Domestic cats are the natural reservoir of Bartonella henselae, B. clarridgeiae and B. koehlerae. To determine the role of wild felids in the epidemiology of Bartonella infections, blood was collected from 14 free-ranging California mountain lions (Puma concolor) and 19 bobcats (Lynx rufus). Bartonella spp. were isolated from four (29%) mountain lions and seven (37%) bobcats. These isolates were characterized using growth characteristics, biochemical reactions, molecular techniques, including PCR-RFLP of selected genes or interspacer region, pulsed-field gel electrophoresis (PFGE), partial sequencing of several genes, and DNA-DNA hybridization. Two isolates were identical to B. henselae genotype II. All other isolates were distinguished from B. henselae and B. koehlerae by PCR-RFLP of the gltA gene using endonucleases HhaI, TaqI and AciI, with the latter two discriminating between the mountain lion and the bobcat isolates. These two novel isolates displayed specific PFGE profiles distinct from B. henselae, B. koehlerae and B. clarridgeiae. Sequences of amplified gene fragments from the three mountain lion and six bobcat isolates were closely related to, but distinct from, B. henselae and B. koehlerae. Finally, DNA-DNA hybridization studies demonstrated that the mountain lion and bobcat strains are most closely related to B. koehlerae. We propose naming the mountain lion isolates B. koehlerae subsp. boulouisii subsp. nov. (type strain: L-42-94), and the bobcat isolates B. koehlerae subsp. bothieri subsp. nov. (type strain: L-17-96), and to emend B. koehlerae as B. koehlerae subsp. koehlerae. The mode of transmission and the zoonotic potential of these new Bartonella subspecies remain to be determined.
Citation: Chomel BB, Molia S, Kasten RW, Borgo GM, Stuckey MJ, Maruyama S, et al. (2016) Isolation of Bartonella henselae and Two New Bartonella Subspecies, Bartonella koehlerae Subspecies boulouisii subsp. nov. and Bartonella koehlerae Subspecies bothieri subsp. nov. from Free-Ranging Californian Mountain Lions and Bobcats. PLoS ONE 11(3): e0148299. doi:10.1371/journal.pone.0148299
Editor: Dongsheng Zhou, Beijing Institute of Microbiology and Epidemiology, CHINA
Received: August 11, 2015; Accepted: January 15, 2016; Published: March 16, 2016
Copyright: © 2016 Chomel et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and have been submitted to GenBank. The GenBank/EMBL/DDBJ accession numbers for the partial sequences of the gltA, ftsZ, rpoB genes and ITS regions of the two reference strains described in this paper are as follows: Bartonella koehlerae subsp. boulouisii (L-42-94), KF246521, KF246530, KF246539, and KF437493, respectively, and for Bartonella koehlerae subsp. bothieri (L-17-96), KF246528, KF246537, KF246545, and KF437500, respectively. GenBank Accession numbers for partial sequences of the above four loci in the other isolates described in this paper are summarized in Table 1.
Funding: This project was funded in part by the George and Phyllis Miller Feline Research Fund, Center for Companion Animal Health, University of California, Davis, the Master of Preventive Veterinary Medicine Research Project Fund (University of California, Davis) and Mérial Inc., Athens, GA. Sophie Molia was a recipient of a Lavoisier grant (French Ministry of Foreign Affairs) and a Barron fellowship (University of California, Davis). Jane E. Koehler received funding support from a Burroughs Wellcome Fund Clinical Scientist Award in Translational Research, a California HIV Research Program Award, and NIH grants U54AI065359 and R01AI103299 from the NIAID. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
The genus Bartonella is comprised of aerobic Gram-negative bacteria. An increasing number of Bartonella species and subspecies are being recognized as emerging pathogens . Seventeen of the 33 Bartonella species and 3 subspecies currently described are associated with human disease ( http://www.bacterio.net/bartonella.htm). The spectrum of diseases caused by Bartonella species in humans is expanding, and includes Carrion’s disease, trench fever, cat scratch disease, bacillary angiomatosis, peliosis hepatis, endocarditis, chronic bacteremia, neuroretinitis, encephalitis, and fever of unknown origin . The most common Bartonella infection in people is caused by B. henselae, the etiological agent of cat scratch disease (CSD). Domestic cats (Felis catus) are known to be the natural reservoir of B. henselae, as well as of B. clarridgeiae and B. koehlerae [3–7]. B. bovis has also been isolated from a few domestic cats, and initially was provisionally named B. weissii by Regnery and colleagues at the Centers for Disease Control in Atlanta, Ga. (R. Regnery, N. Marano, P. Jameson, E. Marston, D. Jones, S. Handley, C. Goldsmith, and C. Greene, 15th Meet. Am. Soc. Rickettsiol., 2000, abstr. 4). Very rarely, B. quintana and B. vinsonii subsp. berkhoffii have been isolated from or detected in domestic cats [8, 9].
Many free-ranging wild felids live in North America. An estimated 5,100 mountain lions (Puma concolor), also known as pumas or cougars  and an equal or larger number of bobcats (Lynx rufus) (P. Swift, unpublished data) live in California. Overlapping habitats can lead to the spread of ectoparasites between wild and free-ranging domestic cats. This interface is epidemiologically important because the majority of Bartonella spp. are vectored by arthropods that could potentially facilitate transmission between felid species and humans.
In previous studies in California, 26 (35%) of 74 free-ranging mountain lions and 33 (53%) of 62 free-ranging bobcats were seropositive for B. henselae . A serological survey of vector-borne zoonoses in 442 mountain lions during the period 1987–2010 revealed a seroprevalence of 37.1% for B. henselae, with the highest exposure in central coastal California . DNA amplified from the blood of three of seven mountain lions, which were strongly seropositive for Bartonella, was genetically similar to B. henselae . Another study reported a seroprevalence of 16% in mountain lions and 31% in bobcats from southern California and Colorado . In Florida, antibodies against B. henselae were also detected in two (28%) mountain lions originating from Texas (Puma concolor stanleyana), and in five (18%) Florida panthers (Puma concolor coryi) . In a larger study of 479 mountain lions and 91 bobcats from North America, Central America, and South America, the overall prevalence of B. henselae antibodies was 19.4% in mountain lions and 23.1% in bobcats . In the United States, seroprevalence of B. henselae in mountain lions from the southwestern region was found to be almost three times higher than in mountain lions from the northwestern and mountain states . Because systematic culture, isolation and PCR-based speciation of Bartonella strains were not performed in previous studies, it is not known whether the Bartonella strains in wild felids, which have the potential for transmission from wild felids to domestic cats or vice-versa, are distinct from those in domestic cats. The objective of this study is to describe the Bartonella species isolated from free-ranging mountain lions and bobcats from California.
Materials and Methods
B. henselae genotype I (Houston 1) type strain ATCC 49882 and B. clarridgeiae ATCC 51734 were obtained from the American Type Culture Collection (Rockville, MD). Strain U4, originally isolated from a naturally infected cat at the University of California, Davis, was used for the Bartonella henselae genotype II (Marseille genotype) strain. B. koehlerae type strain C29 (ATCC 700693) was isolated from a naturally infected barn cat in northern California . B. bovis (previously Candidatus B. weissii), isolated from domestic cats, was kindly provided by Russell Regnery, Centers for Disease Control and Prevention (CDC), Atlanta, Georgia, USA. For DNA-DNA hybridization studies, additional Bartonella strains at the CDC included: B. quintana type strain ATCC VR-358, B. henselae 88–712, B. henselae G6486, B. henselae G6529, B. henselae G8378, B. henselae G5691, B. elizabethae type strain ATCC 49927, B. vinsonii type strain ATCC VR-152, B. vinsonii subsp. berkhoffii type strain ATCC 51672, B. clarridgeiae strain “Big Blackie,” B. bacilliformis type strain ATCC 35685, and B. bacilliformis strain KC 584.
