Search tips
Search criteria 


Logo of cmrPermissionsJournals.ASM.orgJournalCMR ArticleJournal InfoAuthorsReviewers
Clin Microbiol Rev. 2009 July; 22(3): 387–395.
PMCID: PMC2708393

Antibiotic Treatment of Animals Infected with Borrelia burgdorferi


Summary: Despite resolution of the objective manifestations of Lyme disease after antibiotic treatment, a minority of patients have fatigue, musculoskeletal pain, and/or difficulties with concentration or short-term memory of uncertain etiology; these are called post-Lyme disease symptoms or, in more severe cases, post-Lyme disease syndrome or “chronic Lyme disease.” Several recent studies in which Borrelia burgdorferi-infected animals were treated with antibiotic therapy have demonstrated the presence of PCR positivity for B. burgdorferi DNA in the absence of culture positivity. In mice that were treated with antibiotic therapy, residual spirochetes could be taken up by ticks during a blood meal and could be transmitted to SCID mice. These spirochetes are attenuated; their presence is not associated with either inflammation or disease. In this review the methodology and findings of these studies are critically analyzed, and the significance of the results with regard to human Lyme disease is evaluated, with special emphasis on whether these studies provide useful insights into post-Lyme disease syndrome. A serious methodological concern is the failure to consider the pharmacokinetic-pharmacodynamic properties of the antibiotic in choosing the dosage regimen used. We conclude that there is no scientific evidence to support the hypothesis that such spirochetes, should they exist in humans, are the cause of post-Lyme disease syndrome.


Lyme disease is the most common tick-borne infection in North America. Objective clinical manifestations may involve the skin, nervous system, heart, or joints, all of which usually respond well to conventional antibiotic therapy (52). Despite resolution of the objective manifestations of infection after antibiotic treatment, a minority of patients have fatigue, musculoskeletal pain, and/or difficulties with concentration or short-term memory of uncertain etiology (13). Subjective complaints that persist are referred to as post-Lyme disease symptoms; if they persist for >6 months and cause functional impairment they are often referred to as post-Lyme disease syndrome (13, 26, 52). Post-Lyme disease syndrome is sometimes referred to as “chronic Lyme disease,” but this term is poorly defined and is often used to refer to chronic symptoms that are unrelated to Borrelia burgdorferi infection (13, 16). Although post-Lyme disease syndrome is a topic of considerable interest and controversy, it is important to point out that the principal evidence in support of the existence of this syndrome is derived from older retrospective studies in which the diagnosis and treatment of Lyme disease would not meet current standards (10, 45). No prospective treatment study of patients with Lyme disease has been published to prove or disprove that the frequency of such nonspecific symptoms at 6 or 12 months after antibiotic treatment actually exceeds that of the same types of symptoms in individuals without Lyme disease (16, 45). There is also no convincing evidence that post-Lyme disease syndrome will resolve following additional courses of antibiotic therapy (13, 26, 52).

The purpose of this review is to describe the methodology and findings of recently published treatment studies of experimental animals that were infected with B. burgdorferi and to evaluate the significance of the results with regard to human Lyme disease. Special emphasis is placed on whether these studies provide any useful insights into posttreatment Lyme disease symptoms and/or post-Lyme disease syndrome. Possible future approaches for clarifying the outstanding questions are discussed.


Studies of the effects of antibiotic therapy in animals infected with B. burgdorferi have been conducted most often with mice (8, 18, 25, 30, 31, 35, 38, 53, 54) but also with hamsters (21, 22), gerbils (15, 32, 42), dogs (48, 49), and nonhuman primates (39). In most of the studies the animals were immunocompetent, but in several the animals were immunocompromised (25, 37, 48). The criteria for judging that the outcome of treatment was successful varied among the studies. In the initial studies, outcome was based on whether B. burgdorferi could be recovered on culture, a straightforward approach widely used with other infectious agents that are cultivable. In more recent studies, detection of DNA of B. burgdorferi (8, 18, 30, 35, 48, 49, 54), visualization of the spirochete in tissues by immunohistochemistry (18), xenodiagnosis (detection of B. burgdorferi in ticks that had fed on an infected animal) (8, 18), transplantation of tissues from B. burgdorferi-infected animals to uninfected animals (8, 18), or other outcome measures were employed, in addition to culture. Judging of outcomes based on so many diverse parameters and imposition of such stringent criteria for therapeutic success appear to be somewhat unique to experimental infection due to B. burgdorferi. The justification for adopting this approach may have been the presumption that either a local inflammatory response or a vigorous generalized immune response to the spirochete or some residual antigen(s) is responsible for posttreatment Lyme disease symptoms and/or post-Lyme disease syndrome (13, 26, 52).

In the treatment of other infections it is probably unrealistic to expect that antimicrobial therapy per se will eliminate every single microorganism from an infected host, and moreover, such an action would rarely if ever be required for a successful outcome. More conventionally, the role of antimicrobial therapy in vivo can be thought of in terms of “tipping the balance” in favor of the host's own defenses against a particular pathogen. Indeed, for most infections treatment with antibiotics that only inhibit rather than kill a microorganism is just as effective as treatment with bactericidal agents (36).


Study by Hodzic et al.

Cultures and PCR.

Hodzic et al. (18) reported on a series of experiments in which they compared therapy with ceftriaxone (administered intraperitoneally) versus saline in C3H/HeN mice that were infected by needle inoculation with an N40 strain of B. burgdorferi (Table (Table1).1). Although it was demonstrated that as few as a single spirochete could be detected by the culture methodology employed, in antibiotic-treated animals cultures of multiple tissue sites were consistently negative, regardless of whether the animals had been treated early (3 weeks after infection) or late (4 months after infection). There was a single instance of allograft transmission by an antibiotic-treated mouse to an immunocompetent mouse, but this observation appeared to be aberrant, since at that time point none of allografts from the sham-treated mice transmitted infection to the recipient mice.

Study methodologies employed

Despite the absence of positive cultures, DNA of B. burgdorferi could be detected by PCR in some of the ceftriaxone-treated mice. PCR positivity was present principally at the base of the heart and in the tibiotarsus tissue and not in tissue from the ear, inoculation site for B. burgdorferi, subinoculation site, ventricle, or quadriceps muscle (18). Uninfected control mice were not studied. To determine if B. burgdorferi could be recovered from the tissues with a positive PCR result, a confirmatory experiment was done in which these tissues were cultured, in addition to urinary bladder, ear, and inoculation site, but these cultures were also sterile. The prevalence of mice that were PCR positive was higher following antibiotic therapy at 4 months than following therapy at 3 weeks after the onset of infection (10/13 versus 2/8; P = 0.03). Hodzic et al. (18) stated that they were unsuccessful in detection of RNA transcription despite attempts to amplify cDNA, but they did not provide any details.

