Search tips
Search criteria 


Logo of aacPermissionsJournals.ASM.orgJournalAAC ArticleJournal InfoAuthorsReviewers
Antimicrob Agents Chemother. 2004 June; 48(6): 1921–1933.
PMCID: PMC415619

Recommendations for Treatment of Human Infections Caused by Bartonella Species

Members of the genus Bartonella are facultative intracellular bacteria belonging to the alpha 2 subgroup of the class Proteobacteria and are phylogenetically closely related to Brucella species (15, 73). Until 1993, only three diseases were known to be caused by Bartonella species: Carrion's disease (Bartonella bacilliformis), trench fever (Bartonella quintana), and cat scratch disease (CSD; Bartonella henselae). The genus now comprises B. bacilliformis, species of the former genera Rochalimea and Grahamella (14, 18), and additional, recently described species (Table (Table1).1). In mammals, each Bartonella species is highly adapted to its reservoir host; the bacteria can persist in the bloodstream of the host as the result of intraerythrocytic parasitism (49). Intraerythrocytic localization of B. henselae has been demonstrated in cat erythrocytes (88), and B. bacilliformis bacilli have been observed within erythrocytes during the acute phase of Carrion's disease (Oroya fever) (88). Bartonellae also have a tropism for endothelial cells, and intracellular B. henselae can be identified in endothelial cells infected in vitro (28), although intraendothelial cell bacilli have not been identified in vivo.

Epidemiological and clinical data for species of the genus Bartonella

Bartonella species cause long-recognized diseases, such as Carrion's disease, trench fever, and CSD, and more recently recognized diseases, such as bacillary angiomatosis (BA), peliosis hepatis (PH), chronic bacteremia, endocarditis, chronic lymphadenopathy, and neurological disorders (Table (Table2)2) (73). A remarkable feature of the genus Bartonella is the ability of a single species to cause either acute or chronic infection and either vascular proliferative or suppurative manifestations.

Human diseases caused by Bartonella spp.

The pathological response to infection with Bartonella spp. varies substantially with the status of the host immune system. Indeed, infection with the same Bartonella species (e.g., B. henselae) can result in a focal suppurative reaction (CSD in immunocompetent patients), a multifocal angioproliferative response (BA in immunocompromised patients), endovascular multiplication of the bacteria (endocarditis), or an exaggerated inflammatory response without evidence of bacteria in patient tissues (meningoencephalitis) (86).

Some of the diseases due to Bartonella species can resolve spontaneously without treatment, but in other cases, the disease is fatal without antibiotic treatment and/or surgery. The clinical situations are so different that a single treatment for all Bartonella-related diseases has not been identified, and the approach to treatment must be adapted to each species and clinical situation (49). Moreover, the database of clinical studies with a standard case definition, culture confirmation, rigidly defined disease outcomes, and patients with similar host defenses is very limited. Thus, case reports with a very limited number of subjects often serve to dictate therapy. The objective of this minireview is to summarize the antibiotic treatment recommendations for the different infections caused by Bartonella species. We have compiled the in vitro antibiotic susceptibility data and our knowledge of the in vivo efficacies of antibiotics for each clinical manifestation, and finally, we have summarized and ranked our treatment recommendations according to the Infectious Diseases Society of America (IDSA) practice guidelines (see Table Table5)5) (51).

System for ranking recommendations in clinical guidelines recommended by IDSAa


Culture of Bartonella spp.

Because Bartonella spp. are facultative intracellular organisms, isolation can be performed in either cell cultures or axenic media with blood-enriched agar plates (63) (Fig. (Fig.11 and and2).2). However, Bartonella bacteria are very fastidious, and primary isolation is difficult, with detection of colonies only after 1 to 4 weeks of incubation on blood agar plates (63). The growth of subcultured isolates on blood agar plates is more rapid, usually yielding colonies after 3 to 5 days. Cell coculture systems have been reported to be more sensitive and allow more rapid growth of bartonellae than blood agar plates (63). Since 1992, several studies have reported on the isolation of B. henselae from the blood and lymph nodes of patients with CSD, with confirmation by serology, PCR, or culture (9, 71). However, isolation of B. henselae from the lymph nodes of CSD patients is very rare compared to the more frequent detection of B. henselae DNA in these patients by PCR assays (63, 109). At present, there is no optimal procedure for the isolation of Bartonella species; rather, several techniques and agars (e.g., cocultivation with eukaryotic cells, in addition to plating onto rabbit blood and chocolate agars) should be combined in order to isolate strains.

FIG. 1.
Colonies of B. quintana on a blood agar plate.
FIG. 2.
B. quintana as viewed after Gimenez staining. Magnification, ×1,000.

In vitro susceptibilities of Bartonella species to antibiotics.

The results of susceptibility testing with Bartonella spp. are summarized in Table Table3.3. Evaluation of susceptibilities to antibiotics has been performed either in the presence of eukaryotic cells or without cells, i.e., in axenic media. Use of these different methods of culture for the determination of the bacteriostatic activities of antibiotics yielded similar results. Determination of antibiotic susceptibility in axenic media has been carried out either with solid media enriched with 5 to 10% sheep or horse blood or with liquid media (74, 97). It should be noted that the conditions required to grow Bartonella during susceptibility testing do not meet the standardized criteria established by NCCLS. Bacteria of the genus Bartonella are susceptible to many antibiotics when they are grown axenically, including penicillin and cephalosporin compounds, aminoglycosides, chloramphenicol, tetracyclines, macrolide compounds, rifampin, fluoroquinolones, and co-trimoxazole (74, 79). However, the in vitro and the in vivo antibiotic susceptibilities of Bartonella do not correlate well for a number of antibiotics; for instance, penicillin has no in vivo efficacy, despite the very low MICs observed in vitro.

MICs for Bartonella sp. strains determined by the agar dilution technique with Columbia agar supplemented with 5% horse blooda

In vitro antibiotic susceptibilities of Bartonella species cocultivated with eukaryotic cells have also been examined. As with agar-based susceptibilities, these studies demonstrated that Bartonella spp. are susceptible to many antibiotics in vitro (46). However, all of these antibiotics (48) had only bacteriostatic activity (47, 48). It was recently demonstrated in vitro that aminoglycosides alone are bactericidal against Bartonella species grown either in liquid medium (91) or in endothelial cells (78). With a recently established erythrocyte coculture model, it was found that most of the antibiotics tested (i.e., doxycycline, fluoroquinolone compounds, and beta-lactams) were not bactericidal against Bartonella (90). Gentamicin was bactericidal at 4 μg/ml, as was rifampin. At this concentration, gentamicin was shown to enter erythrocytes slowly and to reach a peak level of 0.26 μg/ml after 24 h. However, when the ability of gentamicin to kill extraerythrocytic B. quintana at the concentration of 0.26 μg/ml achieved in the erythrocyte was tested, it was found that gentamicin was not bactericidal, even after 96 h of incubation (90). We hypothesize that erythrocytes may be a reservoir for B. quintana and that the bactericidal activity of gentamicin that was observed occurs mainly when the bacteria emerge from the erythrocytes and are found extracellularly.


Feline animal models have been used to evaluate the efficacies of antimicrobial therapies for B. henselae infections. Regnery et al. (85) and Greene et al. (40) evaluated the efficacies of antibiotics during acute infection in cats inoculated with laboratory-cultivated B. henselae, whereas Kordick et al. (60) studied naturally infected cats with chronic infections. Regnery et al. (85) cultured the blood of the cats at intervals after experimental inoculation and determined that only tetracycline or erythromycin treatment significantly decreased the number of bacteria in the bloodstream. However, there were no significant differences among the four antibiotics with regard to the ultimate resolution of bacteremia (85).