Whole blood samples were collected for culture of Bartonella from 14 free-ranging mountain lions and 19 free-ranging bobcats selected by convenience sampling in California between January 1995 and August 2003. Nine mountain lions were trapped in seven different California counties and kept at the California Department of Fish and Wildlife (CDFW) facility, Rancho Cordova, CA, where blood samples were collected between 1995 and 1998, and five mountain lion blood samples were collected during behavioral studies in San Diego County (Cleveland National Forest) between 2001 and 2003 (Table 1). Similarly, 19 bobcats were trapped in three different counties of the California Coast Range (Table 2). Seven of the 19 bobcats were kept at the CDFW facility, where the blood samples were collected. The animals were sedated using ketamine hydrochloride (Ketaset, Fort Dodge Laboratories, Fort Dodge, Iowa 50501, USA) (11 mg/ kg). Four mountain lions and three bobcats housed at the CDFW facility had blood samples collected for bacterial isolation more than once (Tables 1 and 2). The animal use and care protocols were approved by the California Department of Fish and Wildlife (Dr. Pamela Swift) and followed during collection of blood from these animals. We operated under Protocol 10950/PHS, Animal Welfare Assurance number A3433-01, with capture and sampling procedures approved in Protocol number 17233 by the Animal Care and Use Committee at the University of California, Davis, and Memoranda of Understanding and Scientific Collecting Permits from the California Department of Fish and Wildlife (CDFW).
Blood Sample Collection
All blood samples (1.5 to 2.0 ml per tube) were collected in pediatric lysis-centrifugation tubes (Wampole Laboratories, Cranbury, N.J.) or plastic EDTA tubes (Becton Dickinson, Franklin Lakes, N.J.). Whenever possible, additional serum samples were collected simultaneously from mountain lions and bobcats into serum separating tubes, to assay for Bartonella-specific antibodies. Samples collected in pediatric lysis-centrifugation tubes were brought to the laboratory the same day, stored at 4°C and processed within 48 hours. The samples collected in EDTA tubes were stored either at -70°C or -20°C for one to two weeks, and the serum samples at -20°C, until they were processed.
The whole blood samples (approximately 1.5 to 2.0 ml) were centrifuged at 5000 x g for 30 min at room temperature (after thawing blood samples stored frozen in plastic EDTA tubes). Blood pellets were resuspended in 125 μl of M199S inoculation medium  and plated onto fresh (< 8 days old) heart infusion agar (Difco laboratories, Detroit, MI) containing 5% fresh rabbit blood (HIAR). The plates were then incubated at 35°C in 5% CO2 for four weeks, and cultures were examined at least twice weekly for bacterial growth. The number of colonies observed was recorded as the number of colony-forming units per milliliter (CFU/ml) of blood. Colonies were sub-cultured, harvested, and frozen at -70°C.
Microscopic and biochemical analyses
Gram’s staining and biochemical tests were performed on all isolates. Sterile swabs moistened with filter-sterilized, phosphate-buffered saline (PBS) were used to remove colonies from sub-cultured agar plates to glass slides. Following heat fixation, Gram’s staining was performed, and bacteria were visualized by light microscopy. The motility of cells suspended in heart infusion broth was determined with a 100x oil immersion objective. Standard methods were used to test for select preformed enzymes and carbohydrate utilization . Preformed bacterial enzyme activity was tested using the MicroScan Rapid Anaerobe ID Panel (Dade International Inc., West Sacramento, CA, USA), as previously reported .
Indirect immunofluorescence antibody (IFA) test
Antibody titers against B. henselae were determined using an IFA test . For antigen preparation, B. henselae strain U4 (U. C. Davis), a 16 S rRNA genotype II strain originally isolated from a naturally infected cat at the University of California, Davis, was cultivated with Felis catus whole fetus (FCWF) cells in tissue culture media for 3–5 days. Similarly, one of the mountain lion isolates (isolate L-42-94) was used as the antigen and was cultivated on the same cell line for 3–5 days. Infected FCWF cells were applied to each well of multi-well, super-cured heavy teflon coated slides (CelLine Associates, Inc., Neufield, NJ) and incubated for 24 hours to allow the cells to adhere to the slides. Slides were then rinsed in phosphate-buffered saline (PBS, pH 7.4), air-dried, acetone fixed, and stored at -20°C after air-drying a final time. Wildcat sera were diluted 1:64 in PBS with 5% skim milk, and added to the test wells of the slides. After washing in PBS, fluorescein-labeled, goat anti-cat IgG (Cappel, Organon Teknika Corp., Durham, NC) was used as the conjugate. Positive and negative controls were included on each test slide. Intensity of fluorescence of the bacteria was graded subjectively on a scale of 0 to 4. Fluorescence intensity ≥ 2 at a dilution of 1:64 was considered to be a qualitatively positive result, as previously described . For a quantitative result, positive sera were serially diluted (two-fold dilutions) to obtain an endpoint titer. Reading of the slides was performed independently by two readers for all serum samples.
DNA extraction and PCR
Sub-cultured colonies were scraped off agar plates and suspended in 100 μl of sterile water. The bacterial suspension was heated 15 min at 100°C and centrifuged at 15,000 × g for 10 min at 4°C . The supernatant, diluted 1:10, was then used as a template for amplification of the gltA, 16S rRNA gene, ftsZ, rpoB, ribC and groEL genes, and the 16S-23S intergenic spacer region (ITS) for either PCR-restriction fragment length polymorphism analysis (RFLP) or sequencing. Approximately 380 base pairs (bp) of the gltA gene , 1,500 bp of the 16S rRNA gene [6, 21], 900 bp of the ftsZ gene , 825 bp of the rpoB gene , 580 bp of the ribC gene , 1,500 bp of the groEL gene  and fragments of various sizes of the 16S-23S ITS  were amplified using previously described primers and methods, and verified by gel electrophoresis.
The amplified products were enzymatically digested overnight using the appropriate restriction endonucleases. The amplified product of the gltA gene was digested with TaqI (Promega, Madison, WI), HhaI (New England Biolabs, Beverly, M.A.), MseI (New England Biolabs) and AciI (New England Biolabs); the amplified product of the 16S rRNA gene was digested with DdeI (New England Biolabs); the amplified product of the ribC gene was digested with TaqI; and the amplified product of the 16S-23S ITS region was digested with TaqI and HaeIII. The digestion temperature was 65°C for TaqI and 37°C for all other enzymes. The digested fragments were separated by electrophoresis in a 3% Nusieve GTG agarose gel (Biowhittaker Molecular Applications, Rockland, ME). Fragment sizes were estimated by comparison with a 100 bp ladder (Invitrogen, Carlsbad, CA). Control samples included DNA from a strain isolated from a naturally-infected cat, confirmed previously to be B. henselae by 16S rRNA gene sequencing, and a negative control sample with no DNA template. PCR-RFLP profiles of isolates were compared with B. henselae genotype I and genotype II, B. koehlerae, B. clarridgeiae and B. bovis.