Spirochetes diminish over time.

Although it was not emphasized by the investigators, mice were more likely to be PCR positive and to have a larger number of flaB DNA copies/mg tissue shortly after completion of ceftriaxone treatment than at a later time point, suggesting that the presence of spirochetal DNA was decreasing over time for reasons not elucidated. For example, in the mice treated at 4 months after infection, B. burgdorferi DNA was detected by PCR in eight (100%) of eight mice that were evaluated at 1 month after completion of antibiotic therapy, compared with two (40%) of five mice that were evaluated at 3 months after completion of antibiotic treatment (P = 0.03). PCR-positive samples from mice at 1 month after treatment contained 33.7 ± 60.6 (mean ± standard deviation) flaB DNA copies/mg tissue, compared with 4.1 and 2.8 flaB DNA copies/mg in the two positive samples from mice at 3 months after treatment. Furthermore, spirochetes were visualized at the base of the heart or in tibiotarsus tissue by immunohistochemistry (using rabbit immune serum to B. burgdorferi) in three (37.5%) of eight mice at 1 month posttreatment, compared with one (20%) of five mice at the 3-month posttreatment time point. There was, however, no histologic evidence for inflammation at these or any other tissue sites in these animals (S. Barthold, personal communication, 2009). Serum antibody reactivity to B. burgdorferi whole-cell antigen extract declined significantly in antibiotic- compared to saline-treated mice but did not return to preinfection levels (18). This finding was consistent with the reduction in spirochetes that was documented in antibiotic- versus saline-treated animals.

The normal-appearing morphology of the spirochetes visualized histologically posttreatment implies that the borrelial DNA that was detected by PCR was unlikely to be entirely free DNA in tissues. An intraspirochetal location, even if the spirochete was damaged or attenuated, likely accounts for why B. burgdorferi DNA could be detected for at least 90 days after treatment in the study by Hodzic et al. (18). The microscopic findings do not provide support, however, for the theory that B. burgdorferi persists through the formation of cysts (3).

Xenodiagnosis and transmission of Borrelia burgdorferi by ticks following xenodiagnosis.

Of the 23 mice in total that were treated with ceftriaxone at 4 months after onset of infection in the study by Hodzic et al. (18), 11 (47.8%) had a positive xenodiagnosis (i.e., B. burgdorferi was detected by PCR in Ixodes ticks that fed on these mice). In an experiment that attempted to quantitate the number of spirochetes, the number of flaB DNA copies per tick was 120.6 ± 75.1 in the nymphal stages of those ticks that had fed on antibiotic-treated mice during the larval stage, compared to 35,747 ± 40,705 flaB DNA copies in positive ticks from saline-treated mice. B. burgdorferi could not be cultured from PCR-positive ticks that had fed on antibiotic-treated mice but could be cultured from ticks that had fed on saline-treated mice.

Ticks that had fed on antibiotic-treated mice were subsequently fed on highly immunodeficient (C3H-scid) mice (18). For unstated reasons, ticks were not fed on immunocompetent mice. Although essentially none of the SCID mice became culture positive (based on cultures of the urinary bladder, ear, and inoculation site), B. burgdorferi DNA was detected in one or more tissue sites of these mice, excluding the site of the tick bite (18). None of the SCID mouse tissues, however, showed histologic evidence of inflammation. This was a surprising finding because this strain of mouse (which is deficient in both humoral and cellular acquired immunity) is highly susceptible to infection with B. burgdorferi and would have been expected to develop prominent signs of inflammation. Excluding one tissue sample that was an outlier, the copy number of flaB DNA in the tissue samples from the SCID mice averaged 656.2/mg. Based on a prior study of SCID mice by some of the same investigators (17), >40,000 flaB copies/mg of tissue might have been expected, although this comparison may not be entirely appropriate because B. burgdorferi was introduced by needle inoculation in the earlier investigation rather than by tick bite. Whether spirochetes could be visualized by immunohistochemistry in the SCID mice was not stated. Although the investigators mentioned that they attempted allograft transmission to SCID mice, the results were not reported in the paper.

Conclusions of the investigators in the study by Hodzic et al.

Hodzic et al. (18) concluded that viable but not cultivable spirochetes persisted after antibiotic treatment in this animal system.

Failure to consider pharmacodynamics of antibiotic therapy is a methodological concern in the study by Hodzic et al.

A serious methodological concern pertinent to the study by Hodzic et al. (18) and many of the other animal studies evaluating antibiotic treatment of B. burgdorferi infection is the failure to consider adequately the pharmacokinetic-pharmacodynamic properties of the antibiotic regimen used. Both in vitro and in vivo data demonstrate that the time that β-lactam antibiotics are maintained at or above the MIC for the infecting strain of B. burgdorferi (“time over MIC” [T/MIC]) is the key pharmacodynamic parameter governing the activity of this class of antibiotics against this microorganism (29, 31, 41, 51, 52). In view of the much shorter half-life of ceftriaxone in C3H mice than in humans, one or two daily doses of ceftriaxone in mice falls far short of the T/MIC that occurs in humans (Table (Table2)2) (18, 37, 38, 52).

Selected pharmacokinetic-pharmacodynamic parameters of ceftriaxone and doxycycline in mice and humans

Whether the same observations would have been made had the ceftriaxone dosing been administered in a manner that would have faithfully recapitulated the T/MIC seen in humans is unknown. If one of the antimicrobial effects of ceftriaxone is to attenuate B. burgdorferi and render it incapable of causing disease, but not completely eliminate it, would the same biologic event occur if ceftriaxone was given for a much shorter period of time, even just 24 h (38)? Is such attenuation reversible? Would doxycycline treatment have had a different effect on B. burgdorferi than ceftriaxone treatment, in view of the completely unrelated mechanisms of action of the two drugs?

Study by Bockenstedt et al.

Antibiotic dosing and pharmacokinetic-pharmacodynamic considerations.