In the study by Kordick et al. (60), various antibiotics, including doxycycline and amoxicillin, appeared to be effective in reducing the bacterial count in blood (40). However, subsequent bacteremia was observed after therapy was discontinued, suggesting that antibiotics did not eradicate the infection. Kordick et al. (60) reported that bacteremia in naturally, chronically infected cats was successfully cleared from only 9 of 14 cats treated with enrofloxacin and 2 of 8 cats treated with doxycycline. These reports are difficult to compare because the strain used as the inoculum for the experimental infection was grown on agar, and the virulence of these bacteria was probably different from that of B. henselae in the naturally infected cats. In addition, one trial treated acutely infected cats, while the other treated naturally, chronically infected cats. Acute experimental infections may be more susceptible to antibiotics than chronic infections in naturally infected cats; this may be similar to the situation in humans infected with B. quintana (35).


MICs correlate poorly with the in vivo efficacies of antibiotics in patients with Bartonella-related infections (74). The lack of a bactericidal effect of antibiotics against Bartonella spp. and the different niches that Bartonella occupies in the human host, e.g., sequestration in erythrocytes, may explain such discrepancies between in vitro and clinical data. For serious Bartonella infections, it is critical to use two antibiotics, each of which has good in vivo efficacy against Bartonella. This is particularly important if gentamicin is one of the drugs in the regimen, because the gentamicin protection assay with red blood cells infected in vivo, as well as the in vitro erythrocyte cell culture model, document that bartonellae residing within erythrocytes are protected from gentamicin (90, 93). Thus, with our current knowledge, addition of another antibiotic with good in vivo activity against Bartonella is crucial, because the two antibiotics may eradicate the bacteria in different niches in the host.

We present the relevant clinical studies for each clinical situation (Table (Table4)4) and recommendations for the treatment of human Bartonella infections (see Table Table6),6), with recommendations ranked according to IDSA practice guidelines (Table (Table5)5) (51).

Relevant clinical data on efficacy of antibiotic treatment of Bartonella-related infectionsa
Guidelines and recommendations for the treatment of infections caused by Bartonella speciesa


Identification of B. henselae as the etiologic agent of CSD occurred only after decades of searching for the cause. In 1988, English and collaborators (34) isolated and cultured a bacterium that was named Afipia felis in 1992. This agent was initially considered the etiologic agent of CSD; however, the results of further studies failed to support this conclusion. However, serological evidence linking CSD with a different bacterium, B. henselae, was reported in 1992 (73); and in 1993, Dolan and colleagues (30) isolated Rochalimaea henselae (now named B. henselae) from the lymph nodes of patients with CSD. Nearly simultaneously, this species was also identified as a cause of bacteremia, BA, and PH in immunocompromised patients (57) and bacteremia and endocarditis in both immunocompromised and immunocompetent patients (5).

Cats are the main reservoir of B. henselae, and the bacterium is transmitted to cats by the cat flea (Ctenocephalides felis) (23). Most patients with CSD give a history of contact with a cat and receiving a scratch and/or bite (71). CSD is manifested by gradual regional lymph node enlargement, usually accompanied by a distal scratch and/or red-brown skin papule. The enlarged lymph node is often painful and tender. The infection is usually self-limited, with the frequent development of extensive regional lymph node enlargement that typically lasts 2 to 3 months and occasionally longer. The lymph node may suppurate if it is not drained; if drainage is necessary, needle aspiration is preferred. Most patients with typical CSD remain afebrile and are not systemically ill throughout the course of the disease (9, 21, 71). Lymphadenopathy occurs most often in nodes that drain the area where cat scratches usually occur, mainly the axilla, the neck, and the groin (21, 71).

Systemic or severe disease can complicate CSD in 5 to 14% of cases (21, 71). Atypical presentations include prolonged fever (>2 weeks), malaise, fatigue, myalgia and arthralgia, weight loss, splenomegaly, and Parinaud's oculoglandular syndrome (9). Encephalopathy and neuroretinitis are less common complications of CSD (9).

CSD typically does not respond to antibiotic therapy. The clinical manifestations of the disease may be due to an immunological reaction in the lymph nodes, and there are probably few or no viable Bartonella bacilli by the time that a biopsy is performed. Indeed, although PCR assays with samples from lymph nodes are often positive at the time of acute disease, isolation of the bacteria from lymph nodes has been reported only rarely (30, 64, 109). Numerous reports have evaluated the effectiveness of many antimicrobial agents for the treatment of typical, uncomplicated CSD (9). Most investigators have observed no benefit with antibiotic treatment, whereas anecdotal reports have indicated that ciprofloxacin, rifampin, and co-trimoxazole may be effective. In a 1960 study reporting on the treatment of 83 cases of CSD, Spaulding and Hennessy (101) noted that they were impressed with the failure of any antibiotics to shorten the course of the illness. Margileth (70) retrospectively reviewed the effects of various antibiotics for the treatment of 268 patients with typical CSD. The mean duration of illness was 14.5 weeks for 66 patients without treatment and 14.5 weeks for 113 patients treated with antibiotics thought to be ineffective. In contrast, the mean duration of illness was 2.8 weeks for 89 patients treated with rifampin, ciprofloxacin, gentamicin, or co-trimoxazole.

The only prospective treatment trial, a double-blind, placebo-controlled study of azithromycin treatment of immunocompetent patients with uncomplicated CSD, was reported by Bass et al. (8). An 80% decrease in the initial lymph node volume was documented in 7 of 14 azithromycin-treated patients but in only 1 of 15 placebo-treated controls during the first 30 days of observation (P = 0.026) (8). There was no difference in any clinical outcome measurement except for the rate and degree of decrease of total lymph node volume as determined by sonographic documentation. At 30 days, patients treated with azithromycin had a significantly greater reduction in the total lymph node volume, as demonstrated by sonography, in comparison to the total lymph node volume of the placebo group (8). The investigators did not demonstrate any efficacy of azithromycin for the treatment of disseminated CSD, either for prevention of the evolution of localized CSD to disseminated disease or for prevention of complications such as encephalitis or endocarditis. Thus, a recommendation to treat immunocompetent CSD patients with azithromycin remains very premature at present.

For the reasons outlined above, it is not clear that antibiotic therapy is useful for the treatment of CSD in immunocompetent patients; and because antibiotic therapy adds the risk of adverse drug reactions and the generation of resistant flora, the current recommendation for the mild to moderately ill immunocompetent patient with CSD is no antibiotic treatment (Table (Table6,6, recommendation CIII). After evaluation of an adequate fine-needle aspirate has ruled out fungal or mycobacterial infection and malignancy, patients and parents should be reassured that the adenopathy is benign and that it will probably subside spontaneously within 2 to 4 months (72). Management consists of treatment with analgesics for pain and prudent follow-up. Treatment with an azithromycin regimen (500 mg orally [p.o.] on day 1 and 250 mg p.o. on days 2 to 5 as single daily doses) could be an alternative for patients with large, bulky lymphadenopathy (Table (Table6,6, recommendation BI) (8). The combination of doxycycline (100 mg p.o. or intravenously [i.v.] twice daily) with rifampin (300 mg p.o. twice daily) could also be an alternative. When CSD lymph nodes suppurate, needle aspiration is probably the best treatment, and the patient usually notes decreased pain within 24 to 48 h. If fluid reaccumulates, needle reaspiration may be needed (72).

Complicated CSD.

Various antibiotic regimens have been used to treat patients with complicated CSD (retinitis, encephalopathy, and visceral forms) (56, 108). The combination of doxycycline (100 mg p.o. or i.v. twice daily) with rifampin (300 mg p.o. twice daily) has been successful in treating patients with retinitis (Table (Table6,6, recommendation AII) (56, 84, 108). If treatment is chosen for patients with central nervous system (CNS) disease, the combination of doxycycline and rifampin is preferred. The optimum duration of antibiotic therapy for immunocompetent patients with complicated CSD has not been determined. Of note, there is a marked difference between the dramatic clinical response to antibiotics observed in immunocompromised patients with CSD and the minimal response observed in immunocompetent patients.


