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J Clin Microbiol. 2003 November; 41(11): 5327–5332.
PMCID: PMC262474

Isolation of Bartonella washoensis from a Dog with Mitral Valve Endocarditis

Abstract

We report the first documented case of Bartonella washoensis bacteremia in a dog with mitral valve endocarditis. B. washoensis was isolated in 1995 from a human patient with cardiac disease. The main reservoir species appears to be ground squirrels (Spermophilus beecheyi) in the western United States. Based on echocardiographic findings, a diagnosis of infective vegetative valvular mitral endocarditis was made in a spayed 12-year-old female Doberman pinscher. A year prior to presentation, the referring veterinarian had detected a heart murmur, which led to progressive dyspnea and a diagnosis of congestive heart failure the week before examination. One month after initial presentation, symptoms worsened. An emergency therapy for congestive heart failure was unsuccessfully implemented, and necropsy evaluation of the dog was not permitted. Indirect immunofluorescence tests showed that the dog was strongly seropositive (titer of 1:4,096) for several Bartonella antigens (B. vinsonii subsp. berkhoffii, B. clarridgeiae, and B. henselae), highly suggestive of Bartonella endocarditis. Standard aerobic and aerobic-anaerobic cultures were negative. However, a specific blood culture for Bartonella isolation grew a fastidious, gram-negative organism 7 days after being plated. Phenotypic and genotypic characterizations of the isolate, including partial sequencing of the citrate synthase (gltA), groEL, and 16S rRNA genes, indicated that this organism was identical to B. washoensis. The dog was seronegative for all tick-borne pathogens tested (Anaplasma phagocytophilum, Ehrlichia canis, and Rickettsia rickettsii), but the sample was highly positive for B. washoensis (titer of 1:8,192) and, according to indirect immunofluorescent-antibody assay, weakly positive for phase II Coxiella burnetii infection.

CASE REPORT

On 2 August 2001, a spayed 12-year-old female mixed Doberman pinscher dog weighing 30 kg presented to the Veterinary Centers of America Emergency Animal Hospital and Referral Center for evaluation of a murmur by a board-certified cardiologist. One year prior to presentation, the referring veterinarian had detected a heart murmur and placed the patient on a treatment regimen of 0.33 mg of enalapril/kg of body weight per os (p.o.) twice daily (BID). One week prior to referral, the patient had been evaluated for progressive dyspnea. Thoracic radiographs performed at that time revealed moderate cardiomegaly and severe enlargement of the left atrium, as well as a mild perihilar pulmonary interstitial pattern. A solitary pulmonary nodule, approximately 2 cm in diameter, was also visible within the left caudal lung lobe. Based on thoracic radiographic changes, a presumptive diagnosis of congestive heart failure was made, and the patient was placed on a regimen of 1.67 mg of furosemide/kg p.o. BID. Other diagnostics performed at that time included a serum chemistry profile, a complete blood count, and a measurement of the serum thyroxine concentration. The diagnostics were unremarkable with the exception of mild monocytopenia (990 monocytes/μl; normal range, 1,000 to 4,800/μl) and mild hyperchloridemia (116 meq/liter; normal range, 105 to 115 meq/liter).

The history for the patient included intermittent incontinence that was managed with diethylstilbestrol twice weekly and degenerative joint disease that was treated with intermittent therapy with various nonsteroidal anti-inflammatory agents. Therapy with levothyroxine (0.02 mg/kg p.o. BID) had been carried out for 2 years for hypothyroidism. At 3 years of age, the patient underwent bilateral surgical correction of ruptured cranial cruciate ligaments. The patient also had a previous history of exposure to ticks and fleas.

On presentation to the cardiologist (A. C. Wey), the patient was tachycardic (160 beats/min) but normothermic (39°C, 102.2°F) with a normal respiratory rate of 28 breaths/min. Physical examination revealed multiple soft, small (<1-cm) cutaneous nodules consistent with lipomas. On thoracic auscultation, a grade IV to VI systolic murmur in the left apex was present, as well as an S3 gallop sound and an occasional arrhythmia with pulse deficits. The patient was slow to rise and appeared stiff in the hind limbs when ambulatory, but no joint swellings were noted. Electrocardiography revealed a heart rate of 120 beats/min, sinus arrhythmia with occasional premature atrial and ventricular contractions, and a normal mean electrical axis (60 degrees; normal range, 40 to 100). Echocardiography revealed moderate eccentric left-ventricular dilation (left-ventricular end diastolic diameter, 4.7 cm), severe left atrial enlargement (left atrium, 4.5 cm; left atrium/aorta, 2.0 cm), and severe mitral regurgitation (velocity decreased at 4.2 m/s). A large, hyperechoic mass lesion was noted adherent to the anterior mitral valve leaflet that prolapsed into the left atrium during systole. The anatomy of all other cardiac valves appeared normal, and no other valvular insufficiencies were noted. Based on the echocardiographic findings, a presumptive diagnosis of vegetative endocarditis of the mitral valve was made. Further possible diagnostics discussed with the owner included spinal radiographs, abdominal ultrasound, urine and blood cultures, various serological tests, and joint taps. Only serology for the presence of Bartonella sp. antibodies and a blood culture to attempt Bartonella isolation were performed at that time. However, because the dog had a history of tick and flea exposure, we later performed various serological tests. Therapy initiated at that time included amoxicillin-clavulanic acid (16.7 mg/kg p.o. BID), enrofloxacin (4.5 mg/kg p.o. BID), and an increase in the dosage of furosemide (3.3 mg/kg p.o. BID).

