successfully molted to nymphs. These larvae may have acquired this piroplasm either by transovarial transmission or directly from the bird itself. Based on a literature search, the former is the most likely. Other Babesia researchers have shown that transovarial transmission occurs between I. scapularis females and their eggs [45]. Transovarial transmission is well-established for some Babesia species, such as B. bovis and B. divergens, but it is not documented for small-sized Babesia spp., such as B. microti [23,56,57].
While the majority of songbird-transported ticks infected with B. odocoilei were found during spring migration, PCR-positive ticks were also found during the summer nesting and fledging period and, likewise, during the autumn migration. Depending on bird species, autumn migration typically starts August 1st. When I. scapularis ticks become infected with B. odocoilei anytime during the four life stages (eggs, larvae, nymphs, adults), they can retain the infection throughout the life cycle. During the stage-to-stage molt, B. odocoilei is retained in the midgut, which stays intact, and it maintains its viability. Physiologically, B. odocoilei successfully moves through all four life stages (i.e., female to eggs, eggs to larvae, larvae to nymphs, and nymphs to adults) [11,45].
There is a paucity of information on whether any bird species may be infected with or serve as a reservoir of B. odocoilei. Songbirds may hold B. odocoilei for a short period of time in their bodies; nevertheless, without a bird–tick–pathogen study, which includes drawing blood from songbirds, we will not know the answer. In the case of week-old chickens, Lyme disease spirochetes only remain infectious for one week [22]. In order to conduct a xenodiagnostic study using an avian host and ticks, a special permit for animal research would be required. In addition, a veterinarian would be needed during the spring and fall banding period to conduct venipuncture sampling. Nonetheless, bird banders are apprehensive about putting extra stress on captured birds, especially during peak migration.
The competence of songbirds as reservoirs of B. odocoilei has remained unresolved. Since none of the H. leporispalustris, I. brunneus, and I. muris was positive for B. odocoilei, these bird parasitisms add further evidence to the incompetence of songbirds as reservoirs. Although certain passerine birds may hold B. odocoilei in their systems, even for a short time, further enzootic bird-tick-pathogen research is required to determine the competence of selected songbirds as a reservoir for B. odocoilei.
The occurrence of B. odocoilei in I. scapularis nymphs collected from passerines was approximately 12.63%. Our findings are consistent with other tick researchers in the northern U.S. states who collected questing I. scapularis adults [49]. Since the midgut stays intact during the molt, fully engorged nymphs have equivalent infection prevalence to questing adults. Thus, when engorged I. scapularis nymphs molt, the infection prevalence remains the same in unfed adults. Once a motile life stage (i.e., larva, nymph, female) becomes infected with B. odocoilei, the infection is held throughout each life stage to the next.
Each of the five sites studied meet the criteria (six or more ticks of a motile life stage) for an established population of blacklegged ticks [58]. Whenever songbirds are nesting within an established population of I. scapularis, they have ample opportunity to become parasitized by ticks infected with pathogens, such as B. odocoilei [53]. Songbirds are incidental hosts of larval and nymphal I. scapularis, while white-tailed deer are resident hosts that are reservoirs of B. odocoilei. Coupled together, cervids, songbirds, and I. scapularis ticks enhance the enzootic transmission cycle of B. odocoilei. Transstadial passage and transovarial transmission of B. odocoilei in blacklegged ticks perpetuate this apicomplexan piroplasm in Canada.

5. Conclusions

Songbirds play a role in the wide dispersal of B. odocoilei-infected blacklegged ticks. Based on our findings, we found that bird-transported I. scapularis nymphal ticks in Ontario and Québec have a prevalence of B. odocoilei infection approximating 12.63%. The prevalence of B. odocoilei may be as high as 16.67% in Ontario and Québec. Using molting of ticks, we provide substantial evidence that B. odocoilei perpetuates babesial infection through the complete life cycle of I. scapularis. Our research provides the first documentation of transstadial passage of Babesia odocoilei in I. scapularis from larvae to nymphs in Canada, and this study implicates transovarial transmission in the ecology of B. odocoilei. Notably, white-tailed deer and I. scapularis ticks are the key components that maintain a perpetual enzootic transmission cycle of B. odocoilei. Since babesial piroplasms can cause death in people, especially if they are splenectomized, immunocompromised, or have a tick-borne, zoonotic co-infection [4,59,60,61], further work is needed to determine if B. odocoilei is pathogenic to humans.