B. quintana is transmitted by the human body louse, and humans are the only known reservoir (76). An acute form (trench fever) and a chronic form (chronic bacteremia) of the disease have been reported in immunocompetent individuals (76).

Trench fever, also known as 5-day fever or quintan fever, is a manifestation of initial infection with B. quintana and is characterized by infection of human red blood cells. Detailed descriptions of the disease were first reported in infected troops during World War I (76). Clinical manifestations of trench fever range from asymptomatic infection to severe illness. The classical presentation reported among troops was that of a febrile illness of acute onset, often accompanied by severe headache, dizziness, and pain in the shins. A minority of patients with trench fever developed chronic infection, with or without attacks of fever and aching (20); some of these soldiers developed persistent bacteremia (76). More recently, B. quintana has been demonstrated to cause chronic bacteremia in homeless people (19, 35, 100). In a study performed in emergency rooms of university hospitals in Marseilles, France, 14% of homeless were found to be chronically bacteremic, some for several months, without any signs or symptoms of disease (19, 61).

Most cases of trench fever, the acute form of B. quintana bacteremia, were reported prior to the antibiotic era. There were no fatal cases of trench fever, and the clinical manifestations lasted for 4 to 6 weeks before full recovery. Aspirin was the most effective drug for the pain; and during World War II, soldiers with trench fever were “maintained in hospital no longer than necessary, then sent to convalescent depot where fresh air, good food and progressive exercise quickly restored them to full capacity so that they were able to return to duty” (44). During World War I, soldiers with trench fever cleared the infection in the absence of antibiotic treatment. However, successful treatment of some trench fever patients with tetracycline or chloramphenicol was reported after World War II, although these data remain anecdotal (10). Thus, it seems reasonable to prescribe doxycycline for such patients. In addition, we recommend that patients with the acute form of B. quintana bacteremia be treated with gentamicin (3 mg/kg of body weight i.v. once daily for 14 days), in combination with doxycycline (200 mg p.o. daily) for 28 days (Table (Table6,6, recommendation AI). Treatment of paucisymptomatic, persistent B. quintana bacteremia may be of importance for the prevention of endocarditis in these patients (35). A retrospective review of the treatment histories for patients with chronic bacteremia found that only those who were treated with doxycycline for 4 weeks and gentamicin for 14 days were cured, whereas those treated with beta-lactams or doxycycline alone were not (35). These results have been confirmed recently in a randomized, placebo-controlled clinical trial (36). In that study, homeless people with blood cultures positive for B. quintana were randomized to receive either no treatment (untreated controls) or a combination of gentamicin (3 mg/kg of body weight/day i.v. for 14 days) and doxycycline (200 mg/day p.o. for 28 days). Patients were evaluated by blood cultures, performed between day 28 (the end of treatment) and day 90 postinclusion. In the per-protocol analysis, eradication was obtained for seven of seven treated patients and two of nine untreated controls (P = 0.003). Consequently, patients with chronic B. quintana bacteremia or trench fever should be treated with gentamicin (3 mg/kg i.v. once daily) for the first 14 days, in addition to doxycycline (200 mg daily) for 28 days (Table (Table6,6, recommendation AI) (36). Doxycycline could be given either as a single daily dose of 200 mg every 24 h or as a twice-daily dose of 100 mg every 12 h. Patients with chronic bacteremia should be carefully evaluated for endocarditis, because the presence of this complication will necessitate a longer duration of therapy and closer monitoring. The gentamicin levels in patients with renal insufficiency, obesity, or increased fluid volume should be monitored closely; and a reduced total daily dose of gentamicin should be administered as a twice-daily dosing schedule to avoid the nephrotoxicity of the drug.


Both B. henselae and B. quintana can cause endocarditis and can cause BA in immunocompromised hosts, such as human immunodeficiency virus (HIV)-infected patients (5, 57). Bacillary PH occurs in immunocompromised patients and is caused by B. henselae, but not B. quintana (Table (Table2)2) (57).

BA and PH.

Severe, progressive, disseminated disease may occur in immunocompromised patients, especially those with HIV infection. Without appropriate therapy, infection spreads systemically and can involve virtually any organ, and the outcome is sometimes fatal (9).

BA is a vascular proliferative disease most often involving the skin, but it may involve other organs. The disease was first described in HIV-infected patients (102) and organ transplant recipients (50), but it can also rarely affect immunocompetent patients (105). The clinical differential diagnosis includes pyogenic granuloma, hemangioma, subcutaneous tumors, and Kaposi's sarcoma (76). The skin lesions are very similar to those reported for verruga peruana, the chronic form of Carrion's disease. BA lesions can also involve the bone marrow, liver, spleen, or lymph nodes (24, 54, 69, 77).

PH is defined as a vascular proliferation of sinusoidal hepatic capillaries resulting in blood-filled spaces in the liver. This disease was first described in patients with tuberculosis and advanced cancers and in association with the use of drugs such as anabolic steroids (53). B. henselae is now recognized as an infectious cause of PH in HIV-infected patients (73, 80). PH has also been reported in organ transplant recipients (1). PH can occur simultaneously with peliosis of the spleen, as well as BA of the skin, in HIV-infected patients (58, 64).

Antibiotic treatment of BA and PH has never been studied systematically. Two criteria must be met to achieve successful eradication of Bartonella infections in the immunocompromised patient: first, the specific strain of B. henselae and B. quintana infecting the patient must have excellent in vivo susceptibility to the prescribed antibiotic, and second, the treatment must be of sufficient duration to prevent relapse. The first patient with BA to be described was treated empirically with erythromycin, and the lesions resolved completely (102). Subsequently, erythromycin has become the drug of first choice and has successfully been used to treat many patients with BA (Table (Table4)4) (58, 105). Treatment of BA and PH with oral doxycycline (100 mg twice daily) has also been consistently successful (58). Lesions resolved in several patients treated with ceftriaxone or fluoroquinolone compounds (65, 96), but the progression of BA lesions in patients has been observed during treatment with ciprofloxacin (104). Additionally, a Bartonella species has been isolated from the blood or BA lesions of patients being treated with narrow-spectrum cephalosporins (55), nafcillin, gentamicin, and trimethoprim-sulfamethoxazole (but never from patients being treated with a macrolide, rifamycin, or a tetracycline) (57). We therefore do not recommend fluoroquinolones, trimethoprim-sulfamethoxazole, or narrow-spectrum cephalosporins for the treatment of BA or PH (58). Treatment failures have been reported with many different antibiotics, and these are usually attributable to a lack of susceptibility of Bartonella in vivo and/or an insufficient duration of therapy (58, 75).

The drug of choice for the treatment of BA is erythromycin given p.o. (500 mg p.o. four times daily) for 3 months (Table (Table6,6, recommendation AII), but i.v. administration should be used in patients with severe disease (58). Patients intolerant of erythromycin can be treated with doxycycline (100 mg p.o. or i.v. twice daily) (Table (Table6,6, recommendation AII) (52, 58, 81). The response to treatment appears to be equivalent whether erythromycin or doxycycline is prescribed (56). Combination therapy, with the addition of rifampin (300 mg p.o. twice daily) to either erythromycin or doxycycline, is recommended for immunocompromised patients with acute, life-threatening Bartonella infection. The intravenous route is especially important in cases of gastrointestinal intolerance or poor absorption. The combination of doxycycline and rifampin is preferred for the treatment of patients with CNS Bartonella infection because of the superior CNS penetration of doxycycline compared with those of the other first-line antibiotics.