After 3 days, urine cultures were negative. Serial blood cultures obtained 30 min apart by a sterile technique from three different sites were negative for bacterial pathogens after 1 week. However, the dog was reported to have a high titer of antibodies to various Bartonella species, and the Bartonella-specific blood culture yielded a positive culture after 1 week (see below). At this time, therapy with amoxicillin-clavulanic acid was discontinued, and therapy with doxycycline (10 mg/kg p.o. BID) was initiated.

One month after initial presentation to the referred cardiologist, the patient was presented to another emergency animal hospital for treatment of progressive lethargy, anorexia, and dyspnea. Thoracic radiographs at that time revealed a severe perihilar pulmonary interstitial-to-alveolar pattern and persistent cardiomegaly (left-atrial enlargement). Emergency therapy for congestive heart failure, including intravenous diuresis, oxygen supplementation, and a topical venodilator, were unsuccessful, and the patient experienced cardiopulmonary arrest. Cardiopulmonary resuscitation was not attempted. Unfortunately, necropsy evaluation of the patient was not permitted.

Bartonella species are emerging pathogens in humans, causing severe diseases in immunocompromised individuals (10). At least eight Bartonella species or subspecies are known to be pathogenic for humans, including B. bacilliformis, B. quintana, B. henselae, B. elizabethae, B. grahamii, B. vinsonii subsp. arupensis (1, 18, 27, 47), B. vinsonii subsp. berkhoffii (44), and B. washoensis (10, 32). Furthermore, based on serological evidence, B. clarridgeiae has been associated with cat scratch disease in humans (29, 35, 45). Among these Bartonella species or subspecies, mainly B. quintana and B. henselae (1, 7, 10, 19, 41, 42, 46) but also B. elizabethae and B. vinsonii subsp. berkhoffii have been identified as causative agents of human endocarditis (18, 44), and B. washoensis has been identified as a cause of myocarditis (10, 32). The main reservoir species for B. washoensis appears to be ground squirrels (Spermophilus beecheyi) in Nevada (32) and California (B. B. Chomel, C. C. Chang, A. C. Ziedins, R. W. Kasten, and C. M. Hew, Abstr. 55th Int. Northwest. Conf. Dis. Nat. Commun. Man, 30 July to 2 August, 2000).

The number of Bartonella species or subspecies causing clinical diseases in dogs has been increasing in recent years. B. vinsonii subsp. berkhoffii has been shown to cause endocarditis, arrhythmia, and myocarditis (8, 11, 30), as well as granulomatous lymphadenitis and granulomatous rhinitis (39). B. clarridgeiae was isolated from the blood of a dog suffering from aortic endocarditis (17). B. clarridgeiae DNA was also detected by PCR in a dog with lymphocytic hepatitis (22). B. henselae DNA was initially detected in a dog with peliosis hepatis (28) and more recently in a dog with hepatopathy (22) and in three dogs with various clinical entities (37). These three B. henselae-PCR-positive dogs presented nonspecific clinical abnormalities, such as severe weight loss, protracted lethargy, and anorexia. A fourth dog was diagnosed as being infected with B. elizabethae by PCR amplification and sequencing, increasing the number of Bartonella species identified in infected dogs (37). We report the first isolation of another Bartonella species, B. washoensis, from the blood of a dog suffering from mitral valve vegetative endocarditis.

Strain sources.

The type strains of B. vinsonii subsp. berkhoffii (ATCC 51672) and B. clarridgeiae (ATCC 51734) were obtained from the American Type Culture Collection (Manassas, Va.). Isolate B. henselae strain U4 was obtained from our culture collection at the University of California, Davis. Isolate UCD-dog2 was cultured from the blood of the dog described in this report.

Clinical samples.

Blood (6 ml) was collected aseptically from the dog's external jugular vein at the time of clinical examination by A. C. Wey. Blood samples were subjected to aerobic and aerobic-anaerobic cultures. A blood sample, collected in a plastic EDTA tube (Becton Dickinson, Franklin Lakes, N.J.), was also submitted for specific Bartonella isolation, and the blood was plated on fresh blood agar (5% defibrinated rabbit blood) (15). Serum was submitted for Bartonella antibody titers and was later tested for several tick-borne pathogens (Ehrlichia canis, Anaplasma phagocytophilum, and Rickettsia rickettsii), including Coxiella burnetii, a known agent of endocarditis in humans and animals.

Isolation procedure.