Author Contributions

J.D.S. was responsible for study design, tick identification and tick molting, writing of manuscript, and coordination of tick data. E.L.P. facilitated the analysis of dataset, writing, and completing phylogenetic analysis. M.S.S. tested ticks and compiled data spreadsheets for pathogens. J.E.F. provided laboratory management and manuscript preparation. All authors have read and agree to the published version of the manuscript.

Funding

Funding for this study was provided in part by the Mary Alice Holmes Memorial Foundation and, likewise, by a philanthropic donor Diane Kindree. J.E.F. and E.L.P. acknowledge funding from the Pacific Southwest Regional Center of Excellence for Vector-Borne Diseases, funded by the U.S. Centers for Disease Control and Prevention (Cooperative Agreement 1U01CK000516).

Acknowledgments

We thank bird banders and wildlife rehabilitators for collecting ticks from songbirds. We are grateful to Simon Duval for sharing banding information. We are indebted to Amanda Green for computer graphics.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Babes, V. Sur l’hémoglobinurie bactérienne du boef. CR Acad. Sci. 1888, 107, 692–694. [Google Scholar]
  2. Schnittger, L.; Rodriguez, A.E.; Florin-Christensen, M.; Morrison, D.A. Babesia: A world emerging. Infect. Genet. Evol. 2012, 12, 1788–1809. [Google Scholar] [CrossRef] [PubMed]
  3. Uilenberg, G. Babesia—A historical overview. Veter Parasitol. 2006, 138, 3–10. [Google Scholar] [CrossRef]
  4. Škrabalo, Z.; Deanović, Z. Piroplasmosis in man: Report on a case. Doc. Med. Geogr. Trop. 1957, 9, 11–16. [Google Scholar] [PubMed]
  5. Smith, T.; Kilbourne, F.L. Investigation into the Nature, Causation, and Prevention of Southern Cattle Fever, 1st ed.; United States Government Printing Office: Washington, DC, USA, 1893; pp. 85–116.
  6. Bloch, E.M.; Herwaldt, B.L.; Leiby, D.A.; Shaieb, A.; Herron, R.M.; Chervenak, M.; Reed, W.; Hunter, R.; Ryals, R.; Hagar, W.; et al. The third described case of transfusion-transmitted Babesia duncani. Transfusion 2011, 52, 1517–1522. [Google Scholar] [CrossRef] [PubMed]
  7. Villatoro, T.; Karp, J.K. Transfusion-transmitted babesiosis. Arch. Pathol. Lab. Med. 2019, 143, 130–134. [Google Scholar] [CrossRef] [Green Version]
  8. Brennan, M.B.; Herwaldt, B.L.; Kazmierczak, J.J.; Weiss, J.W.; Klein, C.L.; Leith, C.P.; He, R.; Oberley, M.J.; Tonnetti, L.; Wilkins, P.P.; et al. Transmission of Babesia microti parasites by solid organ transplantation. Emerg. Infect. Dis. 2016, 22, 1869–1876. [Google Scholar] [CrossRef] [Green Version]
  9. Fox, L.M.; Winger, S.; Ahmed, A.; Arnold, A.; Chou, J.; Rhein, L.; Levy, O. Neonatal babesiosis: Case report and review of the literature. Pediatr. Infect. Dis. J. 2006, 25, 169–173. [Google Scholar] [CrossRef]
  10. Cornett, J.K.; Malhotra, A.; Hart, D. Vertical transmission of babesiosis from a pregnant, splenectomized mother to her neonate. Infect. Dis. Clin. Pract. 2012, 20, 408–410. [Google Scholar] [CrossRef]
  11. Kjemtrup, A.M.; Conrad, P.A. Human babesiosis: An emerging tick-borne disease. Int. J. Parasitol. 2000, 30, 1323–1337. [Google Scholar] [CrossRef]
  12. Ramos, C.M.; Cooper, S.M.; Holman, P.J. Molecular and serologic evidence for Babesia bovis-like parasites in white-tailed deer (Odocoileus virginianus) in south Texas. Vet. Parasitol. 2010, 172, 214–220. [Google Scholar] [CrossRef] [PubMed]
  13. Australian Society for Parasitology. Babesia . Available online: http://parasite.org.au/parasite/text/babesia-text.html#top (accessed on 27 July 2020).