Pulsed field gel electrophoresis (PFGE)
For PFGE, a single colony of each isolate was sub-cultured to confluence (in a total of one or two passages) on HIAR at 35°C for 5–7 days in a 5% CO2 atmosphere. Bacteria grown on the agar plates were scraped off, suspended in sterile saline, and washed twice by centrifugation at 15,000 x g for 5 min at 4°C. The turbidity of the suspension was adjusted to McFarland standard 6 , and 0.5 mL of this suspension was mixed gently but thoroughly with an equal volume of 2% ultrapure low-melting-point agarose (Gibco BRL Life Technologies). The mixture was solidified in plug molds at 4°C, and the agarose plugs were transferred into lysozyme solution (10 mM Tris [pH 7.2], 50 mM NaCl, 0.2% sodium deoxycholate, 0.5% sodium lauroyl sarcosine, and 1 mg/mL lysozyme) and incubated at 37°C overnight. The plugs were rinsed with sterile water and incubated in proteinase K solution (100 mM EDTA [pH 8.0], 0.2% sodium deoxycholate, 1% sodium lauroyl sarcosine, and 1 mg/mL proteinase K) at 50°C overnight. The proteinase K incubation was repeated a second time. The plugs then were washed four times in 10 mL of washing buffer (50 mM EDTA and 20 mM Tris [pH 8.0]) for 1 h at room temperature with gentle agitation. Proteinase K was inactivated by the addition of 1 mM phenyl-methyl-sulfonyl-fluoride solution during the second wash. The plugs were stored in wash buffer at 4°C before endonuclease digestion.
Before digestion, the plugs were transferred to 1.5-mL sterile microtubes with 0.1× wash buffer at 4°C overnight and then equilibrated in 1× endonuclease-specific reaction buffer for 1 h. SmaI restriction endonuclease (New England BioLabs) was used for the analysis of total Bartonella genomic DNA from the different species and isolates by digesting bacterial chromosomal DNA in reaction buffer at 28°C overnight. After digestion, plugs were equilibrated in 0.5× TBE buffer (45 mM Tris-borate and 1 mM EDTA [pH 8.0]) for 30 min. The chromosomal restriction fragments were separated by PFGE in a CHEF-DRIII system (Bio-Rad) using a 1.5% pulsed-field certified agarose gel (Bio-Rad) in 0.5× TBE buffer. The electrophoresis was equilibrated at 14°C for 26 h at a constant voltage of 5.7 V/cm for the SmaI-digested plugs. Separation of the digested genomic DNA in plugs was achieved with pulse times of 3–10s. After electrophoresis, the gel was stained and photographed. Lambda ladder pulsed-field gel marker (48.5–970 kbp; Bio-Rad) was used for molecular weight standards. B. henselae Houston-1 (ATCC 49882) was always included as a positive control for assurance of the consistent performance of the digestion and electrophoresis conditions .
Sequencing of gene fragments for phylogenetic analysis
PCR products used for DNA sequencing were purified with QIAquick PCR purification kit (QIAGEN Sciences, Maryland) and sequencing was done using a fluorescence-based automated sequencing system (Retrogen Sequencing, San Diego, CA). For the phylogenetic analysis, forward and reverse direction sequences of the 379 bp gltA gene fragment, 935 bp ftsZ gene fragment, 893 bp rpoB gene fragment, and the various sized fragments (721 bp to 723 bp) of the 16S-23S ITS region were joined to form a concatenated sequence. Sequence data were imported into MEGA version 5.0 software (http://www.megasoftware.net) and aligned by the Clustal W program. A neighbor-joining tree was constructed  and bootstrap replicates were performed to estimate node reliability of the phylogenetic tree, with values obtained from 1000 randomly selected samples of the aligned sequence data. The evolutionary distances were computed using the Kimura’s two-parameter method .
DNA-DNA hybridization methods
Mountain lion strain L-42-94 was grown on HIAR plates at 35°C in 5% CO2 for 7 days, scraped from the agar surface and washed twice with sterile 0.1M NaCl. The methods used for DNA extraction and purification as well as the hydroxyapatite method have been described previously . DNA was labeled enzymatically in vitro with [alpha-32P] dCTP by use of a nick translation reagent kit (GIBCO BRL, Gaithersburg, Md.), according to the manufacturer's instructions. Divergence in related sequences was estimated to approximately 1% for each degree of decreased thermal stability in a heterologous re-associated DNA duplex, compared with that in the homologous re-associated DNA duplex . Calculation of divergence was to the nearest 0.5%.
Primary isolation of Bartonella species
During primary isolation, very small colonies were observed growing on HIAR plates after a minimum of 14 days following plating of the pelleted blood from four (29%) of the 14 mountain lions (Table 1) and seven (37%) of the 19 bobcats (Table 2). None of the five mountain lions from southern California had detectable bacteremia, whereas the prevalence of bacteremia was 44% (4/9) in the mountain lions from northern and central California. All bacterial colonies were homogeneous, round, grey-white in color, 0.3 to 1.0 mm in diameter and embedded in the medium, and either rough, such as for mountain lion isolate L-42-94, or smooth for bobcat isolates L-10-97, L-11-97.
Each of the three blood samples collected from mountain lion L-42-94 between January 30th, 1995 and May 3rd, 1995 yielded organisms (range: 3,200 CFU/ml in January to 60 CFU/ml in May 1995) (Table 1). Similarly, the second bacteremic mountain lion (L-27-96) had a high level of bacteremia (1,730 to 1,860 CFU/ml of blood). The third culture-positive mountain lion (L-39-97) was a young female that had been captured at eight weeks of age, at which time it was serologically negative and culture negative. This mountain lion was kept in a cage in an enclosed area. When re-tested at eight, nine and 14 months of age, the animal was bacteremic and seropositive (Table 1). The last isolate (FM98061) was from a female mountain lion kitten that was highly bacteremic (3,000 CFU/ml). We were able to document bacteremia in some of these wild felids for at least six months. In the seven bacteremic bobcats, the level of bacteremia varied from 5 CFU/ml to more than 1,000 CFU/ml (Table 2).
Microscopic and biochemical analysis
The phenotypic characteristics of the four mountain lion and seven bobcat strains were compared with B. henselae, B. koehlerae, and B. clarridgeiae (Table 3). Microscopic examination of the bacteria isolated from blood revealed short, slender Gram-negative rods. No motility was detected. Tests for catalase and urease activity were negative. By measuring preformed enzymes (Rapid Anaerobe ID Panel profile number 10477640), the strains were found to be biochemically inert except for the production of peptidases. The preformed enzyme score reading was 10077640 for three of the four mountain lion isolates and 10477640 for six of seven of the bobcat isolates. In contrast, the scores for B. henselae ATCC 49882 and B. koehlerae ATCC 700693 were 00077640 and 10073240, respectively . For one bobcat and one mountain lion isolate, the preformed enzyme profile was identical to that of B. henselae.
Serology results of samples from bobcats and mountain lions
All bacteremic bobcats and mountain lions were seropositive (titer ≥1:64), using an IFA with B. henselae genotype II antigen (strain U4, U.C. Davis). In addition, four of the 10 non-bacteremic mountain lions and six of the 12 non-bacteremic bobcats were seropositive (Tables 1 and 2). For mountain lion L-42-94, a decrease of the antibody titer was concomitant with a decline in the level of bacteremia (Table 1). IFA titers were identical or very close (within one dilution factor) when using either B. henselae or L-42-94 strain as the antigen (data not shown).
