Even after appropriate treatment, a proportion of Lyme disease patients suffer from a constellation of symptoms, collectively called Post-Treatment Lyme Disease Syndrome (PTLDS). Brain PET scan of patients with PTLDS have demonstrated likely glial activation indicating persistent neuroinflammatory processes. It is possible that unresolved bacterial remnants can continue to cause neuroinflammation. In previous studies, we have shown that non-viable Borrelia burgdorferi can induce neuroinflammation and apoptosis in an oligodendrocyte cell line. In this follow-up study, we analyze the effect of sonicated remnants of B. burgdorferi on primary rhesus frontal cortex (FC) and dorsal root ganglion (DRG) explants. Five FC and three DRG tissue fragments from rhesus macaques were exposed to sonicated B. burgdorferi and analyzed for 26 inflammatory mediators. Live bacteria and medium alone served as positive and negative control, respectively. Tissues were also analyzed for cell types mediating inflammation and overall apoptotic changes. Non-viable B. burgdorferi induced significant levels of several inflammatory mediators in both FC and DRG, similar to live bacteria. However, the levels induced by non-viable B. burgdorferi was often (several fold) higher than those induced by live ones, especially for IL-6, CXCL8 and CCL2. This effect was also more profound in the FC than in the DRG. Although the levels often differed, both live and dead fragments induced the same mediators, with significant overlap between FC and DRG. In the FC, immunohistochemical staining for several inflammatory mediators showed the presence of multiple mediators in astrocytes, followed by microglia and oligodendrocytes, in response to bacterial remnants. Staining was also seen in endothelial cells. In the DRG, chemokine/cytokine staining was predominantly seen in S100 positive (glial) cells. B. burgdorferi remnants also induced significant levels of apoptosis in both the FC and DRG. Apoptosis was confined to S100 + cells in the DRG while distinct neuronal apoptosis was also detected in most FC tissues in response to sonicated bacteria. Non-viable B. burgdorferi can continue to be neuropathogenic to both CNS and PNS tissues with effects likely more profound in the former. Persistence of remnant-induced neuroinflammatory processes can lead to long term health consequences.
Lyme disease (LD), caused by the bacterium Borrelia burgdorferi is the leading vector borne illness in the US and northern hemisphere. According to the latest estimates, the incidence of LD is approximately 476,000 cases per year1. Bacterial transmission occurs through tick bite, followed typically by appearance of a bulls-eye type rash called erythema migrans that appears at the site of tick attachment. This early localized phase is generally accompanied by fever, headache, and malaise, followed by an early dissemination phase affecting multiorgan systems. These include other skin areas, heart, joints and the nervous system, both central and peripheral. Early Lyme disease is treated successfully with antibiotics in most cases, when diagnosed early and treated appropriately2. However, about 10–35% of patients treated for erythema migrans or early LD have persistent or intermittent musculoskeletal, cognitive, or fatigue complaints of mild to moderate intensity at 6 to 12 months of follow up3,4,5. Other notable symptoms include, joint pain, headache, lower back pain, irritability, paresthesia, sleep issues and depression3. These symptoms are collectively termed Post-Treatment Lyme Disease Syndrome or PTLDS. In a recent study, positron emission tomography (PET) scan of PTLDS patients with radiotracer [C11]DPA-713 showed likely glial activation in the brain many months after treatment6. This radiotracer can bind/quantify cerebral TSPO, an 18-KDa translocator protein that shows increased expression in reactive astrocytes and activated microglia. The results of the study indicated that unresolved neuroinflammatory processes can persist in a cohort of patients with PTLDS.
The underlying pathophysiological mechanisms governing the PTLDS symptoms are the subject of intense controversy. Several theories have been put forward including persistent organisms impervious or inaccessible to antibiotics7,8, autoimmunity to bacterial antigens9, coinfections with other tick-borne pathogens10, post-infective fatigue syndromes, and microbiome changes11. In addition to these, in our previous study we showed that non-viable B. burgdorferi, (a state that can be achieved naturally in vivo or through the action of antibiotics), can cause inflammation and apoptosis in an oligodendrocyte cell line MO3.1312. Primary human microglia have also been shown to induce chemokines and cytokines in response to antibiotic killed or sonicated B. burgdorferi13. This suggested that in the subset of patients with persistent glial activation, residual antigens from antibiotic treatment, could be a source of this neuroinflammation.
Since our and other in vitro studies used immortalized oligodendrocytes or primary microglia alone, it was not clear if such a phenotype can occur in primary brain tissues in response to non-viable B. burgdorferi. It is possible, for instance, that this neuroinflammatory effect is masked in a tissue setting in the presence of other cells. Also, as DRG plays a role in neuropathic pain14, in this follow-up study, we analyzed the neuropathological effect of sonicated B. burgdorferi not only on primary rhesus frontal cortex tissues but also primary rhesus dorsal root ganglion tissues, sourced from multiple animals. Live B. burgdorferi was used as a positive control for induction of neuroinflammation and apoptosis. The results show that like our in vitro study on the oligodendrocyte cell line, non-viable B. burgdorferi is neuropathological to both central and peripheral nervous system (CNS and PNS) primary tissue explants, with effects beyond the oligodendrocytes.