The response to treatment can be dramatic in immunocompromised patients. In one patient who received a single 250-mg oral dose of erythromycin, blood cultures became sterile and a palpable subcutaneous lesion disappeared within hours (but recurred months later). More chronic lesions resolve more slowly, but after approximately 4 to 7 days of therapy, cutaneous BA lesions usually improve and resolve completely after 1 month of treatment (11). Bacillary PH responds more slowly than cutaneous BA, but hepatic lesions should improve after several months of treatment.

Relapses of PH and BA lesions in bone and skin have been reported frequently (38, 55, 62, 103). Relapses occur when antibiotics are given for a shorter duration (<3 months), especially in severely immunocompromised HIV-infected patients (58, 96). For this reason and from our extensive experience treating patients with BA and PH, we recommend that treatment be given for at least 3 months for BA and 4 months for PH (Table (Table6,6, recommendation AII) (25, 56). All immunocompromised patients with a Bartonella infection should receive antibiotic therapy (erythromycin 500 mg p.o. four times daily or doxycycline 100 mg p.o. twice daily); patients who have relapses after the recommended treatment should then receive secondary prophylactic antibiotic treatment with erythromycin (500 mg p.o. four times daily) or doxycycline (100 mg p.o. twice daily) as long as they are immunocompromised (56). Of note, AIDS patients receiving prophylaxis with a macrolide or rifamycin antibiotic for Mycobacterium avium complex infection appear to be protected from developing infections with Bartonella species (57). Some immunocompromised patients develop a potentially life-threatening Jarisch-Herxheimer-like reaction within hours after institution of antibiotic therapy (55). Physicians should advise patients of this possible treatment complication, and patients with severe respiratory and/or cardiovascular compromise should be monitored carefully following institution of antimicrobial therapy (56).


Evidence of Bartonella infection was found in 3% of all patients diagnosed with endocarditis tested at reference centers in three different countries (73). B. quintana (32, 37, 82, 83, 98, 99), B. henselae (31, 37, 41, 82, 83), and other species, such as Bartonella elizabethae (27) and Bartonella vinsonii subsp. berkhoffii (92), have been isolated from individual patients with bacterial endocarditis. Of the Bartonella species, B. quintana is the one that most commonly causes endocarditis, followed by B. henselae. The first case of Bartonella endocarditis was reported in an HIV-infected homosexual man in 1993 (98). B. quintana endocarditis has subsequently been reported in three non-HIV-infected, homeless men in France (32). All three patients required valve replacements because of extensive valvular damage, and pathological investigation confirmed the diagnosis of endocarditis.

B. quintana endocarditis is most often observed in homeless people with chronic alcoholism and exposure to body lice and in patients without previously known valvulopathy. B. henselae endocarditis most often occurs in patients with known valvulopathy who have contact with cats or cat fleas (37).

Bartonella endocarditis is usually indolent and culture negative, and thus, diagnosis is often delayed, resulting in a mortality rate higher than that for some other forms of endocarditis. It was previously demonstrated (37) that patients with Bartonella endocarditis have a higher death rate and undergo valvular surgery more frequently than patients with endocarditis caused by other pathogens. Selection of an adequate treatment regimen is critical, even when Bartonella infection is suspected but not yet documented. Among 101 patients with Bartonella endocarditis recently described in a retrospective study (83), 82 received aminoglycosides for a mean of 15 ± 11 days with either a beta-lactam (64 cases) or other antibiotics (vancomycin, doxycycline, rifampin, or co-trimoxazole). Seventy-four of the 82 patients who received an aminoglycoside recovered, whereas 13 of 19 of those who received no aminoglycoside recovered (P = 0.02) (84). Among the patients treated with aminoglycosides, 65 of the 69 who recovered had received aminoglycosides for 14 or more days, whereas 9 of the 13 patients who recovered had been treated for less than 14 days (P = 0.02). Patients receiving an aminoglycoside were more likely to recover fully and, if they were treated for at least 14 days, were more likely to survive, confirming the important role of this antibiotic in the treatment of Bartonella endocarditis (83). These data strongly support the use of aminoglycoside therapy for at least 14 days for patients with suspected Bartonella sp. endocarditis (Table (Table6,6, recommendation AII). Aminoglycoside therapy should be accompanied by treatment with a beta-lactam compound, preferably ceftriaxone (which is especially important for patients for whom blood cultures are negative, to adequately treat other potential bacteria that cause culture-negative endocarditis, e.g., β-lactamase-producing Haemophilus spp.). Thus, we recommend that patients with suspected (but culture-negative) Bartonella endocarditis receive treatment with gentamicin for the first 2 weeks and ceftriaxone (Table (Table6,6, recommendation BII) with or without doxycycline (Table (Table6,6, recommendation BII) for 6 weeks (83).

Because chronic B. quintana bacteremia has been shown to be optimally treated with doxycycline plus gentamicin (36), in the absence of any prospective study for the treatment of documented Bartonella endocarditis, it is logical that the same regimen should be used for endocarditis when a Bartonella sp. has been identified as the causative agent. It is important that no difference in the frequency of surgery was observed in patients whether or not they were treated with aminoglycosides. This may be explained by the severity of valvular lesions at the time when the diagnosis of endocarditis is made (37, 83). Patients should be monitored closely, and the dose of gentamicin should be chosen and adjusted according to the renal function of the patient, with a twice-daily dosing schedule for patients with renal insufficiency or those at risk for the development of aminoglycoside-induced renal failure. If renal dysfunction precludes the use of gentamicin for documented Bartonella endocarditis, rifampin could be considered as the second drug to be added to doxycycline.


Oroya fever (acute Carrion's disease)

B. bacilliformis is a sandfly-transmitted Bartonella species (3) that is responsible for life-threatening septicemia with acute hemolysis known as Oroya fever (2). This infection occurs most commonly in the Andes of Peru, especially in immunologically naive people, such as tourists and transient workers (39, 68, 94, 95). Oroya fever results from the massive invasion of human red blood cells by B. bacilliformis and causes death in 40 to 85% of infected humans who do not receive treatment (45). In 35% of cases, Oroya fever is complicated by superinfections, primarily non-serovar Typhi Salmonella enterica and S. enterica serovar Typhimurium infections and sepsis caused by Enterobacter, Staphylococcus aureus, Pseudomona aeruginosa, and other organisms.

Before the antibiotic era, the only available treatment for the acute anemia of Oroya fever was blood transfusion, but the effectiveness of this treatment was poor and the mortality rate was high (about 80% of cases) (94). Penicillin G, chloramphenicol, tetracycline, and erythromycin have been used for the treatment of Oroya fever. Treatment with these drugs produces rapid defervescence, with disappearance of the organisms from the blood, usually within 24 h (10). However, because many patients suffer from secondary infections, especially salmonellosis and infections caused by other enteropathogenic bacteria, chloramphenicol has become the recommended antibiotic therapy (26, 106). In Peru, 14 of 16 (88%) patients with Oroya fever who were not treated died, but none of any of 10 patients who were treated with chloramphenicol died (Table (Table4)4) (39). In a large series of acute cases of Oroya fever reported recently, all 23 patients who received chloramphenicol with another antibiotic were cured, whereas 6 of 42 patients treated with chloramphenicol alone failed therapy and needed penicillin (3 patients) and 3 developed chronic verruga peruana lesions within the first 3 months of recovery after the acute phase (Table (Table4)4) (66). Therapeutic failures and persistent bacteremia have been reported when chloramphenicol was used, and successful treatment with this drug does not appear to eliminate the patient's risk for development of the eruptive phase of B. bacilliformis infection. Because chloramphenicol is effective in most but not all patients with Oroya fever, simultaneous treatment with another antibiotic (especially a beta-lactam compound) is recommended (Table (Table6,6, recommendation AII) (66). Trimethoprim-sulfamethoxazole, macrolides (roxithromycin), and fluoroquinolones (norfloxacin and ciprofloxacin) have also been used successfully in some patients (68). Fluoroquinolone compounds have been used successfully in the last 5 years in adults and children over age 6 years and represent an alternative to chloramphenicol for the treatment of Oroya fever (Table (Table6,6, recommendation BIII) (C. Maguina, unpublished data). Note that fluoroquinolones should be used with caution in children.