  14. Holman, P.J.; A Waldrup, K.; Wagner, G.G. In vitro cultivation of a Babesia isolated from a white-tailed deer (Odocoileus virginianus). J. Parasitol. 1988, 74, 111–115. [Google Scholar] [CrossRef] [PubMed]
  15. Goff, W.L.; Jessup, D.A.; Waldrup, K.A.; Thomford, J.W.; Conrad, P.A.; Boyce, W.M.; Gorham, J.R.; Wagner, G.G. The isolation and partial characterization of a Babesia sp. from desert bighorn sheep (Ovis canadensis nelsoni). J. Eukaryot. Microbiol. 1993, 40, 237–243. [Google Scholar] [CrossRef]
  16. Thomford, J.W.; Conrad, P.A.; Boyce, W.M.; Holman, P.J.; Jessup, D.A. Isolation and in vitro cultivation of Babesia parasites from free-ranging desert bighorn sheep (Ovis canadensis nelsoni) and mule deer (Odocoileus hemionus) in California. J. Parasitol. 1993, 79, 77–84. [Google Scholar] [CrossRef] [PubMed]
  17. Scott, J.D. First record of locally acquired human babesiosis in Canada caused by Babesia duncani: A case report. Sage Open Med. Case Rep. 2017, 5. [Google Scholar] [CrossRef] [Green Version]
  18. Herwaldt, B.L.; Persing, D.H.; Precigout, E.A.; Goff, W.L.; Mathiesen, D.A.; Taylor, P.W.; Eberhard, M.L.; Gorenflot, A.F. A Fatal case of babesiosis in Missouri: Identification of another piroplasm that infects humans. Ann. Intern. Med. 1996, 124, 643. [Google Scholar] [CrossRef]
  19. Ord, R.L.; Lobo, C.A. Human babesiosis: Pathogens, prevalence, diagnosis, and treatment. Curr. Clin. Microbiol. Rep. 2015, 2, 173–181. [Google Scholar] [CrossRef]
  20. Hamer, S.A.; Goldberg, T.L.; Kitron, U.D.; Brawn, J.D.; Anderson, T.K.; Loss, S.R.; Walker, E.D.; Hamer, G.L. Wild birds and urban ecology of ticks and tick-borne pathogens, Chicago, Illinois, USA, 2005–2010. Emerg. Infect. Dis. 2012, 18, 1589–1595. [Google Scholar] [CrossRef]
  21. Scott, J.D. The establishment of a blacklegged tick population by migratory songbirds in Ontario, Canada. J. Vet. Sci. Med. 2012, 1, 5. [Google Scholar] [CrossRef]
  22. Richter, D.; Spielman, A.; Komar, N.; Matuschka, F.-R. Competence of American Robins as reservoir hosts for Lyme disease spirochetes. Emerg. Infect. Dis. 2000, 6, 133–138. [Google Scholar] [CrossRef] [Green Version]
  23. Nicholson, W.A.; Sonenshine, D.E.; Noden, B.H. Ticks (Ixodida). In Medical and Veterinary Entomology, 3rd ed.; Mullen, G.R., Durden, L.A., Eds.; Academic Press/Elsevier: London, UK, 2019; pp. 603–672. [Google Scholar]
  24. Hersh, M.H.; Osfeld, R.S.; McHenry, D.J.; Tibbetts, M.; Brunner, J.L.; Killilea, M.E.; LoGiudice, K.; Schmidt, K.A.; Keesing, F. Co-infestation of blacklegged ticks with Babesia microti and Borrelia burgdorferi is higher than expected and acquired from small mammal hosts. PLoS ONE 2014, 9, e99348. [Google Scholar] [CrossRef] [PubMed]
  25. Clifford, C.M.; Anastos, G.; Elbl, A. The Larval Ixodid Ticks of the Eastern United States; Entomological Society of America Lanham: Maryland, MD, USA, 1961. [Google Scholar]
  26. Keirans, J.E.; Hutcheson, H.J.; Durden, L.A.; Klompen, J.S.H. Ixodes (Ixodes) scapularis (Acari: Ixodidae): Redescription of all active stages, distribution, hosts, geographical variation, and medical and veterinary importance. J. Med. Entomol. 1996, 33, 297–318. [Google Scholar] [CrossRef] [PubMed]
  27. Cooley, R.A. The Genera Boophilus, Rhipicephalus, and Haemaphysalis (Ixodidae) of the New World (National Institute of Health Bulletin No. 187); U.S. Government: Washington, DC, USA, 1946; p. 54.