Bacterial strain and culture
B. burgdorferi strain B31, clone 5A19, was used throughout the course of this study. This strain possesses the full complement of plasmids required for infectivity and pathogenicity and was routinely cultured in Barbour-Stoenner-Kelly (BSK-H) medium (Sigma Aldrich, St. Louis-MO) supplemented with amphotericin (0.25 µg/mL), phosphomycin (193 µg/mL) and rifampicin (45.4 µg/mL), for about 5–6 days, under microaerophilic conditions. Concentration of bacteria was determined using a dark field microscope, and the required number was harvested by centrifugation at 2095×g for 30 min at room temperature, without brakes.
Bacteria was resuspended to the original concentration in RPMI 1640 medium (BioWhittaker, Fisher Scientific, Waltham, MA) supplemented with 10% fetal bovine serum (FBS) (Hyclone, GE Lifesciences, Pittsburgh, PA) and subsequently diluted in the same medium to the desired concentrations. Non-viable bacteria were obtained by sonication according to previously published protocols12. Briefly, after resuspending the bacterial pellet in RPMI 1640, volume equivalent of live bacteria was sonicated at 40% pulse, 15% amplitude 15 s each, 7 times with a sonicator (Model 120, Fisher Scientific) and diluted in RPMI 1640 to the required equivalent concentration. Non-viability of the sonicated bacteria was verified by microscopy before each experiment.
Ex vivo assays
Frontal cortex (FC) and dorsal root ganglion (DRG) tissues were obtained from uninfected rhesus macaques (Macaca mulatta) that were euthanized from the breeding colony due to persistent diarrhea, or injury. Euthanasia was performed according to the protocols recommended and approved by the Tulane Institutional Animal Care and Use Committee. Assays were performed according to previously published protocols15. Briefly, freshly obtained FC tissues were sliced in a tissue slicer (Ted Pella Inc., Redding, CA) to approximately 2 mm thickness each and transferred to 12 well tissue culture plates containing RPMI 1640 with 10% FBS (Experimental medium, EM). The medium was replaced with fresh EM containing 1 × 107/mL of live B. burgdorferi or its sonicated equivalent in the presence or absence of Brefeldin A at a final concentration of 10 µg/mL (Molecular Probes, Eugene, OR). The latter is a fungal metabolite that prevents protein transport and enhances visualization of intracellular proteins during immunohistochemistry. As DRG tissues are very small, individual DRG or sections halved with a scalpel were used. The tissues were cocultured with the bacteria/sonicated fragments for 4 h at 37 °C, 5% CO2. Tissues in EM alone (with or without Brefeldin A) were used as Medium (negative) controls, while live bacteria were used as a positive control for chemokine/cytokine and apoptosis induction. Supernatants were collected, centrifuged at 2095×g, for 10 min at 4 °C, transferred to O-ring collection tubes (Sarstedt Inc., Newton, NC) and stored at − 20 °C, until analysis by Multiplex ELISA. Tissues were fixed in 2% paraformaldehyde overnight, washed and transferred to 30% sucrose for 2–3 days, cryopreserved in O.C.T (optimal cutting temperature) compound and stored at − 80 °C until sectioning.
Quantitation of chemokines and cytokines
Supernatants from the ex vivo assays were analyzed for IL-6, CXCL8, CCL2 by Enzyme-Linked Immuno-Sorbent assays (ELISAs) using custom non-human primate (NHP)-Procartaplex kits from Lifetechnology Corporation (Grand Island, NY), at the Pathogen Detection and Quantification Core, Tulane National Primate Research Center, and performed according to the manufacturer’s protocols. An additional custom 23-plex NHP chemokine/cytokine kit (Procartaplex, Lifetech Corp.) was used to analyze other chemokines/cytokines induced in response to live or non-viable B. burgdorferi ex vivo. The included analytes were BDNF, BLC (CXCL13), FGF-2, G-CSF (CSF-3), GM-CSF, IFN γ, IL-1β, IL-1RA, IL-4, IL-7, IL-10, IL-12p70, IL-15, IL-17A(CTLA-8), IL-18, IL-23, IP-10 (CXCL10), I-TAC (CXCL11), MIP-1α (CCL3), NGFβ, SCF, TNFα and VEGF-A. IL-6 levels in some samples were quantified using monkey IL-6 calorimetric ELISA kit according to the manufacturer’s instructions (Thermofisher Scientific, Waltham, MA). The results were graphed using Microsoft Excel® and figures were assembled using Microsoft Powerpoint® and Adobe® Photoshop CS6.
Terminal deoxynucleotidyl transferase dUTP nick-end labeling (TUNEL) assay
The effect of non-viable B. burgdorferi on cell viability of tissues was determined by TUNEL assay. Cryosections, approximately 7–10 µm thick, were stained for neuron specific MAP2, and the TUNEL assay was performed thereafter following the manufacturer’s instructions (EMD Millipore Apoptag Fluorescein kit), and as described in Ramesh et al.16. An anti-human mouse monoclonal against human MAP2 (1:50) was used as primary antibody. Appropriate secondary antibody conjugated to Alexa Fluor 568 (1:1000; Thermofisher Scientific, Waltham, MA) was used to visualize neurons. At the end of the assay, the slides were mounted with an anti-quenching reagent, cover-slipped and visualized under a fluorescent microscope. To obtain quantitative data, for each section apoptotic nuclei were counted in 10–20 fields. Average apoptotic nuclei per field was calculated for each treatment and graphed using Microsoft Excel® software.