For the gltA gene, all mountain lion and bobcat isolates showed a profile similar to that of B. henselae genotype I and genotype II after digestion with HhaI (Table 4). Digestion of the gltA gene with MseI was not discriminatory, as it shared a similar profile with both B. henselae genotype I and genotype II and B. koehlerae. However, digestion with TaqI identified a profile similar to B. koehlerae for three of the four mountain lion isolates and six of the seven bobcat isolates. When using AciI endonuclease, a distinction could be made between three of the four mountain lion isolates with a profile similar to B. clarridgeiae, whereas the profile of all seven bobcats and the fourth mountain lion was similar to B. henselae and B. koehlerae (Table 4, Fig 1). One bobcat isolate (SC443) and one mountain lion isolate (FM98061) showed a profile similar to B. henselae whether using TaqI, HhaI, MseI or AciI (Table 4). For the 16S rRNA gene digested with DdeI, all mountain lion and bobcat isolates had a profile similar to B. henselae genotype II (Table 5). For the ribC gene, the profile was similar to B. henselae genotype I and genotype II when digesting with TaqI endonuclease, and the profile was similar to B. henselae genotype II for the 16S-23S ITS digested with endonucleases TaqI and HaeIII (Table 5).
Lanes 1, 4 and 19 show 100 BP Ladder; Lane 2, Mt Lion L27-96; Lane 3, Mt Lion L42-94; Lane 5, Mt Lion L-39-97; Lane 6, Mt Lion FM98061; Lane 7, Bobcat L08-96; Lane 8, Bobcat L17-96; Lane 9, Bobcat DS08; Lane 10, Bobcat L10-97; Lane 11, Bobcat L11-97; Lane 12, Bobcat SC443; lane 13, Bobcat DS507; Lane 14, B. henselae Type I; Lane 15, B. henselae Type II; Lane 16, B. clarridgeiae; Lane 17, B. koehlerae; Lane18, B. bovis (“weissii” isolate).
Pulsed field Gel Electrophoresis (PFGE)
Two mountain lion isolates (L-42-94 and L-27-96) displayed the same, very distinct and specific bands, distinguishing them from B. henselae genotype I and genotype II, and also from B. koehlerae (Fig 2). Additionally, two selected bobcat isolates (L-17-96; and L-08-96) displayed identical, very distinct and specific bands, distinguishing them from B. henselae genotype I and genotype II, from B. koehlerae, and from the mountain lion isolates (Fig 2).
Lane A1, molecular size standards (48.5 to 970 kbp); lane A2, B. henselae (type I Houston-I strain; ATCC 49882); lane A3, B. clarridgeiae (ATCC 51734); lane A4, B. koehlerae (ATCC 700693) (from reference 41); lane B1, B. henselae (type II Marseille strain; U4 U.C. Davis); lane B2, Mt Lion strain L42-94; lane B3, Mt Lion L27-96; lane B4, Bobcat strain L-17-96 (this study).
Sequencing of gltA, rpoB and ftsZ gene fragments and a 16S-23S ITS fragment for phylogenetic analysis
The sequence of 379 bp in the 3’-end of the gltA gene was determined for the strains isolated from mountain lions and for the strains isolated from bobcats (Fig 3 includes, as an example, two representative mountain lion strains [L-42-94, FM98061] and two representative bobcat strains [SC443, L-17-96]). Mountain lion isolates L-42-94, L-39-97 and L-27-96 (GenBank Accession Numbers: KF246521, KF246522 and KF246523, respectively [Table 6]) matched 100%, and bobcat isolates L-08-96, L-17-96, DS08, L-10-97, L-11-97 and DS507 (GenBank Accession Numbers: KF246529, KF246528, KF246524, KF246527, KF246526, and KF246525, respectively) matched 100% (Table 7). The alignment between the mountain lion and bobcat isolate sequences showed one bp substitution (a C in bobcat isolates and a T in mountain lion isolates), which translates to a synonymous amino acid. The gltA sequence of bobcat Sc443 (GenBank #KF466249) was 100% identical to B. henselae. The gltA sequences of mountain lion FM98061 (GenBank #KF466248) and bobcat isolate L-17-96 shared 94% homology with B. henselae (16 to 17 bp difference) and 95.6% homology with B. koehlerae (10 to 11 bp difference). All other gltA gene sequences available in the EMBL-GenBank database had a lower percent similarity (<93% similarity) when compared to these bobcat and mountain lion gltA sequences. When the corresponding, predicted amino acid sequences of the gltA genes were compared, all wild felid sequences were identical to each other, and four amino acids among 120 (3%) remained different from the amino acid sequence of the B.henselae gltA gene.
The phylogenetic tree was constructed from 270 bp sequences, inferred using the Neighbor-Joining method, and 1000 replicates in the bootstrap test. Scale bar indicates 5 substitutions per nucleotide position.
The sequence of 893 bp in the 3’-end of the rpoB gene also was determined for the strains isolated from mountain lions and from bobcats (Fig 4 includes, as an example, two representative mountain lion strains [L-42-94, FM98061] and three bobcat strains [SC443, DS08 and L-17-96]). The rpoB gene sequences of bobcat Sc443 (GenBank #KF466253) and mountain lion FM98061 (GenBank #KF466252) were 100% identical and 99.6% identical to B. henselae (1 bp difference), but translated to the same amino acid as B. henselae rpoB. The sequences of the other mountain lion isolates (GenBank #KF246539 [L-42-94]; #KF246540 [L-39-97]; and #KF246541 [L-27-96]) matched 100% to each other, as well as most bobcat isolates (GenBank #KF246542 [DS507]; #KF246543 [L-11-97]; #KF246544 [L-10-97]; #KF246545 [L-17-96]; and #KF246546 [L-08-96]) all matched 100%, but shared a 96.6 to 97% homology with B. henselae (23 to 26 bp difference) and 96.5% homology with B. koehlerae (26 to 27 bp difference). However, bobcat isolate DS08 (GenBank #KF246547) had one bp substitution leading to a non-synonymous amino acid change. The alignment between the mountain lion and bobcat isolate sequences showed three bp substitutions; two of the substitutions were synonymous and the third substitution was non-synonymous but conserved (mountain lion: valine versus bobcat: alanine). All other rpoB gene sequences available in the EMBL-GenBank database had a lower percent similarity (< 93%).
The phylogenetic tree was constructed from 771 bp sequences, inferred using the Neighbor-Joining method, and 1000 replicates in the bootstrap test. Scale bar indicates 5 substitutions per nucleotide position.
A 935 bp fragment of the ftsZ gene also was analyzed. The ftsZ sequences from mountain lion isolates L-42-94, L-27-96 and l-39-97 (GenBank accession numbers: KF246530, KF246532 and KF246531, respectively) matched 100%, and ftsZ sequences from bobcat isolates L-08-96, L-17-96, DS08, L-10-97, L-11-97 and DS507 matched 100% (GenBank accession numbers: KF246538, KF246537, KF246533, KF246536, KF246535 and KF246534, respectively, Table 6). Alignment between mountain lion and bobcat isolate sequences showed two bp substitutions, which translated to a synonymous amino acid sequence. The ftsZ sequences for mountain lion isolate FM98061 (GenBank #KF466250) and bobcat isolate SC443 (GenBank #KF466251) matched 100%, and the ftsZ sequence of both isolates had one bp substitution compared to the corresponding ftsZ fragment in B. henselae. However, the substitution still translated to the same amino acid as B. henselae ftsZ.