A blood sample was collected in a plastic 2-ml EDTA tube and frozen at −70°C until plated. The blood sample was cultured on heart infusion agar containing 5% rabbit blood and incubated in 5% CO2 at 35°C for up to 4 weeks. Identification of the isolates as Bartonella spp. was initially based on morphological and growth characteristics, as previously described (17, 24). The isolates were then confirmed by PCR and restriction fragment length polymorphism (RFLP) analysis and sequence analysis of the citrate synthase (gltA), groEL, and 16S rRNA genes, as previously described (23, 36, 38).

Microscopic and biochemical analysis.

DNA extraction. A loopful (10 μl) of the bacterial isolate grown from the dog's blood was heated at 95°C for 10 min in 100 μl of sterile water. The supernatant was used as a DNA template, as previously described (12, 17).

PCR assay.

Five microliters of extracted DNA from the bacterial isolate was added to a 45-μl reaction mixture consisting of 15 mM Tris-HCl (pH 8.0), 50 mM KCl, 1.5 mM MgCl2, a 200 μM concentration of each deoxynucleoside triphosphate, 1.25 U of AmpliTaq Gold DNA polymerase (Perkin Elmer, Foster City, Calif.), and a 0.25 μM concentration of each primer. The primers used for the gltA gene were 5′-GGGGACCAGCTCATGGTGG-3′ and 5′-AATGCAAAAAGAACAGTAAACA-3′ (38). Thermocycling was performed in an MJ Research PTC-100 (Watertown, Mass.) apparatus under the following conditions: 94°C for 10 min and 45 cycles of 94°C for 0.5 min, 57°C for 1 min, and 72°C for 2 min, followed by 72°C for 5 min. For the 16S rRNA gene, the primers were 5′-AGAGTTTGATCCTGGCTCAG-3′ and 5′-AAGGAGGTGATCCAGCCGCA-3′ (23), and the running cycles were as follows: 95°C for 10 min and 35 cycles of 93°C for 0.5 min, 60°C for 1 min, and 72°C for 1 min, followed by 72°C for 8 min. For the groEL gene, the primers were 5′-CGTGAAGTTGCCTCAAAAACC-3′ and 5′-AATCCATTCCGCCCATTC-3′ (36), and the running cycles were as follows: 95°C for 10 min and 40 cycles of 95°C for 1 min, 56°C for 1 min, and 72°C for 1 min, followed by 72°C for 5 min.

RFLP analysis.

An approximately 400-bp fragment amplified from the gltA gene was verified by gel electrophoresis and then digested with the TaqI (Promega, Madison, Wis.), HhaI, AciI, and MseI (New England Laboratories, Beverly, Mass.) restriction endonucleases (5, 43). The digestion conditions used were the ones recommended by the enzymes' manufacturers. Banding patterns of the digests were compared to those of digests from B. vinsonii subsp. berkhoffii (ATCC 51672), B. henselae (strain U-4; University of California, Davis), and B. clarridgeiae (ATCC 51734).

DNA sequencing.

The PCR products from the gltA, 16S rRNA, and groEL genes used for DNA sequencing were purified with Microcon centrifugal filter devices (Millipore Corp., Bedford, Mass.) and sequenced with a fluorescence-based automated sequencing system (Davis Sequencing, Davis, Calif.), as previously described (14, 36). The FastA program of SeqWeb version 2 (Wisconsin Package; Accelrys Inc., San Diego, Calif.) was applied first to search the GenBank and EMBL databases for the closest bacterial species or subspecies. Then, the GAP and Evolution programs were used for sequence alignments and determination of the percentage of DNA similarity.

IFA tests. (i) Bartonella spp.

B. henselae, B. clarridgeiae, B. vinsonii subsp. berkhoffii, and B. washoensis indirect immunofluorescent-antibody (IFA) tests were performed as previously described (14-16). The intensity of bacillus-specific fluorescence was scored subjectively from 1 to 4, and a fluorescence score of ≥2 at a dilution of 1:64 was reported as a positive result, as previously described (14-16). Except for B. washoensis, the same two readers performed a double-blind reading of each slide. Positive serum control samples were obtained from dogs that had been confirmed to be infected with Bartonella. Specific IFA serology for B. washoensis was performed at the Division of Vector-Borne Infectious Diseases, Centers for Disease Control and Prevention, Fort Collins, Colo.

(ii) E. canis, A. phagocytophilum, R. rickettsii, and C. burnetii.

An IFA test was used to detect antibodies to E. canis (North Carolina State University canine strain), A. phagocytophilum (New York strain, human origin), and R. rickettsii (Domino canine strain) on 30-well Teflon-coated slides (9, 40). Serial twofold dilutions of the dog's serum were reacted with fluorescein isothiocyanate anti-canine immunoglobulin G conjugate (Cappel; ICN Pharmaceuticals, Inc., Costa Mesa, Calif.). Endpoint titers were determined as the last dilution at which brightly stained organisms could be detected on a fluorescence microscope with exciter and barrier filters. Antibodies against phase I and phase II of C. burnetii infection were evaluated with a commercially available IFA substrate slide (Fuller Laboratories, Fullerton, Calif.) at a 1:64 dilution (17).