Verruga peruana.

Among the native population of the Andes of Peru, Carrion's disease also presents as a chronic illness called “verruga peruana.” The infection is characterized by benign cutaneous vascular lesions which typically consist of round papules that are frequently pruritic and bleeding, and the infection is accompanied by osteoarticular pain (6, 66, 68). Only 5% of patients with verruga peruana recall having had an acute febrile illness in the previous 3 months (66). B. bacilliformis can be isolated from blood cultures and can be observed in blood films in 13% of patients with verruga peruana, indicating that these patients are sometimes bacteremic (66).

Verruga peruana is caused by the same bacterium that causes Oroya fever, but chloramphenicol is ineffective treatment for this eruptive stage of infection with B. bacilliformis (68). The treatment used for verruga peruana has traditionally been streptomycin (15 to 20 mg/kg of body weight intramuscularly [i.m.] once daily) for 10 days (Table (Table6,6, recommendation AII), but the use of the i.m. route remains problematic, especially in children (66). Since 1975, rifampin has become the drug of choice for treatment of the eruptive phase of Carrion's disease (Table (Table6,6, recommendation AII) (66). In a recent study, 55 of 77 patients with the eruptive phase of Carrion's disease received antimicrobial therapy; 46 of the 55 patients received oral rifampin (10 mg/kg/day for 10 to 14 days) and 9 received i.m. streptomycin (15 mg/kg/day for 10 days). Thirty-seven (80%) of the 46 patients treated with rifampin had a good response, whereas 5 (56%) of the 9 patients treated with streptomycin had a good response (Table (Table4).4). The efficacy of rifampin has been found to be comparable to that of streptomycin, with the disappearance of cutaneous lesions within a month of therapy. However, failures of rifampin treatment have also been reported (68). Rapid resistance to rifampin can develop when rifampin is used alone, and thus, rifampin alone is not recommended for the treatment of any Bartonella infection except verruga peruana. More recently, ciprofloxacin at 500 mg p.o. twice daily for 7 to 10 days has been used with success for the treatment of adults with multiple eruptive-phase lesions, as has azithromycin (67).

Data for treatment during pregnancy are scarce. There are conflicting reports on the safety of chloramphenicol during pregnancy (4). Gray baby syndrome is seen in premature babies given chloramphenicol. Eight pregnant women with B. bacilliformis infection were evaluated in a study by Maguina and Gotuzzo (66); five of the women presented in the acute phase and three presented in the eruptive phase. Two of the five women in the acute phase died. Among the three surviving pregnant patients who were treated with chloramphenicol, one had an abortion with typhoid fever, the second had fetal demise, and the third delivered the baby without complications. Among the three pregnant women who had verruga peruana and who were treated with rifampin, the babies were born with no complications or lesions (66).


Well-designed clinical trials with numerous subjects, a standard case definition, and molecular biology assay and/or culture confirmation are needed in order to better define the optimum treatment for Bartonella infections. Multicenter clinical trials will be necessary in order to accrue a sufficient number of patients with Bartonella infections, such endocarditis, BA, and CSD.


Bacteria of the genus Bartonella are responsible for emerging and reemerging diseases worldwide and can present as illnesses ranging from benign and self-limited diseases to severe and life-threatening diseases. Bartonella infections present a unique treatment challenge because they are persistent and often relapse and they involve an intraerythrocytic phase that apparently provides a protective niche for the bartonellae. The extreme diversity of disease manifestations is dependent on the infecting species of Bartonella and on the immune status of the patient. Because there are only two reports of randomized clinical trials for the treatment of Bartonella infections, an unequivocal treatment for all Bartonella infections does not exist, and thus, antibiotic treatment recommendations differ for each clinical situation. Treatment of Bartonella infections should be adapted to each clinical situation, to the infecting Bartonella species, and to whether the disease is in the acute or the chronic form. It is important that when the more severe Bartonella infections are recognized, diagnosed, and treated in a timely manner, the outcome is usually favorable.


We thank S. Dumler for reviewing the manuscript.

J.E.K. receives support from NIH R01 grants AI052813 and AI43703, The Burroughs Wellcome Fund, and the University of California, San Francisco, Academic Senate.