  28. Durden, L.A.; Keirans, J.E. Nymphs of the Genus Ixodes (Acari: Ixodidae) of the United States: Taxonomy, Identification Key, Distribution, Hosts, and Medical/Veterinary Importance; Thomas Say Publications in Entomology, Entomological Society of America: Lanham, MD, USA, 1996; p. 95. [Google Scholar]
  29. Keirans, J.E.; Clifford, C.M. The genus Ixodes in the United States: A scanning electron microscope study and key to the adults. J. Med. Entomol. 1978, 15, 1–38. [Google Scholar] [CrossRef]
  30. Humair, P.; Douet, V.; Morena, C.F.; Schouls, L.M.; Van de Pol, I.; Gern, L. Molecular identification of bloodmeal source in Ixodes ricinus ticks using 12 rDNA as a genetic marker. J. Med. Entomol. 2007, 44, 869–880. [Google Scholar] [CrossRef] [PubMed]
  31. Casati, S.; Sager, H.; Gern, L.; Piffaretti, J.-C. Presence of potentially pathogenic Babesia sp. for human in Ixodes ricinus in Switzerland. Ann. Agric. Environ. Med. 2016, 13, 65–70. [Google Scholar]
  32. Edgar, R.C. MUSCLE: Multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004, 32, 1792–1797. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Kumar, S.; Stecher, G.; Li, M.; Knyaz, C.; Tamura, K. MEGA X: Molecular evolutionary genetics analysis across computing platforms. Mol. Biol. Evol. 2018, 35, 1547–1549. [Google Scholar] [CrossRef]
  34. Darriba, D.; Taboada, G.L.; Doallo, R.; Posada, D. jModelTest 2: More models, new heuristics and parallel computing. Nat. Methods 2012, 9, 772. [Google Scholar] [CrossRef] [Green Version]
  35. US Fish and Wildlife Service. Flyways. Available online: https://www.fws.gov/birds/management/flyways.php (accessed on 30 July 2020).
  36. Scott, J.D.; Durden, L.A. Amblyomma dissimile Koch (Acari: Ixodidae) parasitizes bird captured in Canada. Syst. Appl. Acarol. 2015, 20, 854–860. [Google Scholar]
  37. Morshed, M.G.; Scott, J.D.; Fernando, K.; Beati, L.; Mazerolle, D.F.; Geddes, G.; Durden, L.A. Migratory songbirds disperse ticks across Canada, and first isolation of the Lyme disease spirochete, Borrelia burgdorferi, from the avian tick, Ixodes auritulus. J. Parasitol. 2005, 91, 780–790. [Google Scholar] [CrossRef]
  38. Scott, J.D.; Lee, M.-K.; Fernando, K.; Durden, L.A.; Jorgensen, D.R.; Mak, S.; Morshed, M.G. Detection of Lyme disease spirochete, Borrelia burgdorferi sensu lato, including three novel genotypes in ticks (Acari: Ixodidae) collected from songbirds (Passeriformes) across Canada. J. Vector Ecol. 2010, 35, 124–139. [Google Scholar] [CrossRef] [PubMed]
  39. Scott, J.D.; Anderson, J.F.; Durden, L.A. Widespread dispersal of Borrelia burgdorferi-infected ticks collected from songbirds across Canada. J. Parasitol. 2012, 98, 49–59. [Google Scholar] [CrossRef] [PubMed]
  40. Scott, J.D.; Durden, L.A. New records of the Lyme disease bacterium in ticks collected from songbirds in central and eastern Canada. Int. J. Acarol. 2015, 41, 241–249. [Google Scholar] [CrossRef]
  41. Scott, J.D.; Clark, K.L.; Foley, J.E.; Bierman, B.C.; Durden, L.A. Far-reaching dispersal of Borrelia burgdorferi sensu lato-infected blacklegged ticks by migratory songbirds in Canada. Healthcare 2018, 6, 89. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  42. Scott, J.D.; Clark, K.L.; Foley, J.E.; Anderson, J.F.; Bierman, B.C.; Durden, L.A. Extensive distribution of the Lyme disease bacterium, Borrelia burgdorferi sensu lato, in multiple tick species parasitizing avian and mammalian hosts across Canada. Healthcare 2018, 6, 131. [Google Scholar] [CrossRef] [Green Version]