Isolation and identification of B. washoensis.

Standard blood cultures for aerobic and anaerobic bacteria failed to grow bacteria. However, blood collected from the dog at the same time and cultured from the frozen and thawed EDTA tube grew a nonhemolytic gram-negative organism after 7 days, with only a few (60 CFU per ml) small (0.5- to 1-mm) white colonies. These colony growth characteristics and morphologies were suggestive of Bartonella spp., based on size, color, and time for colonies to appear. Microscopic examination demonstrated small gram-negative rods. PCR amplification with gltA primers produced a 400-bp fragment strongly suggestive of Bartonella. Digestion with TaqI, HhaI, AciI, and MseI endonucleases produced a unique RFLP profile.

A search (FastA) of the GenBank and EMBL databases with the gltA fragment (352 bp) resulted in the closest matches to B. washoensis (accession no. AF050108) and Bartonella sp. strain Sb944nv (AF470616) isolated from a California ground squirrel, with z scores of 1,334.8 and 1,330.9, respectively, where z is an indication of relatedness. A direct comparison of the dog isolate to B. washoensis (AF050108) with the GAP program yielded a 100% identity. Comparison of this sequence with other Bartonella gltA sequences (Evolution/Grow Tree program) resulted in a cluster containing the dog's isolate, B. washoensis, and the California ground squirrel Bartonella sp. strain Sb944nv (AF470616) isolate with identical sequences. Numerous other strains isolated from Nevada rodents (ground squirrels, least chipmunks, and bushytail woodrats) were also closely related to the dog isolate, with a divergence of 1.94 to 3.59 base substitutions per 100 bases (Table (Table1).1). A group of isolates cultured from deer mice (Peromyscus maniculatus) appear to be more divergent, with values of 7.01 to 7.68 base substitutions per 100 bases. Divergences of other standard Bartonella strains were 6.98 (B. vinsonii subsp. arupensis) to greater than or equal to 7.68 (B. henselae) base substitutions per 100 bases. Similarly, a fragment of the groEL gene (306 bp) of the dog isolate was compared to Bartonella strains listed in the GenBank and EMBL databases. The dog isolate was identical to B. washoensis and Bartonella sp. strain Sb944nv (AF484066) from a ground squirrel and similar to Bartonella sp. strain Sb1963nv (AF484067) from another California ground squirrel, with a base substitution rate of 0.33 per 100 bases compared to at least 6.82 per 100 bases for other Bartonella strains (Table (Table2).2). Finally, when a fragment of the 16S rRNA gene (511 bp) was compared, the dog isolate was 100% identical to B. washoensis (AF070463). A slightly longer fragment (577 bp) indicated a minor divergence, with 0.17 base substitutions per 100 bases, although the 16S rRNA gene comparison indicated a variance of less than 3 base substitutions per 100 bases for the group analyzed.

TABLE 1.
Estimated number of nucleotide substitutions per 100 bases for a 315-base segment of the gltA gene
TABLE 2.
Estimated number of nucleotide substitutions per 100 bases for a 306-base segment of the groEL gene

Serological analysis.

Serum antibodies to B. clarridgeiae, B. vinsonii subsp. berkhoffii, and B. henselae were detected in the dog by IFA assay at the reciprocal titer of 4,096. Because of the dog's history of being exposed to fleas and ticks, the dog serum was later tested for potential tick-borne pathogens. The dog was seronegative for A. phagocytophilum, E. canis, and R. rickettsii but was weakly positive for the C. burnetii phase II antigen. After identification of the isolate as B. washoensis, the dog serum was tested against this specific antigen and revealed a reciprocal titer of 8,192.

Conclusions.

We report the first isolation of B. washoensis from a dog and the second isolation of this species outside of its natural rodent reservoir. It is also the first known case of endocarditis associated with B. washoensis, as it caused fever and myocarditis in the human patient (32). In this dog, several factors are suggestive that B. washoensis was the etiological agent, including (i) isolation of the organism from the blood, (ii) failure to isolate other bacteria by conventional blood culture, and (iii) the presence of high titers of antibody against various Bartonella species, including B. washoensis, as previously reported for cases of Bartonella endocarditis in humans (21, 42) and dogs (K. A. MacDonald, B. B. Chomel, M. D. Kittleson, R. W. Kasten, W. P. Thomas, and P. A. Pesavento. Abstr. Am. Coll. Vet. Intern. Med., 21st Annu. Forum, J. Vet. Intern. Med. 17:399, 2003). Unfortunately, tissues were not available for microscopic examination or PCR testing of the damaged valve.

The valvular lesion was located on the mitral valve, as previously reported for other Bartonella endocarditis cases in dogs (8). However, most Bartonella endocarditis cases in dogs usually involve the aortic valve or both cardiac valves (8, 11; MacDonald et al., Abstr. Am. Coll. Vet. Intern. Med.). Similarly, in a series of 33 human patients with Bartonella endocarditis, 29 (88%) had involvement of the aortic valve, including 2 with concurrent aortic and mitral valvular involvement, compared to only 4 patients with only involvement of the mitral valve (41). In a more recent study of 61 confirmed cases of Bartonella endocarditis, involvement of only the aortic valve (36 cases) was four times more frequent than involvement of only the mitral valve (9 cases) (42).