Sequences for the 16S-23S ITS region from mountain lion isolates L-42-94, l-27-96 and l-39-97 matched 100% (GenBank #KF437493, KF437495, and KF437494, respectively), and sequences from bobcat isolates L-08-96, L-17-96, L-10-97, L-11-97 and DS507 matched 100% (GenBank #KF437501, KF437500, KF437499, KF437498, and KF437497, respectively, Table 6). However, bobcat isolate DS08 had one mutation compared to the other bobcat isolates. Mountain lion isolate FM98061 and bobcat isolate SC443 16S-23S ITS region sequences matched 100% (GenBank #KF466254 and KF466255, respectively). When compared to the corresponding 16S-23S ITS fragment sequence in B. henselae, the 16S-23S ITS sequences of both these isolates had three bp substitutions. Insertions and deletions (five total) in the 16S-23S ITS region sequence resulted in a fragment of: 723 bp in size for bobcat isolates L-08-96, L-17-96, L-10-97, L-11-97, DS507 and DS08; 722 bp for mountain lion isolate FM98061 and bobcat isolate SC443; and 721 bp for mountain lion isolates L-42-94, L-27-96, L-39-97.
Phylogenetic analysis based on concatenated sequences of gene fragments
Analysis of concatenated fragments of the gltA, ftsZ and rpoB genes and the 16S-23S rRNA ITS showed that three of the four mountain lion isolates were identical and clustered together. The six bobcat isolates were identical and were most closely related to, but distinct from, these three mountain lion isolates (Fig 5). They branched on a tree that also included B. koehlerae and B. henselae. As observed by PCR-RFLP, the two isolates from mountain lion FM98061 and bobcat SC443 were clustered with B. henselae.
DNA-DNA hybridization studies
Levels of DNA relatedness were determined by hybridizing labeled DNA from the mountain lion isolate L-42-94, the type strain of B. koehlerae (ATCC 700693), the type strain of B. henselae (ATCC 49882), and an additional strain of B. henselae (G6486) (Table 7, top horizontal row) with unlabeled DNA from L-42-94 and 14 Bartonella species or subspecies (Table 7, far left column). Labeled DNA from the type strain of B. koehlerae had an average relatedness to the mountain lion strain L-42-94 of 87% with 6.5% divergence in optimal DNA reassociation reactions at 55°C. In stringent DNA reassociation reactions at 70°C, they were 55% related. Labeled DNA from the type strain of B. henselae showed a relatedness to the mountain lion Bartonella isolate L-42-94 of 75% at 55°C with 7.0% divergence, and 43% at 70°C.
Using labeled L-42-94 DNA hybridized with unlabeled DNA from the type strain of B. koehlerae, the mountain lion L-42-94 DNA showed a relatedness of 75% at 55°C with 5.5% divergence, and of 59% at 70°C (Table 7). Using labeled L-42-94 DNA hybridized with unlabeled DNA from the type strain of B. henselae, L-42-94 showed a relatedness of 77% at 55°C with 6.0% divergence, and of 48% at 70°C. Based on DNA hybridization studies, our isolate L-42-94 was most closely related to B. koehlerae: range and relatedness of L-42-94 to the type strain of B. koehlerae was 75% to 87%, with 5.5% to 6.5% divergence at 55°C; range and relatedness of L-42-94 to the type strain of B. henselae was 75% to 77%, with 6.0% to 7.0% divergence at 55°C. The relatedness of L-42-94 to type strains B. quintana ATCC VR-358, B. vinsonii ATCC VR-152, and B. elizabethae ATCC 49927 ranged from 52% to 68% at 55°C. DNA from L-42-94 was least related (35% to 48%) to B. clarridgeiae strain “Big Blackie” and B. bacilliformis strain KC 584 by DNA-DNA hybridization studies.
Numerous studies have demonstrated the high prevalence of prolonged B. henselae bacteremia in domestic cats of northern California and the subsequent risk of cat scratch disease in their owners [1, 5, 18]. In addition, it has been well documented that infectious organisms can be readily transferred from wild mammals to domestic pets or humans, either directly, or via an arthropod vector . We therefore sought to determine whether wild felids in northern California provide a bacteremic reservoir for Bartonella, and if so, to define the infecting Bartonella species. In this study, we report the isolation of B. henselae and the first isolation of two new B. koehlerae subspecies from free-ranging wild felids in North America.
Evidence of Bartonella infection in wild felids in northern California was first reported in bobcats from Marin County, CA, when serum testing revealed seroreactivity to B. henselae antigen in 74% of 25 bobcats . More recently, Bartonella DNA was detected in strongly seropositive California mountain lions, and sequences of amplified DNA fragments were reported to be identical to B. henselae . Bartonella spp. also have been found in African felids. Kelly et al.  reported the isolation of B. henselae from an African cheetah from Zimbabwe. Similarly, B. henselae and an unidentified Bartonella strain with a PCR-RFLP profile similar to B. koehlerae were isolated from African free-ranging lions (Panthera leo) from Kruger National Park, South Africa . Moreover, B. henselae was isolated from semi-captive lions from three ranches in the Free State Province, South Africa .
In our study, we found a prevalence of Bartonella bacteremia in 29% and 37% of California mountain lions and bobcats, respectively, providing further evidence that Bartonella bacteremia is common in free-ranging wild felids. Such a prevalence of Bartonella bacteremia is similar to what has been reported for B. henselae in domestic cats from northern California [5, 18], as well as for Bartonella spp. from other wild carnivores in northern California, including 42% of 53 gray foxes (Urocyon cinereoargenteus) infected with B. rochalimae , 28% of 109 coyotes (Canis latrans) infected with B. vinsonii subsp. berkhoffii  in central California, and 26% of 42 raccoons (Procyon lotor) bacteremic with B. rochalimae . Domestic cats are the only previously known, culture-positive reservoir of B. henselae, B. clarridgeiae and B. koehlerae . In this study, we demonstrated that wild felids from California are likely the natural reservoirs of several Bartonella species, and they can be long-term carriers of these Bartonella spp, as previously documented in domestic cats [3, 36].
The strains isolated from mountain lions and bobcats were morphologically similar to B. henselae, but were not apparent on blood agar until two weeks after plating. In contrast, after culturing blood of infected domestic cats, B. henselae colonies are usually visible within a few days. This characteristic of two weeks’ incubation time to appearance of colonies also was observed in domestic specific-pathogen free kittens experimentally infected with one of the mountain lion isolates .
The biochemical profiles of mountain lion and bobcat isolates were consistent with the general profile observed for Bartonella species. RFLP analysis of a PCR-amplified gltA gene fragment indicated that two endonucleases, TaqI and AciI, are useful to specifically distinguish the mountain lion and bobcat strains from each another and from B. henselae and B. koehlerae. By pulsed field gel electrophoresis and sequencing of the 16S rRNA gene, it appeared that these wild felid isolates are different from any isolate found in domestic cats. PFGE band patterns were identical for three of the four mountain lion isolates but differed from the bobcat isolates. However, one bobcat and one mountain lion were infected not with a new Bartonella subspecies, but with B. henselae, suggesting that diverse Bartonella species can infect these two mammalian reservoir species.