Some, but not all of these questions, were answered in a study reported several years earlier by Bockenstedt et al. (8). In contrast to the study by Hodzic et al. (18), C3H/HeJ mice in the study by Bockenstedt et al. were infected with an N40 strain of B. burgdorferi mice by an Ixodes tick bite rather than by needle inoculation (Table (Table1).1). At 30 days after infection, mice were treated with either ceftriaxone (by subcutaneous administration) or doxycycline (by gavage) for 30 days. Unlike in the study by Hodzic et al. (18), antibiotic doses were adjusted for age-related weight gain (8). However, Bockenstedt et al. (8) similarly ignored the much shorter half-lives of these antibiotics in mice than in humans and failed to replicate the antibiotic exposure to either drug that occurs in humans (Table (Table2)2) (4, 37, 44). The pharmacokinetic-pharmacodynamic parameter that correlates best with the efficacy of doxycycline for the treatment of infections due to other microorganisms is the area under the time-concentration curve of free drug (i.e., drug not bound to protein) divided by the MIC (4), and limited data suggest that this is also true for infection due to B. burgdorferi (27).

In a much earlier study, 60% of B. burgdorferi-infected mice remained culture positive despite treatment with a 2-week course of doxycycline at a dose of 13 mg/kg twice daily (31). Cognizant of these results and that of a treatment study of Brucella infection in mice (12), Bockenstedt et al. increased the dose of doxycycline to 50 mg/kg twice daily (8). The MIC of doxycycline for the N40 strain of B. burgdorferi used by Bockenstedt et al. has not been reported, but for other strains of B. burgdorferi, MICs of doxycycline are typically 4- to >10-fold higher than the 0.06-μg/ml MIC of doxycycline for the strain of Brucella melitensis in the study relied upon by Bockenstedt et al. (19, 23). Furthermore, 100% of the mice were cured of the Brucella infection with a 45-day course of doxycycline (50 mg/kg twice daily), whereas a 21-day course of therapy was less effective and a 30-day course of treatment was not attempted (12). These discrepancies raise concerns about the appropriateness of the dose and duration of doxycycline employed in the study by Bockenstedt et al.

Cultures, PCR, and xenodiagnosis.

In contrast to the case for sham-treated mice, antibiotic-treated mice in the study by Bockenstedt et al. did not have either a positive culture of blood, ear, heart, spleen, or urinary bladder or histologic evidence of arthritis or carditis (8). There was evidence by PCR of persistent B. burgdorferi DNA in mouse tissues (heart, bladder, or joint), however, until study completion at 9 months after doxycycline treatment in at least four of five mice, particularly in joint tissue; in contrast, PCR positivity (at the “lower detection limit of the assay”) was found only in urinary bladder tissue and only in two of four mice that were treated with ceftriaxone. Uninfected control mice were PCR negative. Although the spirochete could be detected in ticks by xenodiagnosis for up to 3 months after antibiotic therapy, such testing was negative at 6 months in both the antibiotic- and saline-treated mice. Xenopositivity for ticks at 9 months after treatment, however, did occur if the mice were first immunosuppressed with corticosteroids, but only for the ticks that fed on saline-treated mice, not for those that fed on antibiotic-treated animals. In the study by Hodzic et al. (18), xenodiagnosis was attempted only up to 3 months after completion of treatment; thus, the study by Bockenstedt et al. should not be assumed to contradict the study by Hodzic et al. on this point (Table (Table11).

After larval stage ticks that had fed on infected mice had molted to the nymphal stage in the study by Bockenstedt et al., they were no longer PCR positive and did not transmit infection to uninfected C3H mice (based on the absence of seroconversion in these mice) (8). No attempt was made to culture B. burgdorferi from PCR-positive ticks. Importantly, Bockenstedt et al. (8) noted that a similar proportion of antibiotic-treated mice had evidence of persistent infection based on xenodiagnostic studies in an earlier experiment in which ceftriaxone or doxycycline was given for just 2 weeks rather than 4 weeks.

Allotransplantation and serology.

Bockenstedt et al. (8) also stated (without providing data) that they were unable to transmit infection from antibiotic-treated mice to SCID mice by allotransplantation, an experiment that was omitted in the study by Hodzic et al. (Table (Table1)1) (18). Antibiotic therapy led to a rapid decline in anti-B. burgdorferi whole-cell lysate antibody titers, but levels were still elevated through 9 months; titers were indistinguishable between mice that tested positive by xenodiagnosis and those that did not test positive. Over the 11-month experimental period, antibody titers also declined in the saline-treated group of infected mice, although they remained at significantly higher levels than in the antibiotic-treated mice.

Conclusions and comparisons with the study by Hodzic et al.

In contrast to Hodzic et al. (18), Bockenstedt et al. (8) concluded that “residual” spirochetes are avirulent and will eventually die or be killed by the host without causing disease. There are numerous methodological differences between the studies by Hodzic et al. and Bockenstedt et al. (Table (Table1).1). The latter investigation employed C3H/HeJ mice (which have a mutation in Toll-like receptor 4 [40]) as opposed to C3H/HeN mice; mice were treated only at 30 days postinfection (rather than at 3 weeks and 4 months postinfection by Hodzic et al. [18]); xenodiagnosis was performed at 1, 3, 6, and 9 months (it was done only at 1 and 3 months in the study by Hodzic et al.); and refeeding of xenodiagnostic ticks was performed with C3H mice as opposed to SCID mice. Whether these methodological differences account for all of the discrepancies between the two studies is not clear.


Straubinger et al. (47-49) studied the efficacy of a 30-day course of amoxicillin (amoxicilline) (oral), doxycycline (oral), ceftriaxone (intravenous), or azithromycin (oral) for the treatment of dogs that were infected with B. burgdorferi by tick feeding using field-collected ticks. Their results are in general agreement with those of Hodzic et al. (18) and Bockenstedt et al. (8) in that they showed that the dogs were more likely to be PCR positive than culture positive after antibiotic treatment. PCR positivity persisted for up to 455 days after the conclusion of antibiotic therapy (47). Like the mice in the studies discussed above, antibiotic-treated dogs usually remained well without development of objective clinical disease. This remained true even when the animals were immunosuppressed with corticosteroids.