Cryosections (7–10 µm thick) were permeabilized in phosphate buffered saline (PBS) containing 0.1% Triton-X-100, blocked with 10% normal goat serum (NGS) for 1 h, followed by staining for IL-6, IL-8 (CXCL8) or MCP-1(CCL2) along with microglia (Iba1), oligodendrocyte (MBP), astrocyte (GFAP) or neuron (MAP2 or NeuN) specific cell markers. The following primary antibodies were used: anti-human rat [(1:20), BD biosciences, Franklin Lakes, NJ] or mouse IL-6 [(1:1000) ProSpec, East Brunswick, NJ], anti-human rabbit (Fitzgerald Industries, Acton, MA) or mouse (Thermofisher Scientific, Waltham, MA) IL-8 (1:20); anti-human rabbit or mouse MCP-1 (1:20, Thermofisher Scientific); anti-human rabbit (Wako, Richmond, VA) or mouse (Santa Cruz biotechnology, Dallas, TX) Iba1 (1:50); anti human mouse MAP2 (1:50, Sigma Aldrich, St. Louis, MO); anti-human mouse NeuN (1:10, Millipore Sigma, Burlington, MA); anti-human mouse GFAP-cy3 (1:200, Sigma Aldrich) or anti-human rabbit GFAP (1:50, BioGenex, Fremont, CA); anti- human rabbit MBP (1:1000, Millipore Sigma). Following staining with primary antibody, sections were stained with appropriate secondary species-specific whole IgG antibody conjugated to Alexa Fluor 488 or Alexa Fluor 568 (both 1:1000, Thermofisher Scientific), in PBS containing 10% NGS, for 45 min–1 h each. The nuclei were stained with TOPRO-3 iodide (1:1000; Thermofisher Scientific), or DAPI (1:5000, Millipore Sigma) when required. Tissues were mounted with anti-quenching reagent, covered with coverslip and visualized for cell specific cytokine/chemokine staining.
Fluorescent microscopy pictures were captured using a Leica DMRE fluorescent microscope (Leica microsystems, Buffalo Grove-IL) and Lumecor SOLA GUI software (Lumencor, Beaverton-OR). Cells were imaged using Nuance Multispectral Imaging System (CRi, PerkinElmer, Waltham-MA). A Nikon Ti2- E fluorescent microscope (Nikon, Melville, NY), with NIS-Elements software (Nikon Instruments) was also used as required. Confocal microscopy was carried out with Leica TCS SP2 confocal microscope (Leica microsystems, Buffalo Grove, IL). Adobe® Photoshop CS6 software was used to assemble the images.
The Student’s t-test (two-tailed) was used to determine the statistical significance of an experimental outcome, with each analysis using duplicate values. The results were considered significantly different if the probability values (p) were ≤ 0.05.
Non-viable B. burgdorferi induces inflammatory mediators in primary rhesus frontal cortex tissues
Frontal cortex tissues from five different rhesus macaques were used for this study. The animal tissues were sourced from both sexes, varied in age from a little over a year to approximately 16 years of age and had both Indian and Chinese strains (Table 1). Freshly obtained tissues were exposed to live or sonicated B. burgdorferi for 4 h, and supernatants were analyzed for CCL2 (MCP-1), CXCL8 (IL-8) or IL-6. As seen in Fig. 1, non-viable B. burgdorferi was able to induce higher levels of CCL2, CXCL8 and IL-6 over medium controls in all 5 tissues, in both sexes, strains and across age groups. While these levels were statistically significant for CCL2 and CXCL8 in all 5 tissues, they were so for 3 out of 5 tissues for IL-6. Live bacteria have been shown to induce inflammatory mediators in rhesus tissues previously and hence were used as a positive control15. Surprisingly, at the same equivalent concentrations, they were less potent than non-viable B. burgdorferi and showed more variations in inflammatory mediator induction. Live bacteria induced significantly higher levels of CCL2 over medium controls in 3/5 tissues, while levels were significantly lower than medium levels in 2/5 (Fig. 1). They induced higher levels of IL-6 (than medium controls) in 4/5 tissues, (being significantly so in 2 of the 4), while being significantly lower than medium levels in 1/5. There was similarity with non-viable B. burgdorferi in induction of CXCL8 as higher levels were seen in all 5 tissues, being significantly so in 4/5. These results indicated that non-viable spirochetes are potent and consistent inducers of inflammatory mediators in primary rhesus frontal cortex tissues, and maybe more so than the live ones. To look at this more concretely, we analyzed for differences in inflammatory mediator induction between live and non-viable B. burgdorferi treatments, and the results are shown in Table 2A. CCL2 levels induced by non-viable B. burgdorferi were significantly higher than those induced by live bacteria in 4/5 animal frontal cortex tissues. IL-6 levels were again higher in those induced by non-viable B. burgdorferi in 4/5 tissues (significantly so in 3 of the 4) and 3/5 for CXCL8 (significantly higher in 2 of the 3). Only one animal (#3) showed higher levels induced by live bacteria and was in the only Chinese rhesus tissue. These results indicate that while there are variations in inflammatory mediator induction in outbred animals, non-viable B. burgdorferi is more potent and consistent inductor of neuroinflammatory mediators in brain tissues than live bacteria.