DNA-DNA hybridization remains a reliable method for defining a species. It has been recommended that a species consists of strains whose DNA is ≥70% related at optimal re-association conditions, ≥55% related under stringent DNA re-association conditions, and also, whose DNA contains ≤5% divergence within related sequences [29, 38]. Labeled DNA from L-42-94 showed relatedness to the type strain of B. koehlerae of 75% (with 5.5% divergence) at 55°C, and 59% at 70°C. The percent DNA relatedness was higher in reciprocal reactions at 55°C but not at 70°C, where labeled DNA from the type strain of B. koehlerae showed a relatedness to the Bartonella mountain lion isolate L-42-94 of 87% (with 6.5% divergence) at 55°C, and 55% at 70°C. Relatedness values that demonstrate non-reciprocity have been identified in strains from many genera, and this finding emphasizes the importance of performing reciprocal DNA relatedness when studying strains that are close to the species definition. Non-reciprocity can be observed when the genomes of the two species being compared are of different sizes . For relatedness under stringent conditions, the mountain lion isolate L-42-94 fulfills the strict criteria for belonging to the same species as B. koehlerae. However, for divergence, L-42-94 does not fulfill the strict criteria for belonging to the same species as B. koehlerae, and thus, L-42-94 meets the criteria for being a subspecies of B. koehlerae.
In natural conditions, it appears that free-ranging wild cats can be infected with Bartonella species found in domestic cats, as demonstrated by the isolation of B. henselae genotype II from a very young bobcat and a young mountain lion. The juvenile mountain lion was held in the CDFW facility; therefore, it is difficult to determine if this specific strain was acquired when this animal was kept in captivity or prior to its rescue from the wild. The strain from the bobcat could have been acquired by exposure to fleas from domestic cats, because stray cats are common in the area where this young bobcat was found (Daren Simpson, personal communication). These results clearly show that B. henselae can naturally infect both domestic cats and wild free-ranging felids.
Of note, the novel strains isolated from the mountain lions and bobcats appear to be highly adapted to their specific host, and could have evolved and adapted from a common Bartonella ancestor within these specific populations. Interestingly, these isolates are phylogenetically intermediate between B. henselae and B. koehlerae, two species for which domestic cats are the main known reservoir. Further studies should be conducted to investigate the evolution of these different Bartonella species among domestic and wild felids. To date, neither of these new Bartonella subspecies has been isolated from domestic cats. However, we previously demonstrated  that domestic cats represent a permissive host for experimental infection with a mountain lion Bartonella isolate (strain L-42-94). We also found that there was no cross-protection between this strain and Bartonella strains that infect domestic felines . We were not able to identify any natural infection of these California free-ranging wild felids with B. clarridgeiae or B. koehlerae, the two Bartonella species that are less commonly isolated from domestic cats in the western USA . The small sample size we tested may not have been sufficient for detection of these two Bartonella species from wild-ranging felids.
The zoonotic potential of these novel Bartonella isolates is unknown. Mountain lion and bobcat attacks on humans are quite rare. However, over the past several decades, the incidence of mountain lion attacks on people has been slowly increasing, with more events occurring during the past 22 years than in the last century . There were 50 documented attacks on children with a 25% fatality rate out of 83 documented mountain lion attacks over the last 100 years . Most children were not alone at the time of the attack (92%), and in many instances adult supervision was present or nearby. Severe head and neck lacerations along with puncture wounds were the most common injuries. Disease transmission in such encounters is also possible, as illustrated by two people who developed Pasteurella infection after being attacked. Additionally, two mountain lions implicated in attacks on humans were confirmed to be rabid . A case of Pasteurella multocida infection also was acquired following a bite by a pet mountain lion . No evidence of cat scratch disease was observed in this case, but the pet had previously been declawed. Potential exposure to ectoparasites infected with Bartonella, especially fleas infesting a mountain lion or a bobcat, could be a risk factor for humans, because fleas have been shown to effectively transmit B. henselae between cats . Additional research is needed to definitively identify the vector and mode of transmission of Bartonella between wild felids.
It is most likely that the northern California bobcats and mountain lions are naturally infected with novel Bartonella species or subspecies that are specific to each felid species, and in addition, sometimes can be infected with B. henselae. This is based on our findings that a) we were able to differentiate the mountain lion isolates from the bobcat isolates by RFLP, PFGE, and partial sequencing of at least four different genes; but b) we could not differentiate between isolates from the same reservoir species; and c) these isolates from bobcats and mountain lions were closely related to, but distinct from, the reference B. henselae and B. koehlerae strains.
The criteria established by La Scola et al.  to define a new Bartonella species indicate that the percentage of similarity should be ≤96% for gltA and ≤95.6% for rpoB. However, with these two Bartonella isolates, the similarity values were below the threshold for gltA (94%-95.6%) gene, but above the threshold for rpoB (96.6% to 97%) gene, and thus these two novel Bartonella isolates are located phylogenetically between B. henselae and B. koehlerae. Because DNA-DNA hybridization reveals that L-42-94 is more closely related to B. koehlerae than B. henselae, we propose creating two new subspecies of B. koehlerae: B. koehlerae subsp. boulouisii and B. koehlerae subsp. bothieri, for which mountain lions and bobcats are the respective natural reservoirs. The identification of a cognate and unique mammalian reservoir for each of these two novel subspecies also should be noted.
Emendation of the description of Bartonella koehlerae
Bartonella koehlerae (Droz S, Chi B, Horn E, Steigerwalt AG, Whitney AM, Brenner DJ. 1999). The characteristics of this taxon are the same as those described for the genus  and those described by Droz et al.  for the species. The species now contains three subspecies: one that was isolated previously from domestic cats and humans [4, 44, 45]; another that was isolated only from mountain lions (Puma concolor); and the third that was isolated only from bobcats (Lynx rufus).
Description of Bartonella koehlerae subsp. koehlerae subsp. nov.
Bartonella koehlerae subsp. koehlerae subsp. nov. (koeh′ ler. ae. N. L. fem. adj. koehlerae. The type strain C-29 (ATCC 700693) was recovered from the blood of a healthy kitten during a prevalence study of B. henselae in domestic cats in the greater San Francisco Bay area, northern California .
Description of Bartonella koehlerae subsp. boulouisii subsp. nov.
Bartonella koehlerae subsp. boulouisii (bou. lou. is′ i. i. N. L. gen. masc. n. boulouisii of Boulouis, in honor of Henri-Jean Boulouis, a veterinary microbiologist and professor at the School of Veterinary Medicine in Maisons-Alfort, France, whose wide interest in the field of Bartonella infections in animals and humans led to the isolation of several new Bartonella species). The main phenotypic characteristics are identical to those of the genus Bartonella. The strain is oxidase and catalase negative. Primary isolation from mountain lion blood occurred on HIAR agar, where the first colonies were observed after 14 days of incubation at 35°C in a candle jar (with a CO2-enriched environment). The code for preformed enzymes obtained in the MicroScan Rapid Anaerobe Panel is 10077640. The new B. koehlerae subspecies shows a unique PCR-RFLP pattern for the citrate synthase gene (gltA) and a unique PFGE pattern that differs from those of B. henselae and B. koehlerae. The type strain, L-42-94, recovered from the blood of a mountain lion (Puma concolor) during a prevalence study of Bartonella infections in wild cats in northern California, has been deposited at the ATCC, USA (ATCC BAA-2635; http://www.atcc.org/) and at the Collection of Institut Pasteur (CIP), Paris, France.
Description of Bartonella koehlerae subsp. bothieri subsp. nov.