In the first treatment study reported by Straubinger et al. (49), 3 (27.3%) of 11 dogs that were treated with either doxycycline or amoxicillin starting at approximately 60 days after tick exposure had a positive culture for B. burgdorferi posttreatment. In a second study by these investigators (48), none of four dogs that were treated with the same dose of doxycycline at 120 days after tick exposure were culture positive, nor were any of the dogs that were treated with azithromycin (n = 4) or ceftriaxone (n = 4). The larger number of culture-positive dogs in the earlier study might have been a chance event or due to a greater burden of spirochetes at the 60- versus 120-day time point. However, for unclear reasons the doxycycline blood levels reported in the second study were considerably higher than those that were found in the first study. Thus, it is tempting to speculate that the higher culture positivity rate in the first study was due to insufficient antibiotic treatment. Similarly, it is of interest that in the first study by Straubinger et al. (49), the single culture-positive dog that received amoxicillin (one of five infected dogs treated with amoxicillin was culture positive) was one of the two dogs that were treated with twice-daily dosing of amoxicillin; the other three dogs were treated with three doses per day.

The studies by Straubinger et al. (47-49) potentially add important clarifications to the mouse experiments discussed above (8, 18). First, they show that PCR positivity in the absence of culture positivity may occur in dogs as well as C3H mice. Second, the results indicate that this phenomenon can also occur after antibiotic treatment with either amoxicillin or azithromycin. Third, the results demonstrate that this phenomenon is not restricted to either the N40 strain of B. burgdorferi or even to a laboratory strain of the spirochete. Last, the exposure of the dogs to doxycycline or azithromycin in the second treatment trial conducted by these investigators (48) seemed more comparable to that seen in humans, suggesting that the reason for persistence of B. burgdorferi DNA is not necessarily improper dosing of the antimicrobial. The studies by Straubinger et al., however, documented a high degree of variability in antibiotic levels in blood specimens of different animals receiving the same dosage regimen. For example, in the first study in which the efficacy of doxycycline was compared with amoxicillin (49), antibiotic levels were assessed at multiple time points for four dogs that were treated with doxycycline and for four other dogs that received amoxicillin. Considerable variability (up to twofold or greater) in drug levels was observed between the dog with the highest drug level and the one with the lowest level for each of the antibiotics. Variability in drug levels between animals was not investigated in the mouse studies performed by either Hodzic et al. (18) or Bockenstedt et al. (8).

It is noteworthy that in untreated dogs more tissue samples were positive by culture than by PCR, in contrast to what was observed in antibiotic-treated animals. In one of the studies by Straubinger et al. (47, 48), PCR positivity after antibiotic treatment was so infrequent and at such a low level quantitatively as to raise the concern that the results were due to amplicon contamination or to a stochastic (random) process, or both. For example, among the four ceftriaxone-treated dogs, only 3 (5.0%) of 60 skin biopsy samples obtained during or after antibiotic treatment were PCR positive and only 1 (1.0%) of 100 tissues obtained postmortem was PCR positive. In the single dog with two positive PCR results, PCR was negative for 3 months after completion of antibiotic therapy, a single sample was PCR positive at 4 months, PCR was negative from month 5 to 12, and PCR was positive again at 13 months. The use of a single uninfected control dog in this experiment was insufficient to exclude the possibility of either low-level contamination or a stochastic event.


PCR has been employed as a measure of outcome in several other treatment studies of B. burgdorferi-infected animals. In studies by Yrjanainen et al. (54) and by Malawista et al. (30), mice were treated with a 5-day course of ceftriaxone. In neither of these studies did the investigators observe PCR positivity in the absence of culture positivity. However, in the study by Yrjanainen et al. (54), PCR was applied only to urinary bladder tissue and in the study by Malawista et al. (30), it was applied only to urinary bladder and ear tissue. Conceivably, there would have been a disproportionately higher rate of PCR versus culture positivity if tissue specimens from the base of the heart or tibiotarsal area had been evaluated. Yrjanainen et al. (54) raised the question of whether administration of an antibody to tumor necrosis factor alpha (TNF-α) might reactivate B. burgdorferi infection and restore culture positivity. The rationale for why this should occur in B. burgdorferi infection, which is a distinctly different kind of infection from mycobacterial or fungal infections, which are known to be reactivated by TNF-α inhibitors (50), was not made clear in the report. It is also unclear why TNF-α inhibition should reactivate B. burgdorferi when treatment with corticosteroids (38, 48) or transmission to SCID mice (18) in other studies did not. Furthermore, the frequency of culture-positive animals was not significantly different in those mice that were treated with anti-TNF-α and those not receiving this agent, implying that the higher rate of culture positivity in the mice receiving anti-TNF-α might have been a chance event (51).

In a study by Pahl et al. (35), B. burgdorferi-infected mice were treated with a subcurative dose of penicillin G given subcutaneously twice daily for 14 days starting on day 8 after infection. This dose did not eliminate the spirochete, and the differences in numbers of spirochetes in tissue based on PCR in favor of treatment versus control animals vanished by 4 weeks after completion of antibiotic therapy. Although details were not provided, the investigators indicated that B. burgdorferi could be cultured from PCR-positive tissues.

In a study of B. burgdorferi-infected mice, Pavia et al. (38) observed that administration of five daily doses of ceftriaxone was associated with negative cultures of urinary bladder and ear tissue, irrespective of whether the mice were concomitantly treated with corticosteroids. Similarly, Kazragis et al. (25) found consistently negative cultures for B. burgdorferi in SCID mice with B. burgdorferi infection that were treated with a 9-day course of ceftriaxone. Neither of these studies, however, evaluated PCR positivity or xenodiagnosis. These studies do, however, raise the question of whether the outcome of ceftriaxone therapy of infected animals would be the same with courses of antibiotic therapy much shorter than 30 days in duration.

Table Table33 provides a brief summary of the principal findings for the treatment studies of animals infected with B. burgdorferi discussed above.

Summary of the principal findings of selected treatment studies of animals infected with Borrelia burgdorferi


The following are outstanding questions regarding the phenomenon of PCR positivity without culture positivity after antibiotic treatment of experimental animals with B. burgdorferi infection.

  1. Does the duration of treatment affect the development of PCR positivity in the absence of culture positivity? What is the shortest duration of treatment possible?
  2. Do pharmacodynamic considerations such as total daily antibiotic exposure affect the development of PCR positivity in the absence of culture positivity?
  3. What are causes of the attenuation of the spirochetes that persist posttreatment? Are they in the process of dying? Are they producing mRNA, and if so, which mRNA? Are they motile? Can they replicate? Are they genetically altered? Can they regain pathogenicity?
  4. Does development of PCR positivity in the absence of culture positivity occur in SCID mice that are treated with antibiotic therapy; i.e., does the process occur independently of an adaptive immune response?
  5. Is PCR positivity reduced over time in SCID mice; i.e., does PCR positivity resolve spontaneously due to the death of damaged spirochetes?