1. Ahsan, N., M. J. Holman, T. R. Riley, C. S. Abendroth, E. G. Langhoff, and H. C. Yang. 1998. Peliosis hepatis due to Bartonella henselae in transplantation: a hemato-hepato-renal syndrome. Transplantation 65:1000-1003. [PubMed]
2. Alexander, B. 1995. A review of bartonellosis in Ecuador and Colombia. Am. J. Trop. Med. Hyg. 52:354-359. [PubMed]
3. Amano, Y., J. Rumbea, J. Knobloch, J. Olson, and M. Kron. 1997. Bartonellosis in Ecuador: serosurvey and current status of cutaneous verrucous disease. Am. J. Trop. Med. Hyg. 57:174-179. [PubMed]
4. Amstey, M. S. 2000. Chloramphenicol therapy in pregnancy. Clin. Infect. Dis. 30:237. [PubMed]
5. Anderson, B. E., and M. A. Neuman. 1997. Bartonella spp. as emerging human pathogens. Clin. Microbiol. Rev. 10:203-219. [PMC free article] [PubMed]
6. Arias-Stella, J., P. H. Lieberman, R. A. Erlandson, and J. Arias-Stella, Jr. 1986. Histology, immunohistochemistry, and ultrastructure of the verruga in Carrion's disease. Am. J. Surg. Pathol. 10:595-610. [PubMed]
7. Baker, J. A. 1946. A rickettsial infection in Canadian voles. J. Exp. Med. 84:37-51. [PMC free article] [PubMed]
8. Bass, J. W., B. C. Freitas, A. D. Freitas, C. L. Sisler, D. S. Chan, J. M. Vincent, D. A. Person, J. R. Claybaugh, R. R. Wittler, M. E. Weisse, R. L. Regnery, and L. N. Slater. 1998. Prospective randomized double blind placebo-controlled evaluation of azithromycin for treatment of cat-scratch disease. Pediatr. Infect. Dis. J. 17:447-452. [PubMed]
9. Bass, J. W., J. M. Vincent, and D. A. Person. 1997. The expanding spectrum of Bartonella infections. II. Cat-scratch disease. Pediatr. Infect. Dis. J. 16:163-179. [PubMed]
10. Bass, J. W., J. M. Vincent, and D. A. Person. 1997. The expanding spectrum of Bartonella infections. I. Bartonellosis and trench fever. Pediatr. Infect. Dis. J. 16:2-10. [PubMed]
11. Berger, T. G., and L. A. Perkocha. 1991. Bacillary angiomatosis. AIDS Clin. Rev. 1991:81-95. [PubMed]
12. Bermond, D., H. J. Boulouis, R. Heller, G. Van Laere, H. Monteil, B. B. Chomel, A. Sander, C. Dehio, and Y. Piemont. 2002. Bartonella bovis Bermond et al. sp. nov. and Bartonella capreoli sp. nov., isolated from European ruminants. Int. J. Syst. Evol. Microbiol. 52(Pt 2):383-390. [PubMed]
13. 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. Evol. Microbiol. 50(Pt 6):1973-1979. [PubMed]
14. Birtles, R. J., T. G. Harrison, N. A. Saunders, and D. H. Molyneux. 1995. Proposals to unify the genera Grahamella and Bartonella, with descriptions of Bartonella talpae comb. nov., Bartonella peromysci comb. nov., and three new species, Bartonella grahamii sp. nov., Bartonella taylorii sp. nov., and Bartonella doshiae sp. nov. Int. J. Syst. Bacteriol. 45:1-8. [PubMed]
15. 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]
16. 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]
17. 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]
18. Brenner, D. J., S. O'Connor, H. H. Winkler, and A. G. Steigerwalt. 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. 43:777-786. [PubMed]
19. Brouqui, P., B. La Scola, V. Roux, and D. Raoult. 1999. Chronic Bartonella quintana bacteremia in homeless patients. N. Engl. J. Med. 340:184-189. [PubMed]
20. Byam, W., J. H. Caroll, J. H. Churchill, L. Dimond, V. E. Sorapure, R. M. Wilson, and L. L. Lloyd. 1919. Trench fever, a louse-born disease. Oxford University Press, London, United Kingdom.
21. Carithers, H. A. 1985. Cat-scratch disease. An overview based on a study of 1200 patients. Am. J. Dis. Child. 139:1124-1133. [PubMed]
22. Chang, C. C., B. B. Chomel, R. W. Kasten, R. M. Heller, H. Ueno, K. Yamamoto, V. C. Bleich, B. M. Pierce, B. J. Gonzales, P. K. Swift, W. M. Boyce, S. S. Jang, H. J. Boulouis, Y. Piémont, G. M. Rossolini, M. L. Riccio, G. Cornaglia, L. Pagani, C. Lagatolla, L. Selan, and R. Fontana. 2000. Bartonella spp. isolated from wild and domestic ruminants in North America. Emerg. Infect. Dis. 6:306-311. [PMC free article] [PubMed]
23. Chomel, B. B., R. W. Kasten, K. Floyd-Hawkins, B. Chi, K. Yamamoto, J. Roberts-Wilson, A. N. Gurfield, R. C. Abbott, N. C. Pedersen, and J. E. Koehler. 1996. Experimental transmission of Bartonella henselae by the cat flea. J. Clin. Microbiol. 34:1952-1956. [PMC free article] [PubMed]
24. Cockerell, C. J., M. A. Whitlow, G. F. Webster, and A. E. Friedman-Kien. 1987. Epithelioid angiomatosis: a distinct vascular disorder in patients with the acquired immunodeficiency syndrome or AIDS-related complex. Lancet ii:654-656. [PubMed]
25. Cotell, S. L., and G. A. Noskin. 1994. Bacillary angiomatosis. Clinical and histologic features, diagnosis, and treatment. Arch. Intern. Med. 154:524-528. [PubMed]
26. Cuadra, M. 1956. Salmonellosis complications in human bartonellosis. Tex. Rep. Biol. Med. 14:97-113. [PubMed]
27. 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]
28. Dehio, C. 2001. Bartonella interactions with endothelial cells and erythrocytes. Trends Microbiol. 9:279-285. [PubMed]
29. Dehio, C., C. Lanz, R. Pohl, P. Behrens, D. Bermond, Y. Piemont, K. Pelz, and A. Sander. 2001. Bartonella schoenbuchii sp. nov., isolated from the blood of wild roe deer. Int. J. Syst. Evol. Microbiol. 51(Pt 4):1557-1565. [PubMed]
30. Dolan, M. J., M. T. Wong, R. L. Regnery, J. H. Jorgensen, M. Garcia, J. Peters, and D. Drehner. 1993. Syndrome of Rochalimaea henselae adenitis suggesting cat scratch disease. Ann. Intern. Med. 118:331-336. [PubMed]
31. Drancourt, M., R. J. Birtles, G. Chaumentin, F. Vandenesch, J. Etienne, and D. Raoult. 1996. New serotype of Bartonella henselae in endocarditis and cat-scratch disease. Lancet 347:441-443. [PubMed]
32. 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]
33. Droz, S., B. Chi, E. Horn, A. G. Steigerwalt, A. M. Whitney, and D. J. Brenner. 1999. Bartonella koehlerae sp. nov., isolated from cats. J. Clin. Microbiol. 37:1117-1122. [PMC free article] [PubMed]
34. English, C. K., D. J. Wear, A. M. Margileth, C. R. Lissner, and G. P. Walsh. 1988. Cat-scratch disease: isolation and culture of the bacterial agent. JAMA 259:1347-1351. [PubMed]
35. Foucault, C., K. Barrau, P. Brouqui, and D. Raoult. 2002. Bartonella quintana bacteremia among homeless people. Clin. Infect. Dis. 35:684-689. [PubMed]
36. Foucault, C., D. Raoult, and P. Brouqui. 2003. Randomized open trial of gentamicin and doxycycline for eradication of Bartonella quintana from blood in patients with chronic bacteremia. Antimicrob. Agents Chemother. 47:2204-2207. [PMC free article] [PubMed]
37. Fournier, P. E., H. Lelievre, S. J. Eykyn, J. L. Mainardi, T. J. Marrie, F. Bruneel, C. Roure, J. Nash, D. Clave, E. James, C. Benoit-Lemercier, L. Deforges, H. Tissot-Dupont, and D. Raoult. 2001. Epidemiologic and clinical characteristics of Bartonella quintana and Bartonella henselae endocarditis: a study of 48 patients. Medicine (Baltimore) 80:245-251. [PubMed]
38. Gazineo, J. L., B. M. Trope, J. P. Maceira, S. B. May, J. M. Coelho, J. S. Lambert, and S. A. Nogueira. 2001. Bacillary angiomatosis: description of 13 cases reported in five reference centers for AIDS treatment in Rio de Janeiro, Brazil. Rev. Inst. Med. Trop. Sao Paulo 43:1-6. [PubMed]