  43. Scott, J.D.; Clark, K.L.; Coble, N.M.; Ballantyne, T.R. Detection and transstadial passage of Babesia species and Borrelia burgdorferi sensu lato in ticks collected from avian and mammalian hosts in Canada. Healthcare 2019, 7, 155. [Google Scholar] [CrossRef] [Green Version]
  44. Perry, B.D.; Nichols, D.K.; Cullom, E.S. Babesia odocoilei Emerson and Wright, 1970 in white-tailed deer, Odocoileus virginianus (Zimmermann), in Virginia. J. Wildl. Dis. 1985, 21, 149–152. [Google Scholar] [CrossRef] [Green Version]
  45. Holman, P.J.; Madeley, J.; Craig, T.M.; Allsopp, B.A.; Allsopp, M.T.; Petrini, K.R.; Waghela, S.D.; Wagner, G.G. Antigenic, phenotypic and molecular characterization confirms Babesia odocoilei isolated from three cervids. J. Wildl. Dis. 2000, 36, 518–530. [Google Scholar] [CrossRef]
  46. Pattullo, K.M.; Wobeser, G.; Lockerbie, B.P.; Burgess, H.J. Babesia odocoilei infection in a Sakatchewan elk (Cervus elaphus canadensis) herd. J. Vet. Diagn. Investig. 2013, 25, 535–540. [Google Scholar] [CrossRef]
  47. Herwaldt, B.L.; Cacciò, S.; Gherlinzoni, F.; Aspöck, H.; Siemenda, S.B.; Piccaluga, P.; Martinelli, G.; Edelhofer, R.; Hollenstein, U.; Poletti, G.; et al. Molecular characterization of a non-Babesia divergens organism causing zoonotic babesiosis in Europe. Emerg. Infect. Dis. 2003, 9, 942–948. [Google Scholar] [CrossRef]
  48. Steiner, F.E.; Pinger, R.R.; Vann, C.N.; Abley, M.J.; Sullivan, B.; Grindle, N.; Clay, K.; Fuqua, C. Detection of Anaplasma phagocytophilum and Babesia odocoilei DNA in Ixodes scapularis (Acari: Ixodidae) collected in Indiana. J. Med. Entomol. 2006, 43, 437–442. [Google Scholar] [CrossRef]
  49. Steiner, F.E.; Pinger, R.R.; Vann, C.N.; Grindle, N.; Civetello, D.; Clay, K.; Fuqua, C. Infection and co-infection rates of Anaplasma phagocytophilum variant, Babesia spp., Borrelia burgdorferi, and richettsial endosymbiont in Ixodes scapularis (Acari: Ixodidae) from sites in Indiana, Maine, Pennsylvania, and Wisconsin. J. Med. Entomol. 2008, 45, 289–297. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  50. Hamer, S.A.; Roy, P.L.; Hickling, G.J.; Walker, E.D.; Foster, E.S.; Barber, C.C.; Tsao, J.I. Zoonotic pathogens in Ixodes scapularis, Michigan. Emerg. Infect. Dis. 2007, 13, 1131–1133. [Google Scholar] [CrossRef] [PubMed]
  51. Schoelkopf, L.; Hutchinson, C.E.; Bendele, K.G.; Goff, W.L.; Willette, M.; Rasmussen, J.M.; Holman, P.J. New ruminant hosts and wider geographic range identified for Babesia odocoilei (Emerson and Wright 1970). J. Wildl. Dis. 2005, 41, 683–690. [Google Scholar] [CrossRef] [Green Version]
  52. Livengood, J.; Hutchinson, M.L.; Thirumalapura, N.; Tewari, D. Detection of Babesia, Borrelia, Anaplasma, and Rickettsia spp. in adult black-legged ticks (Ixodes scapularis) from Pennsylvania, United States, with a Luminex Bead Assay. Vector Borne Zoonotic Dis. 2020, 20, 406–411. [Google Scholar] [CrossRef]
  53. Scott, J.D.; Clark, K.L.; Coble, N.M.; Ballantyne, T.R. Presence of Babesia odocoilei and Borrelia burgdorferi sensu stricto in a tick and dual parasitism of Amblyomma inornatum and Ixodes scapularis on a bird in Canada. Healthcare 2019, 7, 46. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  54. Milnes, E.L.; Thornton, G.; Léveillé, A.N.; Delinatte, P.; Barta, J.R.; Smith, D.A.; Nemeth, N. Babesia odocoilei and zoonotic pathogens identified from Ixodes scapularis ticks in southern Ontario, Canada. Ticks Tick-Borne Dis. 2019, 10, 670–676. [Google Scholar] [CrossRef] [PubMed]