Genetic analysis of the dog isolate indicates that the organism isolated is B. washoensis, as the sequence analysis of fragments from three different genes revealed genetic identity with B. washoensis isolated from a human patient with myocarditis and a California ground squirrel (32). Furthermore, the dog isolate was clustered with several other rodent isolates cultured from animals captured in the vicinity of the human patient. We also found a complete match between the human and dog isolates for the groEL gene partial sequence and a minor mismatch with isolate Sb1963nv, as reported by Kosoy et al. (32).

Analysis of the gltA gene has historically been used to compare Bartonella strains since it provides a good discriminatory power at the species level (5, 38). While analysis of the 16S rRNA gene provides usable information at the genus level, the high degree of similarity among Bartonella strains disallows strong discriminatory power for many of the new species of Bartonella (5, 26). Sequences from other genes, such as groEL, are beginning to be published and provide an opportunity to compare more fragments from each isolate.

The dog's source of infection and the mode of transmission of B. washoensis will most likely remain unexplained. We know that the dog had a history of tick and flea exposure. However, this dog was seronegative for associated bacteria, in contrast to dogs infected with B. vinsonii subsp. berkhoffii, for which a strong association has been reported between seropositivity to Bartonella and seropositivity to several tick-borne pathogens, especially Ehrlichia, Anaplasma, and Babesia spp. (9, 31, 40). Furthermore, the weak positive reaction to the C. burnetii phase II antigen is more likely to result from serological cross-reactivity, as was previously demonstrated for humans (34). B. washoensis has been reported to have a rodent reservoir (10, 32). In California and Nevada, a high percentage of California ground squirrels are infected with this species and represent its main reservoir (32; B. B. Chomel et al. Abstr. 55th Int. Northwest. Conf. Dis. Nat. Commun. Man).

However, the arthropod vector of B. washoensis has not yet been identified. The ground squirrels from northern California, among which B. washoensis bacteremic animals were identified, were heavily infested with fleas (Chomel et al., unpublished observations). As indicated by Kosoy et al. (32), S. beecheyi are commonly and heavily infested with Oropsylla montana, a flea species that readily feeds on humans and generally is considered to be the most important vector of human plague in the United States. These fleas might play a main role as the vector of infection between rodents and also might be involved in the transmission of B. washoensis to dogs and humans. However, the potential role of ticks still cannot be excluded, as several questing adult Ixodes pacificus ticks have also been reported to harbor B. washoensis DNA (13).

Rodents constitute a wide reservoir of Bartonella species in many parts of the world (2, 3, 4, 6, 10, 20, 24, 25, 33, 48). In North America, several Bartonella species or subspecies have been identified, including B. vinsonii, B. vinsonii subsp. arupensis, B. elizabethae, B. peromysci, and B. washoensis (6, 10, 20, 25, 33, 47), and many more are still waiting to be fully described (4, 20, 33, 48). Among these rodent-borne Bartonella spp., four species (B. elizabethae, B. vinsonii subsp. arupensis, B. grahamii, and B. washoensis) have now been related to human infections, causing mainly cardiopathy, endocarditis, or neuroretinitis (10, 32). Furthermore, B. elizabethae DNA was recently identified in a sick dog with a 2-month history of lethargy, decreased appetite, weight loss, and occasional vomiting of undigested food (37). With the present report, it is the second rodent-borne Bartonella species to be found in sick dogs, suggesting that many other Bartonella species may cause severe infections in domestic dogs.

Acknowledgments

This project was supported in part by a grant from the Morris Animal Foundation and a grant from the Center for Companion Animal Health, School of Veterinary Medicine, University of California, Davis.

We thank Barbara Hegarty and Edward Breitschwerdt, College of Veterinary Medicine, North Carolina State University, for testing the dog serum for the various tick-borne pathogens and Michael Kosoy, Division of Vector-Borne Infectious Diseases, Centers for Disease Control and Prevention, for providing assistance for the B. washoensis IFA testing.