Non-viable B. burgdorferi induces inflammatory mediators in primary rhesus Dorsal root ganglion (DRG) tissues
We performed similar experiments in DRG as those described for frontal cortex using 3 animal tissues (Animals 3, 4 and 5). Unlike the frontal cortex, CCL2 was not induced by non-viable B. burgdorferi in the DRG in any of the 3 tissues tested (Fig. 2). In fact, levels were lower than those seen in medium controls and significantly so in one of the three. CXCL8 levels were, however, significantly higher than medium levels in all 3 tissues, while significantly higher IL-6 (over medium levels) was seen in 2/3 tissues. Unlike the results in frontal cortex, results with live bacteria showed more concurrence with non-viable bacteria in the DRG. Like sonicated B. burgdorferi, live bacteria also did not elicit any CCL2 in the DRG indicating this may be due to host effects than treatment. CXCL8, like those induced by non-viable bacteria, was significantly induced in all three DRG tissues by live bacteria. IL-6 levels induced by live bacteria was higher than medium levels in all three tissues also, while significantly so in 2/3. We then performed similar analysis to those done in FC to ascertain any significant differences in levels induced due to the two treatments. As seen in Table 2B, unlike those seen in frontal cortex, the results from DRG were a bit mixed. Only one of the three animals had higher levels of CCL2 induced by non-viable Borrelia compared to the live bacteria induced levels. With respect to CXCL8, non-viable Borrelia induced higher levels compared to live ones in 1/3, while the live bacteria induced a similar effect in 1/3. IL-6 levels, however, were significantly higher in tissue sections exposed to non-viable Borrelia in 2/3 animals while it was higher in those that received live bacteria in 1/3.
Since FC and DRG were sourced from the same animals numbered 3–5, it is also clear that there are significant differences in tissue specific responses to the same pathogen/antigens. Just taking non-viable bacteria for consideration, FC from animals 3, 4 and 5 induced CCL2 in response to Borrelial fragments, but not in the DRG of the same animals. So, the results thus far indicate that inflammatory response to live Borrelia or its fragments depend on the treatment and tissue source, with non-viable B. burgdorferi seemingly more potent inducers than the live bacteria in the brain, while they are somewhat similar in the DRG.
Are there any inflammatory/cytokine signatures that can distinguish live and non-viable B. burgdorferi?
Since the inflammatory mediators tested thus far were induced by both live and non-viable bacteria, we next sought to ascertain if there are any specific inflammatory mediators or cytokines that are induced only by one or the other stimulant that could serve as a signature for the type of antigen (live or dead). We generated a custom 23-plex kit based on the chemokines/cytokines seen in the cerebrospinal fluid (CSF) of patients with Lyme neuroborreliosis (LNB)17 and similarly analyzed the supernatants from FC and DRG tissues to determine inflammatory signature differences between the two treatments. The results are shown in Table 3. Of the 23 mediators tested, only 7 were detected in the supernatants of FC in response to treatments (Table 3A). Only FGF2 was significantly secreted in ng/ml quantity, followed by IL-1RA. Levels of all the other 5 were low to modest. Like the previous results in the FC with IL-6, CXCL8 and CCL2 (Fig. 1), there were more tissue samples that significantly induced a mediator with non-viable Borrelia than with live ones, but not exclusively so. FGF2 was significantly induced in 2/5 tissues by non-viable B. burgdorferi compared to 1/5 with live bacteria. Similar results were observed with GCSF (2/5 vs 1/5), IL-1Ra (3/5 vs 2/5) and SCF (2/5 vs 1/5), while IL-1β, IL-18 and MIP1α were significantly induced by both live and non-viable bacteria in all 5 FC tissues. A similar analysis was also performed in the DRG. Eight mediators were detected in the supernatants of the DRG tissues exposed to either live or sonicated bacteria (Table 3B). However, IL-18 was not secreted in the DRG but IL-17A and VEGF-A were. Lower levels of FGF2 and higher levels of GCSF in comparison to FC induced levels was seen, indicating tissue specific differences in the secretion of mediators but not due to treatment differences. Like the results seen in FC, DRG also did not elicit any inflammatory signature induced exclusively by live or non-viable bacteria. FGF2 and IL-17A were significantly induced in 2/3 DRG tissues in response to sonicated bacteria while 3/3 tissues induced significant levels of these mediators in response to live B. burgdoferi. 2 of the 3 tissues induced significant VEGF-A with non-viable bacteria vs 1/3 with live organisms. 1/3 tissues induced significant IL-1RA with sonicated bacteria vs none with live bacteria in the DRG. SCF was significantly induced in only one animal tissue with both live and dead B. burgdorferi. However, both treatments elicited significant levels of GCSF, IL-1β, and MIP1α in all 3 tissues, overlapping with the FC results.
Inflammatory mediators are induced predominantly in glial cells (and endothelial cells) in response to non-viable B. burgdorferi
In previous studies, live bacteria were shown to induce specific inflammatory mediators from microglia (IL-1β, CXCL13, Cox 2) and astrocytes (IL-6, IL-8, Cox 2) in the FC15 by immunohistochemistry. Likely endothelial cells of the blood vessels were also reported to induce IL-8. In this study we examined the type of cells that responded to non-viable B. burgdorferi to induce inflammatory mediator production. We specifically analyzed for IL-6, IL-8 and MCP-1, in the FC and counterstained for oligodendrocytes (MBP), microglia (Iba1), astrocytes (GFAP) and neurons (MAP2). We also analyzed sections from both brefeldin A plus (Bre+) and brefeldin A minus (Bre−) treatments to increase the chances of double staining. The results are shown in Fig. 3.