  55. Shock, B.C.; Moncayo, A.; Cohen, S.; Mitchell, E.A.; Williamson, P.C.; Lopez, G.; Garrison, L.E.; Yabsley, M.J. Diversity of piroplasms detected in blood-fed and questing ticks from several states in the United States. Ticks Tick-Borne Dis. 2014, 5, 373–380. [Google Scholar] [CrossRef]
  56. Bonnet, S.; Jouglin, M.; Malandrin, L.; Becker, C.; Agoulon, A.; L’hostis, M.; Chauvin, A. Transstadial and transovarial persistence of Babesia divergens DNA in Ixodes ricinus ticks fed on infected blood in a new skin-feeding technique. Parasitology 2007, 134, 197–207. [Google Scholar] [CrossRef]
  57. Mehlhorn, H.; Shein, E. The piroplasms: Life cycle and sexual stages. Adv. Parasitol. 1984, 23, 37–103. [Google Scholar]
  58. Scott, J.D.; Pascoe, E.L.; Sajid, M.S.; Foley, J.E. Monitoring of nesting songbirds detects established population of blacklegged ticks and associated Lyme disease endemic area in Canada. Healthcare 2020, 8, 59. [Google Scholar] [CrossRef] [Green Version]
  59. Homer, M.J.; Aquilar-Delfin, I.; Telford, S.R., III; Krause, P.J.; Persing, D.H. Babesiosis. Clin. Microbiol. Rev. 2000, 13, 451–469. [Google Scholar] [CrossRef] [PubMed]
  60. Anderson, J.F.; Mintz, E.D.; Gadbaw, J.J.; Magnarelli, L.A. Babesia microti, human babesiosis, and Borrelia burgdorferi in Connecticut. J. Clin. Microbiol. 1991, 29, 2779–2783. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  61. Hatcher, J.C.; Greenberg, P.D.; Antique, J.; Jimenez-Lucho, V.E. Severe babesiosis in Long Island: Review of 34 cases and their complications. Clin. Infect. Dis. 2001, 32, 1117–1125. [Google Scholar] [CrossRef] [PubMed]
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Figure 1. Map of Ontario and Québec showing tick collection sites. (1) McGill Bird Observatory, Ste-Anne-de-Bellevue, Québec; 45.43 N, 73.94 W. (2) Montée Biggar, Québec; 45.09 N, 74.22 W. (3) Fatal Light Awareness Program, Toronto, Ontario; 43.74 N, 79.37 W. (4) Ruthven Park National Historic Site Banding Station, Haldimand Bird Observatory, Cayuga, Ontario; 42.97 N, 79.87 W. (5) Long Point Bird Observatory, Long Point (Port Rowan), Ontario; 42.52 N, 80.17 W.
Figure 1. Map of Ontario and Québec showing tick collection sites. (1) McGill Bird Observatory, Ste-Anne-de-Bellevue, Québec; 45.43 N, 73.94 W. (2) Montée Biggar, Québec; 45.09 N, 74.22 W. (3) Fatal Light Awareness Program, Toronto, Ontario; 43.74 N, 79.37 W. (4) Ruthven Park National Historic Site Banding Station, Haldimand Bird Observatory, Cayuga, Ontario; 42.97 N, 79.87 W. (5) Long Point Bird Observatory, Long Point (Port Rowan), Ontario; 42.52 N, 80.17 W.
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Figure 2. Maximum likelihood phylogenetic tree of 18S rRNA sequences from Babesia-positive ticks collected from songbirds in Canada during 2019, with 11 published sequences of nine different reference Babesia species for comparison. Labels include tick ID, bird host species, and location. Alphanumeric values in brackets denote published GenBank sequences. The scale bar represents the percentage of genetic variation along tree branches. Abbreviations: AMRO, American Robin; BAOR, Baltimore Oriole; COYE, Common Yellowthroat; HOWR, House Wren; SWTH, Swainson’s Thrush; VEER, Veery; MB, Montée Biggar (QC); SAdB, Sainte-Anne-de-Bellevue (QC); RP, Ruthven Park (ON).