For mice there is solid evidence for a reduction in the rates of posttreatment PCR positivity and xenopositivity over the course of time. Is this due to clearance of the spirochete by the host's immune response, or is it due to the death of irreversibly damaged spirochetes, or both? This question could be addressed by sequential evaluation of SCID mice that were infected with attenuated spirochetes as described in the study by Hodzic et al. (18).


Does the phenomenon of PCR positivity without culture positivity imply viability of B. burgdorferi? Determination of whether bacterial cells are alive or dead is often challenging. It is an important question not only as it relates to the effects of antibiotics in an infected human or animal but also in terms of food safety and sterility of pharmaceutical products and implantable prosthetic devices (5, 6, 9, 11). The most straightforward confirmation of viability is demonstration of cell division. The “viable but not cultivable hypothesis” (for microorganisms that are initially cultivable) posits that bacterial cells have differentiated into a long-term survival state, rather than having degenerated into an injured state to be followed by an inexorable further deterioration to death (9, 34, 43). Demonstration of the presumed viability of bacteria other than borreliae that have become noncultivable has generally relied on the use of nucleic acid stains, redox indicators, membrane potential probes, flow cytometry, and reporter gene systems and on demonstration of the ability of the bacterial cell to take up amino acids or sugars, synthesize protein, synthesize mRNA, or manifest respiration (6, 9). The validity of such methods is controversial, in part because such reactions might transiently be observed in injured cells, making the timing of the testing a critical variable (6, 9). Unequivocal proof of the viable but noncultivable hypothesis for bacteria has generally rested upon restoration of cultivability, even in circumstances in which the organism is first passed through an animal system (6, 9). Antibiotic treatment of animals with B. burgdorferi infection clearly differs from the classic description of bacterial “persisters” that can be demonstrated following exposure to certain antibiotics in vitro, since in the latter situation reversion back to regular cells with regrowth occurs when the antibiotic levels drop (7, 28).

Evidence that PCR positivity in mice treated for B. burgdorferi infection is due to viable but noncultivable spirochetes is based principally on a single experiment in which xenodiagnostic ticks transmitted the spirochete to SCID mice and then the spirochete disseminated to presumably extravascular tissue sites distant from the inoculation site (18). Whether the acquisition of spirochetes by xenodiagnostic ticks per se implies viability is unknown. If active motility on the part of the spirochete is required, then acquisition of the spirochete by a tick would imply viability. If spirochetes were viable after antibiotic treatment in the experiments performed by Hodzic et al. (18), Bockenstedt et al. (8), and Straubinger et al. (47-49), they clearly were attenuated. Was the attenuation due to irreversible spirochetal injury? If so, what is the nature of the damage? The loss of certain key genes was suggested by Bockenstedt et al. (8) but could not be confirmed in the study by Hodzic et al. (18).


Does the phenomenon of PCR positivity without culture positivity observed in animals after antibiotic treatment also occur in humans treated for Lyme disease, and if so, has it been detected and does it have any relevance to the presence of clinical disease or symptoms? Given the propensity of B. burgdorferi to localize over time in collagen-rich tissues of mice, including joints and tendons (18), investigation of patients with Lyme arthritis might provide insights into the existence of this phenomenon in humans. Indeed, rates of PCR positivity in synovial fluid specimens of untreated patients with Lyme arthritis may be as high as 96% (33). In contrast to the animal studies discussed above, however, the yield of culture for B. burgdorferi of synovial fluid specimens of untreated patients with Lyme arthritis is close to zero (2, 33). Therefore, Lyme arthritis is not a satisfactory model to evaluate whether antibiotic treatment per se induces culture negativity despite continued PCR positivity.

Most patients with Lyme arthritis respond well to a 4-week course of oral antibiotic therapy (52), and PCR testing cannot be carried out after therapy because affected joints are no longer swollen. However, a small subgroup of patients have persistent synovitis for months or even several years after treatment for ≥2 months with oral antibiotics or for ≥1 month with intravenous antibiotics, or usually after both types of therapy, a condition which is referred to as antibiotic-refractory Lyme arthritis. Antibody responses to B. burgdorferi antigens decline similarly in patients with antibiotic-responsive or antibiotic-refractory arthritis, suggesting that spirochetal killing occurs in both groups (24). Because joint inflammation persists for months after antibiotic treatment, it provides an opportunity to assess the duration of PCR positivity after antibiotic therapy. Of 34 patients with antibiotic-refractory arthritis for whom joint fluid was available after antibiotic therapy, only 2 (6%) had a positive PCR result after 4 to 5 months, and just 1 still had a weakly positive result at 6 months (46). No one had a positive result after the 6-month time point. Thus, B. burgdorferi DNA may rarely persist in the joints of patients with Lyme arthritis for several months after recommended treatment with oral and/or intravenous antibiotics (52), but it eventually disappears.

The duration of PCR positivity in urine samples of patients with early Lyme disease associated with erythema migrans has also been evaluated. In one such European study, PCR positivity persisted in the urine for 12 months after antibiotic treatment in 8% of cases (1); cultures were not reported. The amplicons were not sequenced in that study, a potentially important omission since PCR testing for B. burgdorferi DNA in urine specimens has been associated with false-positive results (1, 2).

Could the phenomenon of PCR positivity for B. burgdorferi DNA in the absence of culture positivity after antibiotic therapy provide an explanation for post-Lyme disease syndrome, as suggested by Hodzic et al. (18)? This seems highly unlikely. Clearly the B. burgdorferi cells remaining in animals after antibiotic treatment are biologically different from those in untreated animals. Most importantly, their presence does not elicit a local inflammatory response in mice or dogs, even when the animals are immunocompromised (8, 18, 48). In addition, the decline in antibody response to B. burgdorferi in animals after treatment suggests a reduction in the overall immunologic response to the spirochete (39). Since there is no convincing evidence that B. burgdorferi is capable of elaborating a systemic toxin (14), it is difficult to imagine how residual spirochetes in the absence of a detectable local or generalized immunologic or inflammatory response by the host could lead to chronic subjective symptoms.