REFERENCES

1. Anderson, B. E., and M. A. Neuman. 1997. Bartonella spp. as emerging human pathogens. Clin. Microbiol. Rev. 10:203-219. [PMC free article] [PubMed]
2. Bermond, D., R. Heller, F. Barrat, G. Delacour, C. Dehio, A. Alliot, H. Monteil, B. Chomel, H. J. Boulouis, and Y. Piemont. 2000. Bartonella birtlesii sp. nov., isolated from small mammals (Apodemus spp.). Int. J. Syst. E vol. Microbiol. 50:1973-1979. [PubMed]
3. Birtles, R. J., T. G. Harrison, and D. H. Molyneux. 1994. Grahamella in small woodland mammals in the U.K.: isolation, prevalence, and host specificity. Ann. Trop. Med. Parasitol. 88:317-327. [PubMed]
4. Birtles, R. J., S. M. Hazel, M. Bennett, K. Bown, D. Raoult, and M. Begon. 2001. Longitudinal monitoring of the dynamics of infections due to Bartonella species in UK woodland rodents. Epidemiol. Infect. 126:323-329. [PubMed]
5. Birtles, R. J., and D. Raoult. 1996. Comparison of partial citrate synthase gene (gltA) sequences for phylogenetic analysis of Bartonella species. Int. J. Syst. Bacteriol. 46:891-897. [PubMed]
6. Bown, K. J., B. A. Ellis, R. J. Birtles, L. A. Durden, J. Lello, M. Begon, and M. Bennett. 2002. New World origins for haemoparasites infecting United Kingdom grey squirrels (Sciurus carolinensis), as revealed by phylogenetic analysis of Bartonella infecting squirrel populations in England and the United States. Epidemiol. Infect. 129:647-653. [PubMed]
7. Breathnach, A. S., J. M. Hoare, and S. J. Eykyn. 1997. Culture-negative endocarditis: contribution of Bartonella infections. Heart 77:474-476. [PMC free article] [PubMed]
8. Breitschwerdt, E. B., C. E. Atkins, T. T. Brown, D. L. Kordick, and P. S. Snyder. 1999. Bartonella vinsonii subsp. berkhoffii and related members of the alpha subdivision of the Proteobacteria in dogs with cardiac arrhythmias, endocarditis, or myocarditis. J. Clin. Microbiol. 37:3618-3626. [PMC free article] [PubMed]
9. Breitschwerdt, E. B., B. C. Hegarty, and S. I. Hancock. 1998. Sequential evaluation of dogs naturally infected with Ehrlichia canis, Ehrlichia chaffeensis, Ehrlichia equi, Ehrlichia ewingii, or Bartonella vinsonii. J. Clin. Microbiol. 36:2645-2651. [PMC free article] [PubMed]
10. Breitschwerdt, E. B., and D. L. Kordick. 2000. Bartonella infection in animals: carriership, reservoir potential, pathogenicity, and zoonotic potential for human infection. Clin. Microbiol. Rev. 13:428-438. [PMC free article] [PubMed]
11. Breitschwerdt, E. B., D. L. Kordick, D. E. Malarkey, B. Keene, T. L. Hadfield, and K. Wilson. 1995. Endocarditis in a dog due to infection with a novel Bartonella subspecies. J. Clin. Microbiol. 33:154-160. [PMC free article] [PubMed]
12. Chang, C. C., B. B. Chomel, R. W. Kasten, R. Heller, K. M. Kocan, H. Ueno, K. Yamamoto, C. Elmi, V. C. Bleich, B. M. Pierce, B. J. Gonzales, P. K. Swift, W. M. Boyce, S. S. Jang, H. Boulouis, and Y. Piemont. 2000. Isolation of Bartonella spp. from wild cervids, bovids, and domestic cattle in North America. Emerg. Infect. Dis. 6:306-311. [PMC free article] [PubMed]
13. Chang, C. C., B. B. Chomel, R. W. Kasten, V. Romano, and N. Tietze. 2001. Molecular evidence of Bartonella spp. in questing adult Ixodes pacificus ticks in California. J. Clin. Microbiol. 39:1221-1226. [PMC free article] [PubMed]
14. Chang, C.-C., R. W. Kasten, B. B. Chomel, D. C. Simpson, C. M. Hew, D. L. Kordick, R. Heller, Y. Piemont, and E. B. Breitschwerdt. 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. [PMC free article] [PubMed]
15. Chomel, B. B., R. C. Abbott, R. W. Kasten, K. A. Floyd-Hawkins, P. H. Kass, C. A. Glaser, N. C. Pedersen, and J. E. Koehler. 1995. Bartonella henselae prevalence in domestic cats in California: risk factors and association between bacteremia and antibody titers. J. Clin. Microbiol. 33:2445-2450. [PMC free article] [PubMed]
16. Chomel, B. B., E. T. Carlos, R. W. Kasten, K. Yamamoto, C. C. Chang, R. S. Carlos, M. V. Abenes, and C. M. Pajares. 1999. Bartonella henselae and Bartonella clarridgeiae infection in domestic cats from The Philippines. Am. J. Trop. Med. Hyg. 60:593-597. [PubMed]