IL-6 staining was seen in endothelial cells in FC tissues from multiple animals (Fig. 3 top panel, i). Similar IL-6 staining pattern was also seen in sections from medium only tissues. However, there was an approximately twofold increase in the number of endothelial cells staining for IL-6 in tissues exposed to non-viable Borrelia compared to medium controls (not shown). IL-6 staining was also seen in GFAP stained astrocytes surrounding the endothelial cells (yellow colocalization, indicated by white arrow, Fig. 3 top panel, i) and elsewhere in the tissue, along with microglia and oligodendrocytes (not shown). IL-8 staining was seen similarly in endothelial cells of likely lymph or blood vessels (Fig. 3 top panel, ii, iii), and in Iba1 positive cells (arrow, Fig. 3 top panel, ii). (To confirm that these cells were endothelial cells, additional tissue sections were stained for GFAP/Caveolin-1 (1:100, Sigma Aldrich), or GFAP/ von Willebrand factor (1:50, DAKO). Caveolin-1 is highly expressed in endothelial cells, while von Willebrand factor served as an additional marker to identify endothelial cells18,19. Based on the staining patterns in similar structures, we concluded that the non-GFAP but IL-6/IL-8 positive, non-Iba1 but IL-8 positive cells in Fig. 3 top panel are likely endothelial cells. IL-8 staining was also seen in GFAP positive cells (Fig. 3, middle panel) while MCP-1 was seen in GFAP positive astrocytes (Fig. 3 bottom panel). We did not see any specific staining in neurons. To summarize, in the FC, IL-6 staining was seen in endothelial cells, astrocytes, microglia and oligodendrocytes, IL-8 in endothelial cells, microglia and astrocytes, MCP-1 in astrocytes.
Similar analysis was also conducted for DRG tissues, with staining for IL-6, IL-8 and MCP-1 and counterstained with S100 (satellite glial cells, Schwann cells) or NeuN (neurons). The results are shown in Fig. 4. Staining was seen in primarily in the S100 positive cells for MCP-1, IL-8 (Fig. 4, top and bottom panels) and IL-6 (not shown). A few cells that were non S100 also stained for IL-6 (not shown). Staining in NeuN positive cells was not conclusive.
Non-viable B. burgdorferi induces apoptosis in the FC and DRG
In previous studies, live B. burgdorferi was shown to induce apoptosis in oligodendrocytes and neurons in frontal cortex explants at 4 h15. Studies have also shown that this cell death occurs in an inflammatory environment16,20. Since non-viable B. burgdorferi similarly induced an inflammatory environment in both FC and DRG, we next analyzed their ability to cause cell death by apoptosis. The results are shown in Fig. 5, with live bacteria as a positive control and medium only tissues as a negative control for apoptosis induction. As seen in the Fig. 5A, non-viable B. burgdorferi was able to induce apoptosis in all 5 FC tissues, with levels statistically significant over medium controls. Live bacteria as expected, also showed higher levels of apoptotic nuclei in comparison to medium only control tissues, with levels being statistically significant in 3/5 tissues.
Unlike the inflammatory levels, there was not much significant difference in the apoptotic levels induced by non-viable or live B. burgdorferi in most tissues, except in tissue from Animal 5 where live bacteria induced apoptosis was significantly higher than that induced by non-viable bacteria (Fig. 5A). We next looked for the type of cells undergoing apoptosis in the FC tissues with non-viable B. burgdorferi treatment. Figures 5B and C show apoptotic nuclei predominantly in non-MAP2 cells, (neurons stained for MAP-2 in red), presumably oligodendrocyte glial cells, in response to non-viable B. burgdorferi. However, neuronal apoptosis was also seen (Fig. 5Biii,Ciii) in response to sonicated B. burgdorferi fragments, albeit at much lower levels in comparison to glial cell apoptosis. Neuronal apoptosis in MAP-2 positive cells was seen in 4/5 tissues in response to non-viable bacteria while live bacteria mediated neuronal apoptosis was seen in 5/5 tissues (not shown). We then performed similar analysis in DRG tissues (Fig. 6). Both live and non-viable B. burgdorferi were able to significantly induce apoptosis in all three DRG tissues in comparison to medium only controls (Fig. 6A). No significant difference was observed between apoptosis levels mediated by live or non- viable bacteria in all three tissues. Apoptosis was seen predominantly in S100 positive cells (Fig. 6B,C) in response to non-viable B. burgdorferi and in some non NeuN/non S100 cells (not shown). We did not see apoptosis in neuronal cells in any of the three DRG tissues exposed to sonicated B. burgdorferi fragments (Fig. 6C), while 1 of the 3 DRG tissue showed neuronal apoptosis in response to live bacteria (not shown).