In conclusion, a number of recent studies in which B. burgdorferi-infected animals were treated with antibiotic therapy have demonstrated the presence of PCR positivity in the absence of culture positivity (Table (Table3)3) (8, 18, 48, 49). A serious methodological concern with most of these studies is the failure to consider adequately the pharmacokinetic-pharmacodynamic properties of the antibiotic in choosing the dosage regimen used. In mice that have been treated with antibiotic therapy, residual spirochetes can be taken up by ticks during a blood meal (8, 18), at least for the first several months after treatment, and can be transmitted to SCID mice (18). The biological nature of these spirochetes is unclear. Evidence indicates that they are nonpathogenic. Whether the lack of pathogenicity is simply related to low numbers of residual spirochetes or is due to a more fundamental genotypic or phenotypic alteration is unknown. It is also unknown whether the lack of pathogenicity is irreversible. Since in the mouse studies the number of spirochetes is declining over time, a reasonable conjecture is that they are in the process of dying. There is no scientific evidence to support the hypothesis that such spirochetes, should they exist in humans, are the cause of post-Lyme disease syndrome.


We thank Mario T. Philipp, Stephen Barthold, Linda Bockenstedt, Lisa Giarratano, and Lenise Banwarie for their assistance.

Some studies conducted in our laboratories were supported in part by National Institutes of Health grants AR41511 and AI45801.


An external file that holds a picture, illustration, etc.
Object name is zcm0030922820001.jpg Gary P. Wormser (M.D.) is Chief of the Division of Infectious Diseases and Vice Chairman of the Department of Medicine at New York Medical College. He is Professor of Medicine and Pharmacology. At Westchester Medical Center, Dr. Wormser is Chief of the Section of Infectious Diseases. He is Director and Founder of the Walk-in Lyme Disease Practice for the care and study of patients with tick-borne infections. Dr. Wormser received his B.A. from the University of Pennsylvania (magna cum laude), majoring in mathematics, and his medical degree from the Johns Hopkins University School of Medicine. He did his Internship and Residency in Internal Medicine, as well as his Infectious Diseases Fellowship, at The Mount Sinai Hospital, in New York, NY. Dr. Wormser is board certified in Internal Medicine and Infectious Diseases. Dr. Wormser's principal research interests are Lyme disease and human granulocytic anaplasmosis, with other research activities in HIV infection, infection control, and investigational antimicrobial agents and vaccine preparations.

An external file that holds a picture, illustration, etc.
Object name is zcm0030922820002.jpg Ira Schwartz (Ph.D.) is professor and chairman of the Department of Microbiology and Immunology at New York Medical College. Dr. Schwartz received his Ph.D. in Biochemistry from the City University of New York in 1973 and studied ribosome structure and function during a 2-year postdoctoral fellowship at the Roche Institute of Molecular Biology. He was an assistant professor of biochemistry at the University of Massachusetts, Amherst, from 1975 to 1980 before joining the biochemistry faculty at New York Medical College in 1980. In addition to his primary appointment, Dr. Schwartz is also a professor of medicine and of biochemistry and molecular biology at the college. Research activities in the Schwartz laboratory focus on emerging tick-borne infectious diseases, primarily Lyme disease and human granulocytic anaplasmosis. His group was among the first to develop and apply PCR and quantitative PCR to patient and tick samples, leading to practical measurements of tick-borne disease risk. Schwartz and colleagues have developed molecular typing approaches for differentiating genotypes of Borrelia burgdorferi among Lyme disease patient isolates. This resulted in identification of a B. burgdorferi genotype that more frequently is associated with disseminated infection in early Lyme disease patients. He also organized and coordinated a collaborative effort to produce B. burgdorferi genome arrays. His laboratory is currently using functional genomic approaches to identify genes that are responsible for B. burgdorferi dissemination and pathogenesis.