Figure 2. Maximum likelihood phylogenetic tree of 18S rRNA sequences from Babesia-positive ticks collected from songbirds in Canada during 2019, with 11 published sequences of nine different reference Babesia species for comparison. Labels include tick ID, bird host species, and location. Alphanumeric values in brackets denote published GenBank sequences. The scale bar represents the percentage of genetic variation along tree branches. Abbreviations: AMRO, American Robin; BAOR, Baltimore Oriole; COYE, Common Yellowthroat; HOWR, House Wren; SWTH, Swainson’s Thrush; VEER, Veery; MB, Montée Biggar (QC); SAdB, Sainte-Anne-de-Bellevue (QC); RP, Ruthven Park (ON).
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Figure 3. Common Yellowthroat, female, parasitized by blacklegged ticks, Ixodes scapularis. This ground-foraging bird species was commonly infested by bird-feeding ticks. Photo credits: Ana Morales.
Figure 3. Common Yellowthroat, female, parasitized by blacklegged ticks, Ixodes scapularis. This ground-foraging bird species was commonly infested by bird-feeding ticks. Photo credits: Ana Morales.
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Table
Table 1. Infestation of ixodid ticks collected from songbirds, and prevalence of Babesia odocoilei in songbird-transported ticks in Ontario and Québec, Canada, 2019. Hlp, Haemaphysalis leporispalustris; Ibr, Ixodes brunneus; Imu, Ixodes muris; Isc, Ixodes scapularis. L, larva(e); N, nymph(s); F, female(s). preval. stands for prevalence.
Table 1. Infestation of ixodid ticks collected from songbirds, and prevalence of Babesia odocoilei in songbird-transported ticks in Ontario and Québec, Canada, 2019. Hlp, Haemaphysalis leporispalustris; Ibr, Ixodes brunneus; Imu, Ixodes muris; Isc, Ixodes scapularis. L, larva(e); N, nymph(s); F, female(s). preval. stands for prevalence.
Bird host speciesNo. hostsNo. ticksHlpIbrImuIscNo. ticks/hostBabesia preval. (%)
LNNFLNFLN
American Redstart, Setophaga ruticilla11--------1 ‡1.00
American Robin, Turdus migratorius312--------124.016.67
Baltimore Oriole, Icterus galbula34--------4 (2 §)1.325.00
Black-and-white Warbler, Mniotilta varia11----1 *----1.00
Blue Jay, Cyanocitta cristata34---1----31.30
Blue-winged Warbler, Vermivora cyanoptera11-----1---1.00
Canada Warbler, Cardellina canadensis11-------1-1.00
Carolina Wren, Thryothorus ludovicianus11-----1---1.00
Common Grackle, Qiscalus quiscula11--------11.00
Common Yellowthroat, Geothlypis trichas244211--1 *---39 (2 ‡, 1 §)1.815.63
Gray Catbird, Dumetella carolinensis22--------21.00
Hermit Thrush, Catharus guttatus36--------6 (1 ‡)2.00
House Wren, Troglodytes aedon36----121 †-22.314.29
Mourning Warbler, Geothlypis philadelphia55-----1--41.00
Nashville Warbler, Leiothlypis ruficapilla22--------2 (1 ‡)1.00
Northern Waterthrush, Parkesia noveboracensis44-----2--21.00
Ovenbird, Seiurus aurocapilla11--------1‡1.00
Palm Warbler, Setophoga palmarum11--------11.00
Red-eyed Vireo, Vireo olivaceus11-------1 *-1.00
Rose-breasted Grosbeak, Pheucticus ludovicianus22--------21.00
Ruby-crowned Kinglet, Regulus calendula11--1-----1.00
Song Sparrow, Melospiza melodia34----1 *2--11.30
Swainson’s Thrush, Catharus ustulatus613-1--2 (1 *)1-2 *7 (1 ‡)2.230.00
Swamp Sparrow, Melospiza georgiana11-----1---1.00
Tennessee Warbler, Leiothlypis peregrina11-----1---1.00
Veery, Catharus fuscescens102712--2 *---22 (4 §)2.73.85
White-throated Sparrow, Zonotrichia albicollis44---2----2 (1 ‡)1.00
Winter Wren, Troglodytes hiemalis25-------5-2.50
Yellow Warbler, Setophaga petechia23--------31.50
Total931572413812191171.698.89
* collected as a larva, held to molt, tested as a nymph; † collected as a female, held to lay eggs, tested, eggs were held to hatch, tested as larvae; ‡ collected as a nymph, held to molt, tested as a female; § collected as a nymph, held to molt, tested as a male.