B. koehlerae subsp. bothieri (bo.thi'er.i. N.L. masc. gen. n. bothieri, of Bothier, in honor of François Bothier, a French physician and hematologist from Lyon, France, specialist of blood and blood-borne diseases). The main phenotypic characteristics are identical to those of the genus Bartonella. The strain is oxidase and catalase negative. Primary isolation from bobcat blood occurred on HIAR agar, where the first colonies were observed after 14 days of incubation at 35°C in a candle jar (with a CO2-enriched environment). The code for preformed enzymes obtained in the MicroScan Rapid Anaerobe Panel is 10477640. The new B. koehlerae subspecies shows a unique PCR-RFLP pattern for the citrate synthase gene (gltA) PCR-RFLP and a unique PFGE pattern, which are different from those of B. henselae and B. koehlerae. The type strain, L-17-96, recovered from the blood of a bobcat (Lynx rufus) during a prevalence study of Bartonella infections in wild cats in northern California, has been deposited at the ATCC, USA (ATCC BAA-2636; http://www.atcc.org/) and at the Collection of Institut Pasteur (CIP), Paris, France.
The authors thank Darren Simpson for trapping the mountain lions and bobcats in central California and Dr. Pamela Swift for allowing access to the animals kept at the Wildlife Investigations Laboratory, California Department of Fish and Wildlife, Rancho Cordova, CA, as well as Walter Boyce and Grace Lee for providing the blood of the mountain lions from the San Diego Mountains. The authors also thank K.R. Jones, California Department of Fish and Wildlife, and K.A. Floyd-Hawkins, Department of Medicine and Epidemiology, School of Veterinary Medicine, University of California, Davis, for their technical assistance. The authors thank Arnold G. Steigerwalt for performing the DNA-DNA hybridization, and Don J. Brenner for his thoughtful comments on the manuscript. This project was funded in part by the George and Phyllis Miller Feline Research Fund, Center for Companion Animal Health, University of California, Davis, the Master of Preventive Veterinary Medicine Research Project Fund (University of California, Davis) and Mérial Inc., Athens, GA. Sophie Molia was a recipient of a Lavoisier grant (French Ministry of Foreign Affairs) and a Barron fellowship (University of California, Davis). Jane E. Koehler received funding support from a Burroughs Wellcome Fund Clinical Scientist Award in Translational Research, a California HIV Research Program Award, and NIH grants U54AI065359 and R01AI103299 from the NIAID.
Conceived and designed the experiments: BBC JEK. Performed the experiments: RWK CCC S. Maruyama S. Molia GMB BBC. Analyzed the data: BBC MJS CCC. Contributed reagents/materials/analysis tools: NH S. Maruyama CCC. Wrote the paper: BBC JEK.
- 1. Boulouis HJ, Chang CC, Henn JB, Kasten RW, Chomel BB (2005) Factors associated with the rapid emergence of zoonotic Bartonella infections. Vet Res 36: 383–410. pmid:15845231.
- 2. Chomel BB, McMillan-Cole AC, Kasten RW, Stuckey MJ, Sato S, Maruyama S, et al. (2012) Candidatus Bartonella merieuxii, a potential new zoonotic Bartonella species in canids from Iraq. PLoS Negl Trop Dis 6, e1843. doi: 10.1371/journal.pntd.0001843. pmid:23029597
- 3. Abbott RC, Chomel BB, Kasten RW, Floyd-Hawkins KA, Kikuchi Y, Koehler JE, et al. (1997) Experimental and natural infection with Bartonella henselae in domestic cats. Comp Immunol Microbiol Infect Dis 20: 41–45. pmid:9023040.
- 4. Droz S, Chi B, Horn E, Steigerwalt AG, Whitney AM, Brenner DJ (1999) Bartonella koehlerae sp. nov., isolated from cats. J Clin Microbiol 37: 1117–1122. pmid:10074535
- 5. Koehler JE, Glaser CA, Tappero JW (1994) Rochalimaea henselae infection. A new zoonosis with the domestic cat as reservoir. JAMA 271: 531–535. pmid:8301768
- 6. Regnery RL, Anderson BE, Clarridge JE III, Rodriguez-Barradas MC, Jones DC, Carr JH (1992) Characterization of a novel Rochalimaea species, R. henselae sp. nov., isolated from blood of a febrile, human immunodeficiency virus-positive patient. J Clin Microbiol 30: 265–274. pmid:1371515
- 7. Yamamoto K, Chomel BB, Kasten RW, Hew CM, Weber DK, Lee WI, et al. (2002) Experimental infection of domestic cats with Bartonella koehlerae and comparison of protein and DNA profiles with those of other Bartonella species infecting felines. J Clin Microbiol 40: 466–474. pmid:11825958
- 8. Breitschwerdt EB, Maggi RG, Sigmon B, Nicholson WL (2007) Isolation of Bartonella quintana from a woman and a cat following putative bite transmission. J Clin Microbiol 45: 270–272. pmid:17093037.
- 9. Varanat M, Travis A, Lee W, Maggi RG, Bissett SA, Linder KE, et al. (2009) Recurrent osteomyelitis in a cat due to infection with Bartonella vinsonii subsp. berkhoffii genotype II. J Vet Intern Med 23: 1273–1277. doi: 10.1111/j.1939-1676.2009.0372.x. pmid:19709358
- 10. Paul-Murphy J, Work T, Hunter D, McFie E, Fjelline D (1994) Serologic survey and serum biochemical reference ranges of the free-ranging mountain lion (Felis concolor) in California. J Wild Dis 30: 205–215.
- 11. Yamamoto K, Chomel BB, Lowenstine LJ, Kikuchi Y, Phillips LG, Barr BC, et al. (1998) Bartonella henselae antibody prevalence in free-ranging and captive wild felids from California. J Wildl Dis 34: 56–63. pmid:9476226
- 12. Girard YA, Swift P, Chomel BB, Kasten RW, Fleer K, Foley JE, et al. (2012) Zoonotic vector-borne bacterial pathogens in California mountain lions (Puma concolor), 1987–2010. Vector Borne Zoonotic Dis 12: 913–921. doi: 10.1089/vbz.2011.0858. pmid:22925024
- 13. Bevins SN, Carver S, Boydston EE, Lyren LM, Alldredge M, Logan KA, et al. (2012) Three pathogens in sympatric populations of pumas, bobcats, and domestic cats: implications for infectious disease transmission. PLoS One. 7, e31403 doi: 10.1371/journal.pone.0031403. pmid:22347471
- 14. Rotstein DS, Taylor SK, Bradley J, Breitschwerdt EB (2000) Prevalence of Bartonella henselae antibody in Florida panthers. J Wildl Dis 36: 157–160. pmid:10682759
- 15. Chomel BB, Kikuchi Y, Martenson JS, Roelke-Parker ME, Chang CC, Kasten RW, et al. (2004) Seroprevalence of Bartonella infection in American free-ranging and captive pumas (Puma concolor) and bobcats (Lynx rufus). Vet Res 35: 233–241. pmid:15099499
- 16. MacFadding JF (1980) Biochemical tests for identification of medical bacteria. 2nd Ed. Williams and Wilkins Co, Baltimore, Md.