1. Aberer, E., A. R. Bergmann, A.-M. Derler, and B. Schmidt. 2007. Course of Borrelia burgdorferi DNA shedding in urine after treatment. Acta Derm. Venereol. 87:39-42. [PubMed]
2. Aguero-Rosenfeld, M. E., G. Wang, I. Schwartz, and G. P. Wormser. 2005. Diagnosis of Lyme borreliosis. Clin. Microbiol. Rev. 18:484-509. [PMC free article] [PubMed]
3. Alban, P. S., P. W. Johnson, and D. R. Nelson. 2000. Serum-starvation-induced changes in protein synthesis and morphology of Borrelia burgdorferi. Microbiology 146:119-127. [PubMed]
4. Ambrose, P. G., S. M. Bhavnani, C. M. Rubino, A. Louie, T. Gumbo, A. Forrest, and G. L. Drusano. 2007. Pharmacokinetics-pharmacodynamics of antimicrobial therapy: it's not just for mice anymore. Clin. Infect. Dis. 44:79-86. [PubMed]
5. Asakura, H., M. Watarai, T. Shirahata, and S.-I. Makino. 2002. Viable but nonculturable Salmonella species recovery and systemic infection in morphine-treated mice. J. Infect. Dis. 186:1526-1529. [PubMed]
6. Barer, M. R., and C. R. Harwood. 1999. Bacterial viability and culturability. Adv. Microb. Physiol. 41:94-137. [PubMed]
7. Bigger, J. W. 1944. Treatment of staphylococcal infections with penicillin. Lancet ii:497-500.
8. Bockenstedt, L. K., J. Mao, E. Hodzic, S. W. Barthold, and D. Fish. 2002. Detection of attenuated, non-infectious spirochetes in Borrelia burgdorferi-infected mice after antibiotic treatment. J. Infect. Dis. 186:1430-1437. [PubMed]
9. Bogosian, G., and E. V. Bourneuf. 2001. A matter of bacterial life and death. EMBO Rep. 2:770-774. [PubMed]
10. Cairns, V., and J. Godwin. 2005. Post-Lyme borreliosis syndrome: a meta-analysis of reported symptoms. Int. J. Epidemiol. 34:1340-1345. [PubMed]
11. del Mar Lleo, M., S. Pieroban, M. C. Tafi, C. Signoretto, and P. Canepari. 2000. mRNA detection by reverse transcription-PCR for monitoring viability over time in an Enterococcus faecalis viable but nonculturable population maintained in a laboratory microcosm. Appl. Environ. Microbiol. 66:4564-4567. [PMC free article] [PubMed]
12. Domingo, S., I. Gastearena, A. I. Vitas, I. Lopez-Goni, C. Dios-Vieitez, R. Diaz, and C. Gamazo. 1995. Comparative activity of azithromycin and doxycycline against Brucella sp infection in mice. J. Antimicrob. Chemother. 36:647-656. [PubMed]
13. Feder, H. M. Jr., B. J. B. Johnson, S. O'Connell, E. D. Shapiro, A. C. Steere, G. P. Wormser, and the Ad Hoc International Lyme Disease Group. 2007. A critical appraisal of “chronic Lyme disease.” N. Engl. J. Med. 357:1422-1430. [PubMed]
14. Fraser, C. M., S. Casjens, W. M. Huang, G. G. Sutton, R. Clayton, R. Lathigra, O. White, K. A. Kethum, R. Dodson, E. K. Hickey, M. Gwinn, B. Dougherty, J. F. Tomb, R. D. Fleischmann, D. Richardson, J. Peterson, A. R. Kerlavage, J. Quackenbush, S. Salzberg, M. Hanson, R. van Vugt, N. Palmer, M. D. Adams, J. Gocayne, J. Weidman, T. Utterback, L Watthey, L. McDonald, P. Artiach, C. Bowman, S. Garland, C. Fuji, M. D. Cotton, K. Horst, K. Roberts, B. Hatch, H. O. Smith, and J. C. Venter. 1997. Genomic sequence of a Lyme disease spirochete, Borrelia burgdorferi. Nature 390:580-586. [PubMed]
15. Hansen, K., A. Hovmark, A.-M. Lebech, K. Lebech, I. Olsson, L Halkier-Sorensen, E. Olsson, and E. Asbrink. 1992. Roxithromycin in Lyme borreliosis: discrepant results of an in vitro and in vivo animal susceptibility study and a clinical trial in patients with erythema migrans. Acta Derm. Venereol. 72:297-300. [PubMed]
16. Hatcher, S., and B. Arroll. 2008. Assessment and management of medically unexplained symptoms. Br. Med. J. 336:1124-1128. [PMC free article] [PubMed]
17. Hodzic, E., S. Feng, K. J. Freet, and S. W. Barthold. 2003. Borrelia burgdorferi population dynamics and prototype gene expression during infection of immunocompetent and immunodeficient mice. Infect. Immun. 71:5042-5055. [PMC free article] [PubMed]
18. Hodzic, E., S. Feng, K. Holden, K. J. Freet, and S. W. Barthold. 2008. Persistence of Borrelia burgdorferi following antibiotic treatment in mice. Antimicrob. Agents Chemother. 52:1728-1736. [PMC free article] [PubMed]
19. Hunfeld, K.-P., P. Kraiczy, T. A. Wichelhaus, V. Schafer, and V. Brade. 2000. New colorimetric microdilution method for in vitro susceptibility testing of Borrelia burgdorferi against antimicrobial substances. Eur. J. Clin. Microbiol. Infect. Dis. 19:27-32. [PubMed]
20. Johnson, R. C., C. B. Kodner, P. J. Jurkovich, and J. J. Collins. 1990. Comparative in vitro and in vivo susceptibilities of the Lyme disease spirochete Borrelia burgdorferi to cefuroxime and other antimicrobial agents. Antimicrob. Agents Chemother. 34:2133-2136. [PMC free article] [PubMed]
21. Johnson, R. C., C. Kodner, and M. Russell. 1987. In vitro and in vivo susceptibility of the Lyme disease spirochete, Borrelia burgdorferi, to four antimicrobial agents. Antimicrob. Agents Chemother. 31:164-167. [PMC free article] [PubMed]
22. Johnson, R. C., C. Kodner, M. Russell, and D. Girard. 1990. In vitro and in vivo susceptibility of Borrelia burgdorferi to azithromycin. J. Antimicrob. Chemother. 25(Suppl. A):33-38. [PubMed]
23. Johnson, S. E., G. C. Klein, G. P. Schmid, and J. C. Feeley. 1984. Susceptibility of the Lyme disease spirochete to seven antimicrobial agents. Yale J. Biol. Med. 57:549-553. [PMC free article] [PubMed]
24. Kannian, P., G. McHugh, B. J. B. Johnson, R. M. Bacon, L. J. Glickstein, and A. C. Steere. 2007. Antibody response to Borrelia burgdorferi in patients with antibiotic-refractory, antibiotic-responsive or non-antibiotic treated Lyme arthritis. Arthritis Rheum. 56:4216-4225. [PubMed]
25. Kazragis, R. J., L. L. Dever, J. H. Jorgensen, and A. G. Barbour. 1996. In vitro activities of ceftriaxone and vancomycin against Borrelia spp. in the mouse brain and other sites. Antimicrob. Agents Chemother. 40:2632-2636. [PMC free article] [PubMed]
26. Klempner, M. S., L. T. Hu, J. Evans, C. H. Schmid, G. M Johnson, R. P. Trevino, D. Norton, D. Wall, J. McCall, M. Kosinski, and A. Weinstein. 2001. Two controlled trials of antibiotic treatment in patients with persistent symptoms and a history of Lyme disease. N. Engl. J. Med. 345:85-92. [PubMed]
27. Lee, J., and G. P. Wormser. 2008. Pharmacodynamics of doxycycline for chemoprophylaxis of Lyme disease: preliminary findings and possible implications for other antimicrobials. Int. J. Antimicrob. Chemother. 31:235-239. [PubMed]