We show in this study that non-viable B. burgdorferi can mediate neuroinflammation and apoptosis (Figs. 1, 2, 5, 6) in primary rhesus FC and DRG tissues ex vivo. The bacterial fragments often elicited higher levels of inflammatory mediators than the live bacteria at the same equivalent concentration. This is likely due to the fact that upon lysis, multiple ligands such as lipoproteins, flagellins, DNA, RNA and others, are released, which can stimulate several TLR receptors21, many more than intact bacteria. As bacterial debris likely spreads wider, this could also lead to wider activation of inflammatory signaling pathways resulting in higher levels of inflammatory mediators. This effect was more pronounced in the FC than the DRG and is likely due to the presence of glial cells such as microglia and astrocytes in the CNS. These cells are a significant source of inflammatory mediators, and activation of more of such cells would greatly add to the inflammatory output, as evidenced by the staining of multiple mediators in these cells (Fig. 3). Previous studies have shown that live B. burgdorferi can mediate inflammation and apoptosis in FC explants and were used as a positive control15,20. However, as seen from Fig. 1, not all FC tissue samples induced significant levels of inflammatory mediators over medium controls in response to live bacteria. At least 2/5 animals did not respond to live bacterial stimulus in mediating CCL2, IL-6 release (Fig. 1) while in the same animal tissues they responded to sonicated bacteria. This indicated that not only do the sonicated bacteria induce higher levels of inflammatory mediators than do live bacteria, they are also capable of being neuroinflammatory even if live bacteria are not. As for the variability of results with live bacteria in comparison to previous studies, rhesus macaques are outbred and not genetically identical. Hence some variability is not unexpected, although they did induce mediators in most tissues. We expected to see increased MCP-1 secretion in the DRG cells. Surprisingly, DRG tissues from all three animals did not elicit any significant levels of MCP-1 in comparison to medium controls, with either live or dead bacteria (Fig. 2). As previous studies have only stained for MCP-1 in DRG tissue and not their levels in the supernatants, it is not clear if this is different from previous results, but if so, it could be again be due to genetic variability22,23,24. Another surprising result was the level of inflammatory mediators induced by the FC vs DRG. FC tissue sections were at least 4 times larger than the DRG sections. Yet when compared within the same animal, the levels induced by DRG sections were higher than those induced in the FC. This is likely because perhaps due to its small size, the multiplicity of infection is higher in the DRG.
Since IL-6, IL-8 (CXCL8) and MCP-1 (CCL2) were the three mediators consistently seen to be secreted in FC tissues, these were the mediators initially tested, and extended to the DRG tissues. We further expanded the repertoire to 23 other chemokines and cytokines based on the data published in CSF of LNB patients17. We show that in addition to IL-6, IL-8 and MCP-1, the non-viable bacteria also induced several other chemokines and cytokines, in more tissues than with live bacteria in both the FC and DRG (Table 3). This was undertaken to determine if there were any mediators uniquely induced by either bacterial remnants or by the live ones, and we failed to find any such unique mediator. It is possible that we might find such a mediator through transcriptomics or other omics analysis. Previous studies have demonstrated the presence of IL-10 and VEGF from FC tissues in response to live bacteria15,20. However, we did not find them secreted into the supernatants in our study by either treatment, reiterating the variability seen in rhesus macaques just like in humans. Regarding the other mediators that were significantly secreted into the supernatants of FC or DRG tissues (Table 3), IL-1β, IL-18, MIP1α, IL-17A are considered inflammatory proteins25,26,27. Interestingly, IL-17A has been demonstrated to signal through its receptor in rat neurons to promote pain sensitivity28. Conflicting roles have been reported for GCSF and FGF2. On the one hand they have both been shown to attenuate neuroinflammation and neuronal apoptosis in rodent models29,30,31. On the other hand, GCSF has been shown to drive inflammation in rheumatoid arthritis and others32,33,34, while FGF2 to induce neuronal apoptosis in primary mouse neuron/glial cultures35. VEGF-A, the endothelial growth factor is another molecule demonstrated to have conflicting effects. In rodent models, blocking of VEGF-A has been shown to alleviate painful neuropathies by reducing nociception36. On the other hand, a monoclonal VEGF antibody was demonstrated to exacerbate neuropathy and pain in breast cancer patients37. SCF (also called Kit ligand) is a mast cell chemotactic factor that mediates mast cell degranulation and histamine release38. B. burgdorferi has been demonstrated to activate mast cells and release histamine upon coculture with rat or mouse mast cells39. Mast cell deficiency in Kitwsh−/− mice enabled faster mobilization of B. burgdorferi to the joints, implicating a role in dissemination40. IL-1RA on the other hand, is considered to have anti-inflammatory properties as it inhibits IL-1 mediated signaling41. While the roles of these individual mediators in B. burgdorferi mediated neuroinflammation is yet to be determined, it is likely that both non-viable and live B. burgdorferi induce a mix of majority pro-inflammatory factors with a few anti-inflammatory, neuroprotective mediators to counteract the former. However, it is interesting to note that the majority of these mediators such as IL-6, IL-8 (CXCL8), MCP-1(CCL2), IL-1β, IL-18, GCSF, VEGF-A, IL-17A and FGF2 also have one thing in common, in that they have all been demonstrated to be proalgesic, mediating nociception sensitization in various pain conditions42,43,44,45,46. It is possible that production of these various mediators has a cumulative effect in inducing pain. Testing the CSF of PTLDS patients with chronic pain or CSF, brain tissue/DRG analysis in relevant in vivo animal models with non-viable B. burgdorferi might provide some answers.