17. Chomel, B. B., K. A. MacDonald, R. W. Kasten, C.-C. Chang, A. C. Wey, J. E. Foley, W. P. Thomas, and M. D. Kittleson. 2001. Aortic valve endocarditis in a dog due to Bartonella clarridgeiae. J. Clin. Microbiol. 39:3548-3554. [PMC free article] [PubMed]
18. Daly, J. S., M. G. Worthington, D. J. Brenner, C. W. Moss, D. G. Hollis, R. S. Weyant, A. G. Steigerwalt, R. E. Weaver, M. I. Daneshvar, and S. P. O'Connor. 1993. Rochalimaea elizabethae sp. nov. isolated from a patient with endocarditis. J. Clin. Microbiol. 31: 872-881. [PMC free article] [PubMed]
19. Drancourt, M., J. L. Mainardi, P. Brouqui, F. Vandenesch, A. Carta, F. Lehnert, J. Etienne, F. Goldstein, J. Acar, and D. Raoult. 1995. Bartonella (Rochalimaea) quintana endocarditis in three homeless men. N. Engl. J. Med. 332:419-423. [PubMed]
20. Ellis, B. A., R. L. Regnery, L. Beati, F. Bacellar, M. Rood, G. G. Glass, E. Marston, T. G. Ksiazek, D. Jones, and J. E. Childs. 1999. Rats of the genus Rattus are reservoir hosts for pathogenic Bartonella species: an Old World origin for a New World disease? J. Infect. Dis. 180: 220-224. [PubMed]
21. Fournier, P.-E., J.-L. Mainardi, and D. Raoult. 2002. Value of microimmunofluorescence for diagnosis and follow-up of Bartonella endocarditis. Clin. Diagn. Lab. Immunol. 9:795-801. [PMC free article] [PubMed]
22. Gillespie, T. N., R. J. Washabau, M. H. Goldschmidt, J. M. Cullen, A. R. Rogala, and E. B. Breitschwerdt. 2003. Detection of Bartonella henselae and Bartonella clarridgeiae DNA in hepatic specimens from two dogs with hepatic disease. J. Am. Vet. Med. Assoc. 222:35, 47-51. [PubMed]
23. Gurfield, A. N., H.-J. Boulouis, B. B. Chomel, R. Heller, R. W. Kasten, K. Yamamoto, and Y. Piemont. 1997. Coinfection with Bartonella clarridgeiae and Bartonella henselae and with different Bartonella henselae strains in domestic cats. J. Clin. Microbiol. 35: 2120-2123. [PMC free article] [PubMed]
24. Heller, R., P. Riegel, Y. Hansmann, G. Delacour, D. Bermond, C. Dehio, F. Lamarque, H. Monteil, B. Chomel, and Y. Piemont. 1998. Bartonella tribocorum sp. nov., a new Bartonella species isolated from the blood of wild rats. Int. J. Syst. Bacteriol. 48:1333-1339. [PubMed]
25. Hofmeister, E. K., C. P. Kolbert, A. S. Abdulkarim, J. M. Magera, M. K. Hopkins, J. R. Uhl, A. Ambyaye, S. R. Telford III, F. R. Cockerill III, and D. H. Persing. 1998. Cosegregation of a novel Bartonella species with Borrelia burgdorferi and Babesia microti in Peromyscus leucopus. J. Infect. Dis. 177: 409-416. [PubMed]
26. Houpikian, P., and D. Raoult. 2001. 16S/23S rRNA intergenic spacer regions for phylogenetic analysis, identification, and subtyping of Bartonella species. J. Clin. Microbiol. 39:2768-2778. [PMC free article] [PubMed]
27. Kerkhoff, F. T., A. M. C. Bergmans, A. Van Der Zee, and A. Rothova. 1999. Demonstration of Bartonella grahamii DNA in ocular fluids of a patient with neuroretinitis. J. Clin. Microbiol. 37:4034-4038. [PMC free article] [PubMed]
28. Kitchell, B. E., T. M. Fan, D. L. Kordick, E. B. Breitschwerdt, G. Wollenberg, and C. A. Lichtensteiger. 2000. Peliosis hepatis in a dog infected with Bartonella henselae. J. Am. Vet. Med. Assoc. 216:519-523. [PubMed]
29. Kordick, D. L., E. J. Hilyard, T. L. Hadfield, K. H. Wilson, A. G. Steigerwalt, D. J. Brenner, and E. B. Breitschwerdt. 1997. Bartonella clarridgeiae, a newly recognized zoonotic pathogen causing inoculation papules, fever, and lymphadenopathy (cat scratch disease). J. Clin. Microbiol. 35:1813-1818. [PMC free article] [PubMed]
30. Kordick, D. L., B. Swaminathan, C. E. Greene, K. H. Wilson, A. M. Whitney, S. O'Connor, D. G. Hollis, G. M. Matar, A. G. Steigerwalt, G. B. Malcolm, P. S. Hayes, T. L. Hadfield, E. B. Breitschwerdt, and D. J. Brenner. 1996. Bartonella vinsonii subsp. berkhoffii subsp. nov., isolated from dogs; Bartonella vinsonii subsp. vinsonii; and emended description of Bartonella vinsonii. Int. J. Syst. Bacteriol. 46:704-709. [PubMed]
31. Kordick, S. K., E. B. Breitschwerdt, B. C. Hegarty, K. L. Southwick, C. M. Colitz, S. I. Hancock, J. M. Bradley, R. Rumbough, J. T. McPherson, and J. N. MacCormack. 1999. Coinfection with multiple tick-borne pathogens in a Walker Hound kennel in North Carolina. J. Clin. Microbiol. 37:2631-2638. [PMC free article] [PubMed]