28. Lewis, K. 2008. Multidrug tolerance of biofilms and persister cells. Curr. Top. Microbiol. Immunol. 322:107-131. [PubMed]
29. Luft, B. J., D. J. Volkman, J. J. Halperin, and R. J. Dattwyler. 1988. New chemotherapeutic approaches in the treatment of Lyme borreliosis. Ann. N. Y. Acad. Sci. 539:352-361. [PubMed]
30. Malawista, S. E., S. W. Barthold, and D. Persing. 1994. Fate of Borrelia burgdorferi DNA in tissues of infected mice after antibiotic treatment. J. Infect. Dis. 170:1312-1316. [PubMed]
31. Moody, K. D., R. L. Adams, and S. W. Barthold. 1994. Effectiveness of antimicrobial treatment against Borrelia burgdorferi infection in mice. Antimicrob. Agents Chemother. 38:1567-1572. [PMC free article] [PubMed]
32. Mursic, V. P., B. Wilske, G. Schierz, M. Holmburger, and E. Süss. 1987. In vitro and in vivo susceptibility of Borrelia burgdorferi. Eur. J. Clin. Microbiol. 6:424-426. [PubMed]
33. Nocton, J. J., F. Dressler, B. J. Rutledge, P. N. Rys, D. H. Persing, and A. C. Steere. 1994. Detection of Borrelia burgdorferi DNA by polymerase chain reaction in synovial fluid from patients with Lyme arthritis. N. Engl. J. Med. 330:229-234. [PubMed]
34. Nystrom, T. 2003. Nonculturable bacteria: programmed survival forms or cells at death's door. BioEssays 25:204-211. [PubMed]
35. Pahl, A., U. Kuhlbrandt, K. Brune, M. Rollinghoff, and A. Gessner. 1999. Quantitative detection of Borrelia burgdorferi by real-time PCR. J. Clin. Microbiol. 37:1958-1963. [PMC free article] [PubMed]
36. Pankey, G. A., and L. D. Sabath. 2004. Clinical relevance of bacteriostatic versus bactericidal mechanisms of action in the treatment of gram-positive bacterial infections. Clin. Infect. Dis. 38:864-870. [PubMed]
37. Patel, I. H., and S. A. Kaplan. 1984. Pharmacokinetic profile of ceftriaxone in man. Am. J. Med. 77(4C):17-25. [PubMed]
38. Pavia, C., M. A. Inchiosa, Jr., and G. P. Wormser. 2002. Efficacy of short-course ceftriaxone therapy for Borrelia burgdorferi infection in C3H mice. Antimicrob. Agents Chemother. 46:132-134. [PMC free article] [PubMed]
39. Philipp, M. T., L. C. Bowers, P. T. Fawcett, M. B. Jacobs, F. T. Liang, A. R. Marques, P. D. Mitchell, J. E. Purcell, M. S. Retterree, and R. K. Straubinger. 2001. Antibody response to IR6, a conserved immunodominant region of the VlsE lipoprotein, wanes rapidly after antibiotic treatment of Borrelia burgdorferi infection in experimental animals and in humans. J. Infect. Dis. 184:870-878. [PubMed]
40. Poltorak, A., X. He, I. Smirnova, M. Y. Liu, C. Van Huffel, X. Du, D. Birdwell, E. Alejos, M. Silva, C. Galanos, M. Freudenberg, M., Ricciardi-Castagnoli, P., B. Layton, and B. Beutler. 1998. Defective LPS signaling in C3H/HeJ and C57BL/10ScCr mice: mutations in Tlr4 gene. Science 282:2085-2088. [PubMed]
41. Preac-Mursic, V., W. Marget, U. Busch, D. Pleterski Rigler, and S. Hagl. 1996. Kill kinetics of Borrelia burgdorferi and bacterial findings in relation to the treatment of Lyme borreliosis. Infection 24:9-16. [PubMed]
42. Preac-Mursic, V., B. Wilske, G. Schierz, E. Suss, and B. Gross. 1989. Comparative antimicrobial activity of the new macrolides against Borrelia burgdorferi. Eur. J. Clin. Microbiol. Infect. Dis. 8:651-653. [PubMed]
43. Rice, K. C., and K. W. Bayles. 2008. Molecular control of bacterial death and lysis. Microbiol. Mol. Biol. Rev. 72:85-90. [PMC free article] [PubMed]
44. Saivin, S., and G. Houin. 1988. Clinical pharmacokinetics of doxycycline and minocycline. Clin. Pharmacokinet. 15:355-366. [PubMed]
45. Shapiro, E. D., R. Dattwyler, R. B. Nadelman, and G. P. Wormser. 2005. Response to meta-analysis. Int. J. Epidemiol. 34:1437-1439. [PubMed]
46. Steere, A. C., and S. M. Angelis. 2006. Therapy for Lyme arthritis. Strategies for the treatment of antibiotic-refractory arthritis. Arthritis Rheum. 54:3079-3086. [PubMed]
47. Straubinger, R. K. 2000. PCR-based quantifications of Borrelia burgdorferi organisms in canine tissue over a 500-day postinfection period. J. Clin. Microbiol. 38:2191-2199. [PMC free article] [PubMed]
48. Straubinger, R. K., A. F. Straubinger, B. S. Summers, and R. H. Jacobson. 2000. Status of Borrelia burgdorferi infection after antibiotic treatment and the effects of corticosteroids: an experimental study. J. Infect. Dis. 181:1069-1081. [PubMed]
49. Straubinger, R. K., B. A. Summers, Y.-F. Chang, and M. J. G. Appel. 1997. Persistence of Borrelia burgdorferi in experimentally infected dogs after antibiotic treatment. J. Clin. Microbiol. 35:111-116. [PMC free article] [PubMed]
50. Tsiodras, S., G. Samonis, D. T. Boumpas, and D. P. Kontoyiannis. 2008. Fungal infections complicating tumor necrosis alpha blockade therapy. Mayo Clin. Proc. 83:181-194. [PubMed]
51. Wormser, G. P., S. W. Barthold, E. D. Shapiro, R. J. Dattwyler, J. S. Bakken, A. C. Steere, L. K. Bockenstedt, and J. D. Radolf. 2007. Anti-tumor necrosis factor-α activation of Borrelia burgdorferi spirochetes in antibiotic-treated murine Lyme borreliosis: an unproven conclusion. J. Infect. Dis. 196:1865-1866. [PubMed]
52. Wormser, G. P., R. J. Dattwyler, E. D. Shapiro, J. J. Halperin, A. C. Steere, M. S. Klempner, P. J., Krause, J. S. Bakken, F. Strle, G. Stanek, L. Bockenstedt, D. Fish, J. S. Dumler, and R. D. Nadelman. 2006. The clinical assessment, treatment, and prevention of Lyme disease, human granulocytic anaplasmosis, and babesiosis: clinical practice guidelines by the Infectious Diseases Society of America. Clin. Infect. Dis. 43:1089-1134. [PubMed]
53. Yrjanainen, H., J. Hytonen, K.-O. Soderstrom, J. Oksi, K. Hartiala, and M. K. Viljanen. 2006. Persistent joint swelling and borrelia-specific antibodies in Borrelia garinii-infected mice after eradication of vegetative spirochetes with antibiotic treatment. Microbes Infect. 8:2044-2051. [PubMed]
54. Yrjanainen, H., J. Hytonen, X. Y. Song, J. Oksi, K. Hartiala, and M. K. Viljanen. 2007. Anti-tumor necrosis factor-α treatment activates Borrelia burgdorferi spirochetes 4 weeks after ceftriaxone treatment in C3H/He mice. J. Infect. Dis. 195:1489-1496. [PubMed]

Articles from Clinical Microbiology Reviews are provided here courtesy of American Society for Microbiology (ASM)