The identity of the cells that respond to non-viable B. burgdorferi treatment in inducing inflammatory mediators was also examined. As reported with live B. burgdorferi15, it was predominantly the glial cells that responded to sonicated bacteria. IL-8 and IL-6 staining was also seen in likely endothelial cells in the FC. This has implications for blood brain barrier (BBB) breach. IL-6 can modulate tight junction proteins of endothelial cells in a dose dependent manner, with higher concentrations leading to leakiness of the barrier47. Similar effects with increased IL-8 has also been reported48. Thus it is possible that in vivo, bacterial fragments can cause breach in BBB and cause increased transport of immune cells, inflammatory mediators or even live bacteria. As a point of fact, in non-human primates, presence of intact bacteria (presumably live, and not killed by antibiotics) have been found in the CNS of antibiotic treated animal49. Since the tissues used in this study are short-lived, it is not clear how long the neuroinflammation induced by bacterial remnants can last, and if they are different from live bacteria mediated neuroinflammation in vivo. Interestingly, a previous study by Qin et al. showed that intraperitoneal injection of LPS can cause an increase in CNS TNFα which remained for about 10 months50. Given the likely glial cell activation in patients’ brain months after Lyme disease treatment, it is imperative that such studies in vivo are undertaken, to determine whether non-viable B. burgdorferi remnants can reach the CNS, and/or cause neuroinflammation. In the DRG, MCP-1 and IL-6 staining has been reported in neurons, satellite glial cells and Schwann cells, and IL-8 in satellite glial cells and Schwann cells in response to live bacteria22. In our study, IL-8, IL-6 and MCP-1 staining was seen with S100 positive cells only and not in NeuN stained cells (Fig. 4, and not shown) indicating a glial predominance in inflammatory mediator production. While it is possible that we might have missed neuronal double staining for mediators, it is also possible that neurons do not respond to non-viable B. burgdorferi. In vitro primary neuronal cell cultures assays can provide an answer to this possibility. Nevertheless, as DRG are becoming integral to neuropathic pain studies, release of inflammatory mediators in response to sonicated fragments in the DRG has implications for neuropathic pain14.
Both glial and neuronal apoptosis were recorded in the FC in response to sonicated bacteria. In the DRG, apoptosis was only seen in S100 positive cells and not in NeuN positive areas in any of the three animal tissues. It is not clear if prolonged incubation would result in neuronal apoptosis, and remains to be investigated either in vitro in primary cultures or in organotypic slice cultures. However, this fact, (neuronal apoptosis in CNS vs lack of in the DRG) along with the more profound inflammatory effect in the CNS indicated that while the non-viable bacteria are pathogenic in both tissues, they are likely more deleterious in the CNS in comparison to the PNS.
In conclusion, we show in this study that non-viable remnants of B. burgdorferi are pathogenic to both the CNS and PNS tissues. Presence of chemokines and cytokines in glial cells and endothelial cells in the CNS in response to non-viable fragments has implications for blood–brain barrier breach. Induction of several proalgesic mediators in both the FC and DRG has implications for chronic pain conditions. Persistence of symptoms in some patients post-treatment indicates that in a subset of these patients, B. burgdorferi fragments in the nervous system could be a cause. Such antibiotic refractive conditions need novel anti-inflammatory approaches for therapeutics.
The datasets used and/or analyzed during the current study are available from the corresponding author on reasonable request.
Blood brain barrier
Brain derived neurotrophic factor
B lymphocyte chemoattractant
Central nervous system
Chemokine (C–C) motif ligand 2
Chemokine (C–C) motif ligand 3
Colony stimulating factor 3
Chemokine (C–X–C) motif ligand 8
(C–X–C) motif chemokine ligand 10
(C–X–C) motif chemokine ligand 11
(C–X–C) motif chemokine ligand 13
Dorsal root ganglion
Enzyme linked immunosorbent assay
Fetal bovine serum
Fibroblast growth factor 2
Granulocyte colony stimulating factor
Glial fibrillary acidic protein
Granulocyte macrophage colony stimulating factor
Interleukin 1 receptor alpha
Interferon gamma induced protein 10
Interferon-inducible T-cell alpha chemoattractant
Myelin basic protein
Macrophage inflammatory protein 1 alpha
Nerve growth factor bet
Normal goat serum
Phosphate buffered saline
Positron emission tomography
Peripheral nervous system
Post-treatment Lyme disease syndrome
Stem cell factor
Tumor necrosis factor alpha
Terminal deoxynucleotidyl transferase dUTP nick-end labeling
Vascular endothelial growth factor
Kugeler, K. J., Schwartz, A. M., Delorey, M. J., Mead, P. S. & Hinckley, A. F. Estimating the frequency of lyme disease diagnoses, United States, 2010–2018. Emerg. Infect. Dis. 27, 616–619 (2021).
Wormser, G. P. et al. 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 (2006).
Rebman, A. W. et al. The clinical, symptom, and quality-of-life characterization of a well-defined group of patients with posttreatment lyme disease syndrome. Front. Med. 4, 224 (2017).
Rebman, A. W. & Aucott, J. N. Post-treatment lyme disease as a model for persistent symptoms in lyme disease. Front. Med. 7, 57 (2020).
Aucott, J. N., Rebman, A. W., Crowder, L. A. & Kortte, K. B. Post-treatment Lyme disease syndrome symptomatology and the impact on life functioning: Is there something here?. Qual. Life Res. 22, 75–84 (2013).