Table
Table 2. Prevalence of ixodid ticks collected from songbirds at five locations in Ontario and Québec, 2019.
Table 2. Prevalence of ixodid ticks collected from songbirds at five locations in Ontario and Québec, 2019.
LocationNo. hostsNo. ticksHaemaphysalis leporispalustrisIxodes brunneusIxodes murisIxodes scapularisNo. ticks/hostBabesia preval. (%)
LNNFLNFLN
Long Point (ON)1216214 (3 ‡)1.330
Ruthven Park (ON)2546112537 (2 ‡, 3 §)1.8416.67
Toronto (ON)222 (1 ‡)10
Montée Biggar (QC)18441340 (4 §)2.445.26
Sainte-Anne-de-Bellevue (QC)3649118 (6 *)101 †4 (3 *)24 (2 ‡)1.368.89
Total931572413812191171.698.89
L, larva(e); N, nymph(s); F, female(s). * collected as a larva, held to molt, and tested as a nymph; † collected as a female, held to lay eggs, then female tested, eggs hatch, and larvae tested; ‡ collected as a nymph, held to molt, and tested as a female; § collected as a nymph, held to molt, and tested as a male.
Table
Table 3. Bird–tick–pathogen associations for ixodid ticks testing positive for Babesia odocoilei collected from songbirds in Ontario and Québec, 2019.
Table 3. Bird–tick–pathogen associations for ixodid ticks testing positive for Babesia odocoilei collected from songbirds in Ontario and Québec, 2019.
Sample IDDate collectedLocationBird speciesLife stageGenBank ID
CN19-215 MayRuthven Park (ON)House WrenNymphMT830841
CN19-33B16 MayRuthven Park (ON)Common YellowthroatNymph to femaleMT830842
CN19-4118 MayRuthven Park (ON)Baltimore OrioleNymph to maleMT830843
CN19-5221 MaySainte-Anne-de-Bellevue (QC)Common YellowthroatNymphMT830835
CN19-48B (n = 5)22 MayRuthven Park (ON)Common YellowthroatNymphMT830846
CN19-47B (n = 4)22 MayRuthven Park (ON)Swainson’s ThrushNymphMT830845
CN19-49C23 MayRuthven Park (ON)Common YellowthroatNymph to femaleMT830844
CN19-67A31 MaySainte-Anne-de-Bellevue (QC)Swainson’s ThrushLarva to nymphMT830836
CN19-67B31 MaySainte-Anne-de-Bellevue (QC)Swainson’s ThrushLarva to nymphMT830837
CN19-71 (n = 7)07 JunMontée Biggar (QC)American RobinNymphMT830840
CN19-111A20 JulMontée Biggar (QC)Common YellowthroatNymphMT830838
CN19-12820 AugSainte-Anne-de-Bellevue (QC)VeeryNymphMT830839

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Scott, J.D.; Pascoe, E.L.; Sajid, M.S.; Foley, J.E. Detection of Babesia odocoilei in Ixodes scapularis Ticks Collected from Songbirds in Ontario and Quebec, Canada. Pathogens 2020, 9, 781. https://doi.org/10.3390/pathogens9100781

AMA Style

Scott JD, Pascoe EL, Sajid MS, Foley JE. Detection of Babesia odocoilei in Ixodes scapularis Ticks Collected from Songbirds in Ontario and Quebec, Canada. Pathogens. 2020; 9(10):781. https://doi.org/10.3390/pathogens9100781

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Scott, John D., Emily L. Pascoe, Muhammad S. Sajid, and Janet E. Foley. 2020. "Detection of Babesia odocoilei in Ixodes scapularis Ticks Collected from Songbirds in Ontario and Quebec, Canada" Pathogens 9, no. 10: 781. https://doi.org/10.3390/pathogens9100781

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