- 17. Welch DF, Hensel DM, Pickett DA, San Joaquin VH, Robinson A, Slater LN (1993) Bacteremia due to Rochalimaea henselae in a child: practical identification of isolates in the clinical laboratory. J Clin Microbiol 31: 2381–2386. pmid:8408560
- 18. Chomel BB, Abbott RC, Kasten RW, Floyd-Hawkins KA, Kass PH, Glaser CA, et al. (1995) Bartonella henselae prevalence in domestic cats in California: risk factors and association between bacteremia and antibody titers. J Clin Microbiol 33: 2445–2450. pmid:7494043
- 19. Chang CC, Kasten RW, Chomel BB, Simpson DC, Hew CM, Kordick DL, et al. (2000) Coyotes (Canis latrans) as the reservoir for a human pathogenic Bartonella sp.: molecular epidemiology of Bartonella vinsonii subsp. berkhoffii infection in coyotes from central coastal California. J Clin Microbiol 38: 4193–4200. pmid:11060089
- 20. Norman AF, Regnery R, Jameson P, Greene C, Krause DC (1995) Differentiation of Bartonella-like isolates at the species level by PCR-restriction fragment length polymorphism in the citrate synthase gene. J Clin Microbiol 33: 1797–1803. pmid:7545181
- 21. Gurfield AN, Boulouis HJ, Chomel BB, Kasten RW, Heller R, Bouillin C, et al. (2001) Epidemiology of Bartonella infection in domestic cats in France. Vet Microbiol 80: 185–198. pmid:11295338
- 22. Zeaiter Z, Liang Z, Raoult D (2002) Genetic classification and differentiation of Bartonella species based on comparison of partial ftsZ gene sequences. J Clin Microbiol 40: 3641–3647. pmid:12354859
- 23. Renesto P, Gouvernet J, Drancourt M, Roux V, Raoult D (2001) Use of rpoB gene analysis for detection and identification of Bartonella species. J Clin Microbiol 39: 430–437. pmid:11158086
- 24. Johnson G, Ayers M, McClure SC, Richardson SE, Tellier R (2003) Detection and identification of Bartonella species pathogenic for humans by PCR amplification targeting the riboflavin synthase gene (ribC). J Clin Microbiol 41: 1069–1072. pmid:12624031
- 25. Marston EL, Sumner JW, Regnery RL (1999) Evaluation of intraspecies genetic variation within the 60 kDa heat-shock protein gene (groEL) of Bartonella species. Int J Syst Bacteriol 49: 1015–1023. pmid:10425758
- 26. Rolain JM, Gouriet F, Enea M, Aboud M, Raoult D (2003) Detection by immunofluorescence assay of Bartonella henselae in lymph nodes from patients with cat scratch disease. Clin Diagn Lab Immunol 10: 686–691. pmid:12853405
- 27. Tamura K, Peterson D, Peterson N, Stecher G, Nei M, Kumar S (2011) MEGA5: molecular evolutionary genetics analysis using maximum likelihood, evolutionary distance, and maximum parsimony methods. Mol Biol Evol 28: 2731–2739. doi: 10.1093/molbev/msr121. pmid:21546353
- 28. Kimura M (1980) A simple method for estimating evolutionary rates of base substitutions through comparative studies of nucleotide sequences. J Mol Evol 16: 111–120. pmid:7463489
- 29. Brenner DJ, McWhorter AC, Knutson JK, Steigerwalt AG (1982) Escherichia vulneris: a new species of Enterobacteriaceae associated with human wounds. J Clin Microbiol.; 15(6): 1133–1140. pmid:7107843
- 30. Riley SP, Foley JE, Chomel BB (2004) Exposure to feline and canine pathogens in bobcats and gray foxes in urban and rural zones of a national park in California. J Wildl Dis 40: 11–22. pmid:15137484
- 31. Kelly PJ, Rooney JJA, Marston EL, Jones DC, Regnery RL (1998) Bartonella henselae isolated from cats in Zimbabwe. Lancet 351: 1706.
- 32. Molia S, Chomel BB, Kasten RW, Leutenegger CM, Steele BR, Marker L, et al. (2004) Prevalence of Bartonella infection in wild African lions (Panthera leo) and cheetahs (Acinonyx jubata). Vet Microbiol 100: 31–41. pmid:15135511
- 33. Pretorius AM, Kuyl JM, Isherwood DR, Birtles RJ (2004) Bartonella henselae in African lion, South Africa. Emerg Infect Dis 10: 2257–2258. pmid:15672532
- 34. Henn JB, Gabriel MW, Kasten RW, Brown RN, Theis JH, Foley JE, et al. (2007) Gray foxes (Urocyon cinereoargenteus) as a potential reservoir of a Bartonella clarridgeiae-like bacterium and domestic dogs as part of a sentinel system for surveillance of zoonotic arthropod-borne pathogens in northern California. J Clin Microbiol 45: 2411–2418. pmid:17553970
- 35. Henn JB, Chomel BB, Boulouis HJ, Kasten RW, Murray WJ, Bar-Gal GK, et al. (2009) Bartonella rochalimae in raccoons, coyotes, and red foxes. Emerg Infect Dis. 15: 1984–1987. doi: 10.3201/eid1512.081692. pmid:19961681
- 36. Chomel BB, Boulouis HJ, Maruyama S, Breitschwerdt EB (2006) Bartonella spp. in pets and effect on human health. Emerg Infect Dis 12: 389–394. pmid:16704774
- 37. Yamamoto K, Chomel BB, Kasten RW, Chang CC, Tseggai T, Decker PR, et al. (1998) Homologous protection but lack of heterologous-protection by various species and types of Bartonella in specific pathogen-free cats. Vet Immunol Immunopathol 65: 191–204. pmid:9839874
- 38. Wayne LG, Brenner DJ, Colwell RR, Grimont PAD, Kandler O, Krichevsky MI, et al. (1987) Report of the ad hoc committee on reconciliation of approaches to bacterial systematics. Int J Syst Bacteriol 37:463–464.
- 39. Kadesky KM, Manarey C, Blair GK, Murphy JJ III, Verchere C, Atkinson K (1998) Cougar attacks on children: injury patterns and treatment. J Pediatr Surg 33: 863–865. pmid:9660216
- 40. Kizer KW (1989) Pasteurella multocida infection from a cougar bite. A review of cougar attacks. West J Med 150: 87–90. pmid:2660410
- 41. Chomel BB, Kasten RW, Floyd-Hawkins K, Chi B, Yamamoto K, Roberts-Wilson J, et al. (1996) Experimental transmission of Bartonella henselae by the cat flea. J Clin Microbiol 34: 1952–1956. pmid:8818889
- 42. La Scola B, Zeaiter Z, Khamis A, Raoult D (2003) Gene-sequence-based criteria for species definition in bacteriology: the Bartonella paradigm. Trends Microbiol 11: 318–321. pmid:12875815
- 43. Brenner DJ, O'Connor SP, Winkler HH, Steigerwalt AG (1993) Proposals to unify the genera Bartonella and Rochalimaea, with descriptions of Bartonella quintana comb. nov., Bartonella vinsonii comb. nov., Bartonella henselae comb. nov., and Bartonella elizabethae comb. nov., and to remove the family Bartonellaceae from the order Rickettsiales. Int J Syst Bacteriol 43(4):777–786. pmid:8240958
- 44. Avidor B, Graidy M, Efrat G, Leibowitz C, Shapira G, Schattner A, et al. (2004) Bartonella koehlerae, a new cat-associated agent of culture-negative human endocarditis. J Clin Microbiol. 2004;42(8):3462–8. pmid:15297484.
- 45. Breitschwerdt EB, Maggi RG, Robert Mozayeni B, Hegarty BC, Bradley JM, Mascarelli PE (2010) PCR amplification of Bartonella koehlerae from human blood and enrichment blood cultures. Parasite Vectors 3: 76.