39. Gray, G. C., A. A. Johnson, S. A. Thornton, W. A. Smith, J. Knobloch, P. W. Kelley, L. O. Escudero, M. A. Huayda, and F. S. Wignall. 1990. An epidemic of Oroya fever in the Peruvian Andes. Am. J. Trop. Med. Hyg. 42:215-221. [PubMed]
40. Greene, C. E., M. McDermott, P. H. Jameson, C. L. Atkins, and A. M. Marks. 1996. Bartonella henselae infection in cats: evaluation during primary infection, treatment, and rechallenge infection. J. Clin. Microbiol. 34:1682-1685. [PMC free article] [PubMed]
41. Hadfield, T. L., R. Warren, M. Kass, E. Brun, and C. Levy. 1993. Endocarditis caused by Rochalimaea henselae. Hum. Pathol. 24:1140-1141. [PubMed]
42. Heller, R., M. Kubina, P. Mariet, P. Riegel, G. Delacour, C. Dehio, F. Lamarque, R. Kasten, H. J. Boulouis, H. Monteil, B. Chomel, and Y. Piemont. 1999. Bartonella alsatica sp. nov., a new Bartonella species isolated from the blood of wild rabbits. Int. J. Syst. Bacteriol. 49:283-288. [PubMed]
43. Heller, R., P. Riegel, Y. Hansmann, G. Delacour, D. Bermond, C. Dehio, F. Lamarque, H. Monteil, B. Chomel, and Y. Piémont. 1998. Bartonella tribocorum sp.nov., a new Bartonella species isolated from the blood of wild rats. Int. J. Syst. Bacteriol. 48:1333-1339. [PubMed]
44. Hurst, H. 1942. Trench fever. Br. Med. J. 70:318-320.
45. Ihler, G. M. 1996. Bartonella bacilliformis: dangerous pathogen slowly emerging from deep background. FEMS Microbiol. Lett. 144:1-11. [PubMed]
46. Ives, T. J., P. Manzewitsch, R. L. Regnery, J. D. Butts, and M. Kebede. 1997. In vitro susceptibilities of Bartonella henselae, B. quintana, B. elizabethae, Rickettsia rickettsii, R. conorii, R. akari, and R. prowazekii to macrolide antibiotics as determined by immunofluorescent-antibody analysis of infected Vero cell monolayers. Antimicrob. Agents Chemother. 41:578-582. [PMC free article] [PubMed]
47. Ives, T. J., E. L. Marston, R. L. Regnery, and J. D. Butts. 2001. In vitro susceptibilities of Bartonella and Rickettsia spp. to fluoroquinolone antibiotics as determined by immunofluorescent antibody analysis of infected Vero cell monolayers. Int. J. Antimicrob. Agents 18:217-222. [PubMed]
48. Ives, T. J., E. L. Marston, R. L. Regnery, J. D. Butts, and T. C. Majerus. 2000. In vitro susceptibilities of Rickettsia and Bartonella spp. to 14-hydroxy-clarithromycin as determined by immunofluorescent antibody analysis of infected Vero cell monolayers. J. Antimicrob. Chemother. 45:305-310. [PubMed]
49. Jacomo, V., P. J. Kelly, and D. Raoult. 2002. Natural history of Bartonella infections (an exception to Koch's postulate). Clin. Diagn. Lab. Immunol. 9:8-18. [PMC free article] [PubMed]
50. Kemper, C. A., C. M. Lombard, S. C. Deresinski, and L. S. Tompkins. 1990. Visceral bacillary epithelioid angiomatosis: possible manifestations of disseminated cat scratch disease in the immunocompromised host: a report of two cases. Am. J. Med. 89:216-222. [PubMed]
51. Kish, M. A. 2001. Guide to development of practice guidelines. Clin. Infect. Dis. 32:851-854. [PubMed]
52. Koehler, J. E. 1995. Bartonella-associated infections in HIV-infected patients. AIDS Clin. Care 7:97-102. [PubMed]
53. Koehler, J. E. 1996. Bartonella infections. Adv. Pediatr. Infect. Dis. 11:1-27. [PubMed]
54. Koehler, J. E., P. E. Leboit, B. M. Egbert, and T. G. Berger. 1988. Cutaneous vascular lesions and disseminated cat-scratch disease in patients with the acquired immunodeficiency syndrome (AIDS) and AIDS-related complex. Ann. Intern. Med. 109:449-455. [PubMed]
55. Koehler, J. E., F. D. Quinn, T. G. Berger, P. E. Leboit, and J. W. Tappero. 1992. Isolation of Rochalimaea species from cutaneous and osseous lesions of bacillary angiomatosis. N. Engl. J. Med. 327:1625-1631. [PubMed]
56. Koehler, J. E., and D. A. Relman. 2002. Bartonella species, p. 925-931. In V. L. Yu, R. Weber, and D. Raoult (ed.), Antimicrobial therapy and vaccines. Apple Trees Production, LLC, New York, N.Y.
57. Koehler, J. E., M. A. Sanchez, C. S. Garrido, M. J. Whitfeld, F. M. Chen, T. G. Berger, M. C. Rodriguez-Barradas, P. E. LeBoit, and J. W. Tappero. 1997. Molecular epidemiology of Bartonella infections in patients with bacillary angiomatosis-peliosis. N. Engl. J. Med. 337:1876-1883. [PubMed]
58. Koehler, J. E., and J. W. Tappero. 1993. Bacillary angiomatosis and bacillary peliosis in patients infected with human immunodeficiency virus. Clin. Infect. Dis. 17:612-624. [PubMed]
59. 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]
60. Kordick, D. L., M. G. Papich, and E. B. Breitschwerdt. 1997. Efficacy of enrofloxacin or doxycycline for treatment of Bartonella henselae or Bartonella clarridgeiae infection in cats. Antimicrob. Agents Chemother. 41:2448-2455. [PMC free article] [PubMed]
61. Kostrzewski, J. 1949. The epidemiology of trench fever. Bull. Acad. Polonaise Sci. Lett. Classe Med. 7:233-263. [PubMed]
62. Krekorian, T. D., A. B. Radner, J. M. Alcorn, P. Haghighi, and F. C. Fang. 1990. Biliary obstruction caused by epithelioid angiomatosis in patient with AIDS. Am. J. Med. 820-822. [PubMed]
63. La Scola, B., and D. Raoult. 1999. Culture of Bartonella quintana and Bartonella henselae from human samples: a 5-year experience (1993 to 1998). J. Clin. Microbiol. 37:1899-1905. [PMC free article] [PubMed]
64. Leong, S. S., R. A. Cazen, G. S. Yu, L. LeFevre, and J. W. Carson. 1992. Abdominal visceral peliosis associated with bacillary angiomatosis. Ultrastructural evidence of endothelial destruction by bacilli. Arch. Pathol. Lab. Med. 116:866-871. [PubMed]
65. Lucey, D., M. J. Dolan, C. W. Moss, M. Garcia, D. G. Hollis, S. Wegner, G. Morgan, R. Almeida, D. Leong, K. S. Greisen, et al. 1992. Relapsing illness due to Rochalimaea henselae in immuno competent hosts: implication for therapy and new epidemiological associations. Clin. Infect. Dis. 14:683-688. [PubMed]
66. Maguina, C., P. J. Garcia, E. Gotuzzo, L. Cordero, and D. H. Spach. 2001. Bartonellosis (Carrion's disease) in the modern era. Clin. Infect. Dis. 33:772-779. [PubMed]
67. Maguina, C., and E. Gotuzzo. 2000. Bartonellosis—new and old. Infect. Dis. Clin. N. Am. 14:1-22. [PubMed]
68. Maguina Vargas, C. 1998. Bartonellosis o enfermedad de carrion. Nuevos aspectos de una vieja enfermedad, p. 7-195. AFA Editores Importadores, Lima, Peru.
69. Marasco, W. A., S. Lester, and J. Parsonnet. 1989. Unusual presentation of cat scratch disease in a patient positive for antibody to the human immunodeficiency virus. Rev. Infect. Dis. 11:793-803. [PubMed]
70. Margileth, A. M. 1992. Antibiotic therapy for cat-scratch disease: clinical study of therapeutic outcome in 268 patients and a review of the literature. Pediatr. Infect. Dis. J. 11:474-478. [PubMed]
71. Margileth, A. M. 1993. Cat scratch disease. Adv. Pediatr. Infect. Dis. 8:1-21. [PubMed]
72. Margileth, A. M. 2000. Recent advances in diagnosis and treatment of cat scratch disease. Curr. Infect. Dis. Rep. 2:141-146. [PubMed]
73. Maurin, M., R. J. Birtles, and D. Raoult. 1997. Current knowledge of Bartonella species. Eur. J. Clin. Microbiol. Infect. Dis. 16:487-506. [PubMed]
74. Maurin, M., S. Gasquet, C. Ducco, and D. Raoult. 1995. MICs of 28 antibiotic compounds for 14 Bartonella (formerly Rochalimaea) isolates. Antimicrob. Agents Chemother. 39:2387-2391. [PMC free article] [PubMed]