32. Kosoy, M., M. Murray, R. D. Gilmore, Jr., Y. Bai, and K. L. Gage. 2003. Bartonella strains from ground squirrels are identical to Bartonella washoensis isolated from a human patient. J. Clin. Microbiol. 41:645-650. [PMC free article] [PubMed]
33. Kosoy, M. Y., R. L. Regnery, T. Tzianabos, E. L. Marston, D. C. Jones, D. Green, G. O. Maupin, J. G. Olson, and J. E. Childs. 1997. Distribution, diversity, and host specificity of Bartonella in rodents from the southeastern United States. Am. J. Trop. Med. Hyg. 57:578-588. [PubMed]
34. La Scola, B., and D. Raoult. 1996. Serological cross-reactions between Bartonella quintana, Bartonella henselae, and Coxiella burnetii. J. Clin. Microbiol. 34:2270-2274. [PMC free article] [PubMed]
35. Margileth, A. M., and D. F. Baehren. 1998. Chest-wall abscess due to cat-scratch disease (CSD) in an adult with antibodies to Bartonella clarridgeiae: case report and review of the thoracopulmonary manifestations of CSD. Clin. Infect. Dis. 27: 353-357. [PubMed]
36. Marston, E. L., J. W. Sumner, and R. L. Regnery. 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. [PubMed]
37. Mexas, A. M., S. I. Hancock, and E. B. Breitschwerdt. 2002. Bartonella henselae and Bartonella elizabethae as potential canine pathogens. J. Clin. Microbiol. 40:4670-4674. [PMC free article] [PubMed]
38. Norman, A. F., R. Regnery, P. Jameson, C. Greene, and D. C. Krause. 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. [PMC free article] [PubMed]
39. Pappalardo, B. L., T. Brown, J. L. Gookin, C. L. Morrill, and E. B. Breitschwerdt. 2000. Granulomatous disease associated with Bartonella infection in 2 dogs. J. Vet. Intern. Med. 14:37-42. [PubMed]
40. Pappalardo, B. L., M. T. Correa, C. C. York, C. Y. Peat, and E. B. Breitschwerdt. 1997. Epidemiologic evaluation of the risk factors associated with exposure and seroreactivity to Bartonella vinsonii in dogs. Am. J. Vet. Res. 58:467-471. [PubMed]
41. Raoult, D., P. E. Fournier, M. Drancourt, T. J. Marrie, J. Etienne, J. Cosserat, P. Cacoub, Y. Poinsignon, P. Leclercq, and A. M. Sefton. 1996. Diagnosis of 22 new cases of Bartonella endocarditis. Ann. Intern. Med. 125:646-652. (Erratum, 127:249, 1997.) [PubMed]
42. Raoult, D., P. E. Fournier, F. Vandenesch, J. L. Mainardi, S. J. Eykyn, J. Nash, E. James, C. Benoit-Lemercier, and T. J. Marrie. 2003. Outcome and treatment of bartonella endocarditis. Arch. Intern. Med. 163:226-230. [PubMed]
43. Regnery, R. L., B. E. Anderson, J. E. Clarridge III, M. C. Rodriguez-Barradas, D. C. Jones, and J. H. Carr. 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. [PMC free article] [PubMed]
44. Roux, V., S. J. Eykyn, S. Wyllie, and D. Raoult. 2000. Bartonella vinsonii subsp. berkhoffii as an agent of afebrile blood culture-negative endocarditis in a human. J. Clin. Microbiol. 38:1698-1700. [PMC free article] [PubMed]
45. Sander, A., A. Zagrosek, W. Bredt, E. Schiltz, Y. Piémont, C. Lanz, and C. Dehio. 2000. Characterization of Bartonella clarridgeiae flagellin (FlaA) and detection of antiflagellin antibodies in patients with lymphadenopathy. J. Clin. Microbiol. 38:2943-2948. [PMC free article] [PubMed]
46. Spach, D. H., K. P. Callis, D. S. Paauw, Y. B. Houze, F. D. Schoenknecht, D. F. Welch, H. Rosen, and D. J. Brenner. 1993. Endocarditis caused by Rochalimaea quintana in a patient infected with human immunodeficiency virus. J. Clin. Microbiol. 31:692-694. [PMC free article] [PubMed]
47. Welch, D. F., K. C. Carroll, E. K. Hofmeister, D. H. Persing, D. A. Robison, A. G. Steigerwalt, and D. J. Brenner. 1999. Isolation of a new subspecies, Bartonella vinsonii subsp. arupensis, from a cattle rancher: identity with isolates found in conjunction with Borrelia burgdorferi and Babesia microti among naturally infected mice. J. Clin. Microbiol. 37:2598-2601. [PMC free article] [PubMed]
48. Ying, B., M. Y. Kosoy, G. O. Maupin, K. R. Tsuchiya, and K. L. Gage. 2002. Genetic and ecologic characteristics of Bartonella communities in rodents in southern China. Am. J. Trop. Med. Hyg. 66:622-627. [PubMed]

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