75. Maurin, M., and D. Raoult. 1993. Antimicrobial susceptibility of Rochalimaea quintana, Rochalimaea vinsonii and the newly recognized Rochalimaea henselae. J. Antimicrob. Chemother. 32:587-594. [PubMed]
76. Maurin, M., and D. Raoult. 1996. Bartonella (Rochalimaea) quintana infections. Clin. Microbiol. Rev. 9:273-292. [PMC free article] [PubMed]
77. Milam, M. W., M. J. Balerdi, J. F. Toney, P. R. Foulis, C. P. Milam, and R. H. Behnke. 1990. Epithelioid angiomatosis secondary to disseminated cat scratch disease involving the bone marrow and skin in a patient with acquired immune deficiency syndrome: a case report. Am. J. Med. 88:180-183. [PubMed]
78. Musso, D., M. Drancourt, and D. Raoult. 1995. Lack of bactericidal effect of antibiotics except aminoglycosides on Bartonella (Rochalimaea) henselae. J. Antimicrob. Chemother. 36:101-108. [PubMed]
79. Myers, W. F., D. M. Grossman, and C. L. Wisseman, Jr. 1984. Antibiotic susceptibility patterns in Rochalimaea quintana, the agent of trench fever. Antimicrob. Agents Chemother. 25:690-693. [PMC free article] [PubMed]
80. Perkocha, L. A., S. M. Geaghan, B. T. S. Yen, S. L. Nishimura, S. P. Chan, R. Garcia-Kennedy, G. Honda, A. C. Stoloff, H. Z. Klein, R. L. Goldman, S. Van Meter, L. Ferrell, and P. E. LeBoit. 1990. Clinical and pathological features of bacillary peliosis hepatis in association with human immunodeficiency virus infection. N. Engl. J. Med. 323:1581-1586. [PubMed]
81. Ramirez Ramirez, C. R., S. Saavedra, and C. H. Ramirez Ronda. 1996. Bacillary angiomatosis: microbiology, histopathology, clinical presentation, diagnosis and management. Bol. Asoc. Med. P. R. 88:46-51. [PubMed]
82. 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. [PubMed]
83. 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]
84. Reed, J. B., D. K. Scales, M. T. Wong, C. P. Lattuada, M. J. Dolan, and I. R. Schwab. 1998. Bartonella henselae neuroretinitis in cat scratch disease. Ophthalmology 105:459-466. [PubMed]
85. Regnery, R. L., J. A. Rooney, A. M. Johnson, S. L. Nesby, P. Manzewitsch, K. Beaver, and J. G. Olson. 1996. Experimentally induced Bartonella henselae infections followed by challenge exposure and antimicrobial therapy in cats. Am. J. Vet. Res. 57:1714-1719. [PubMed]
86. Resto-Ruiz, S., A. Burgess, and B. E. Anderson. 2003. The role of the host immune response in pathogenesis of Bartonella henselae. DNA Cell Biol. 22:431-440. [PubMed]
87. Rolain, J. M., C. Foucault, R. Guieu, B. La Scola, P. Brouqui, and D. Raoult. 2002. Bartonella quintana in human erythrocytes. Lancet 360:226-228. [PubMed]
88. Rolain, J. M., B. La Scola, Z. Liang, B. Davoust, and D. Raoult. 2001. Immunofluorescent detection of intraerythrocytic Bartonella henselae in naturally infected cats. J. Clin. Microbiol. 39:2978-2980. [PMC free article] [PubMed]
89. Rolain, J. M., M. Maurin, A. Bryskier, and D. Raoult. 2000. In vitro activities of telithromycin (HMR 3647) against Rickettsia rickettsii, Rickettsia conorii, Rickettsia africae, Rickettsia typhi, Rickettsia prowasekii, Coxiella burnetii, Bartonella henselae, Bartonella quintana, Bartonella bacilliformis, and Ehrlichia chaffeensis. Antimicrob. Agents Chemother. 44:1391-1393. [PMC free article] [PubMed]
90. Rolain, J. M., M. Maurin, M. N. Mallet, D. Parzy, and D. Raoult. 2003. Culture and antibiotic susceptibility of Bartonella quintana in human erythrocytes. Antimicrob. Agents Chemother. 47:614-619. [PMC free article] [PubMed]
91. Rolain, J. M., M. Maurin, and D. Raoult. 2000. Bactericidal effect of antibiotics on Bartonella and Brucella spp.: clinical implications. J. Antimicrob. Chemother. 46:811-814. [PubMed]
92. 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]
93. Schulein, R., A. Seubert, C. Gille, C. Lanz, Y. Hansmann, Y. Piemont, and C. Dehio. 2001. Invasion and persistent intracellular colonization of erythrocytes. A unique parasitic strategy of the emerging pathogen Bartonella. J. Exp. Med. 193:1077-1086. [PMC free article] [PubMed]
94. Schultz, M. G. 1968. A history of bartonellosis (Carrion's disease). Am. J. Trop. Med. Hyg. 17:503-515. [PubMed]
95. Schultz, M. G. 1968. Daniel Carrion's experiment. N. Engl. J. Med. 278:1323-1326. [PubMed]
96. Slater, L. N., D. F. Welch, D. Hensel, and D. W. Coody. 1990. A newly recognized fastidious gram-negative pathogen as a cause of fever and bacteremia. N. Engl. J. Med. 323:1587-1593. [PubMed]
97. Sobraques, M., M. Maurin, R. Birtles, and D. Raoult. 1999. In vitro susceptibilities of four Bartonella bacilliformis strains to 30 antibiotic compounds. Antimicrob. Agents Chemother. 43:2090-2092. [PMC free article] [PubMed]
98. 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]
99. Spach, D. H., A. S. Kanter, N. A. Daniels, D. J. Nowowiejski, A. M. Larson, R. A. Schmidt, B. Swaminathan, and D. J. Brenner. 1995. Bartonella (Rochalimaea) species as a cause of apparent “culture-negative” endocarditis. Clin. Infect. Dis. 20:1044-1047. [PubMed]
100. Spach, D. H., A. S. Kanter, M. J. Dougherty, A. M. Larson, M. B. Coyle, D. J. Brenner, B. Swaminathan, G. M. Matar, D. F. Welch, R. K. Root, and W. E. Stamm. 1995. Bartonella (Rochalimaea) quintana bacteremia in inner-city patients with chronic alcoholism. N. Engl. J. Med. 332:424-428. [PubMed]
101. Spaulding, W. B., and J. N. Hennessy. 1960. Cat scratch disease. A study of eighty-three cases. Am. J. Med. 28:504-509. [PubMed]
102. Stoler, M. H., T. A. Bonfiglio, R. T. Steigbigel, and M. Pereira. 1983. An atypical subcutaneous infection associated with acquired immune deficiency syndrome. Am. J. Clin. Pathol. 80:714-718. [PubMed]
103. Szaniawski, W. K., P. C. Don, S. R. Bitterman, and J. R. Schachner. 1990. Epithelioid angiomatosis in patients with AIDS: a report of seven cases and review of the literature. J. Am. Acad. Dermatol. 23:41-48. [PubMed]
104. Tappero, J. W., and J. E. Koehler. 1991. Cat scratch disease and bacillary angiomatosis. JAMA 266:1938-1939. [PubMed]
105. Tappero, J. W., J. E. Koehler, T. G. Berger, C. J. Cockerell, T. H. Lee, M. P. Busch, D. P. Stites, J. C. Mohle-Boetani, A. L. Reingold, and P. E. LeBoit. 1993. Bacillary angiomatosis and bacillary splenitis in immunocompetent adults. Ann. Intern. Med. 118:363-365. [PubMed]
106. Uertega, O., and E. H. Payne. 1955. Treatment of the acute febrile phase of Carrion's disease with chloramphenicol. Am. J. Trop. Med. Hyg. 4:507-511. [PubMed]
107. Welch, D., K. Carrol, E. Hofmeister, D. Persing, D. Robison, A. Steigerwalt, and D. 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]
108. Wong, M. T., M. J. Dolan, C. P. Lattuada, Jr., R. L. Regnery, M. L. Garcia, E. C. Mokulis, R. C. Labarre, D. P. Ascher, J. A. Delmar, J. W. Kelly, D. R. Leigh, A. C. Mcrae, J. B. Reed, R. E. Smith, and G. P. Melcher. 1995. Neuroretinitis, aseptic meningitis, and lymphadenitis associated with Bartonella (Rochalimaea) henselae infection in immunocompetent patients and patients infected with human immunodeficiency virus type 1. Clin. Infect. Dis. 21:352-360. [PubMed]
109. Zeaiter, Z., P. E. Fournier, and D. Raoult. 2002. Genomic variation of Bartonella henselae strains detected in lymph nodes of patients with cat scratch disease. J. Clin. Microbiol. 40:1023-1030. [PMC free article] [PubMed]

Articles from Antimicrobial Agents and Chemotherapy are provided here courtesy of American Society for Microbiology (ASM)