Coughlin, J. M. et al. Imaging glial activation in patients with post-treatment Lyme disease symptoms: A pilot study using [(11)C]DPA-713 PET. J. Neuroinflammation 15, 346 (2018).
Embers, M. E. et al. Persistence of Borrelia burgdorferi in rhesus macaques following antibiotic treatment of disseminated infection. PLoS ONE 7, e29914 (2012).
Hodzic, E., Imai, D., Feng, S. & Barthold, S. W. Resurgence of persisting non-cultivable Borrelia burgdorferi following antibiotic treatment in mice. PLoS ONE 9, e86907 (2014).
Bolz, D. D. & Weis, J. J. Molecular mimicry to Borrelia burgdorferi: Pathway to autoimmunity?. Autoimmunity 37, 387–392 (2004).
Sloupenska, K. et al. Seroprevalence of antibodies against tick-borne pathogens in czech patients with suspected post-treatment lyme disease syndrome. Microorganisms 9, 2217 (2021).
Morrissette, M. et al. A Distinct microbiome signature in posttreatment lyme disease patients. MBio 11, 10 (2020).
Parthasarathy, G., Fevrier, H. B. & Philipp, M. T. Non-viable Borrelia burgdorferi induce inflammatory mediators and apoptosis in human oligodendrocytes. Neurosci. Lett. 556, 200–203 (2013).
Greenmyer, J. R., Gaultney, R. A., Brissette, C. A. & Watt, J. A. Primary human microglia are phagocytically active and respond to Borrelia burgdorferi with upregulation of chemokines and cytokines. Front. Microbiol. 9, 811 (2018).
Sommer, C., Leinders, M. & Uceyler, N. Inflammation in the pathophysiology of neuropathic pain. Pain 159, 595–602 (2018).
Ramesh, G. et al. Interaction of the Lyme disease spirochete Borrelia burgdorferi with brain parenchyma elicits inflammatory mediators from glial cells as well as glial and neuronal apoptosis. Am. J. Pathol. 173, 1415–1427 (2008).
Ramesh, G., Benge, S., Pahar, B. & Philipp, M. T. A possible role for inflammation in mediating apoptosis of oligodendrocytes as induced by the Lyme disease spirochete Borrelia burgdorferi. J. Neuroinflammation 9, 72 (2012).
Pietikainen, A. et al. Cerebrospinal fluid cytokines in Lyme neuroborreliosis. J. Neuroinflammation 13, 273 (2016).
Frank, P. G., Woodman, S. E., Park, D. S. & Lisanti, M. P. Caveolin, caveolae, and endothelial cell function. Arterioscler. Thromb. Vasc. Biol. 23, 1161–1168 (2003).
Dmitrieva, N. I. & Burg, M. B. Secretion of von Willebrand factor by endothelial cells links sodium to hypercoagulability and thrombosis. Proc. Natl. Acad. Sci. USA 111, 6485–6490 (2014).
Ramesh, G., Martinez, A. N., Martin, D. S. & Philipp, M. T. Effects of dexamethasone and meloxicam on Borrelia burgdorferi-induced inflammation in glial and neuronal cells of the central nervous system. J. Neuroinflammation 14, 28 (2017).
Parthasarathy, G. & Philipp, M. T. Inflammatory mediator release from primary rhesus microglia in response to Borrelia burgdorferi results from the activation of several receptors and pathways. J. Neuroinflammation 12, 60 (2015).
Ramesh, G., Santana-Gould, L., Inglis, F. M., England, J. D. & Philipp, M. T. The Lyme disease spirochete Borrelia burgdorferi induces inflammation and apoptosis in cells from dorsal root ganglia. J. Neuroinflammation 10, 88 (2013).
Ramesh, G., Meisner, O. C. & Philipp, M. T. Anti-inflammatory effects of dexamethasone and meloxicam on Borrelia burgdorferi-induced inflammation in neuronal cultures of dorsal root ganglia and myelinating cells of the peripheral nervous system. J. Neuroinflammation 12, 240 (2015).
Martinez, A. N., Ramesh, G., Jacobs, M. B. & Philipp, M. T. Antagonist of the neurokinin-1 receptor curbs neuroinflammation in ex vivo and in vitro models of Lyme neuroborreliosis. J. Neuroinflammation 12, 243 (2015).
Kaneko, N., Kurata, M., Yamamoto, T., Morikawa, S. & Masumoto, J. The role of interleukin-1 in general pathology. Inflamm. Regen. 39, 12 (2019).
Cook, D. N. The role of MIP-1 alpha in inflammation and hematopoiesis. J. Leukoc. Biol. 59, 61–66 (1996).
Zenobia, C. & Hajishengallis, G. Basic biology and role of interleukin-17 in immunity and inflammation. Periodontol. 2015(69), 142–159 (2000).
Richter, F. et al. Interleukin-17 sensitizes joint nociceptors to mechanical stimuli and contributes to arthritic pain through neuronal interleukin-17 receptors in rodents. Arthritis Rheum. 64, 4125–4134 (2012).
Dumbuya, J. S. et al. G-CSF attenuates neuroinflammation and neuronal apoptosis via the mTOR/p70SK6 signaling pathway in neonatal Hypoxia-Ischemia rat model. Brain Res. 1739, 146817 (2020).
Tang, C. et al. FGF2 attenuates neural cell death via suppressing autophagy after rat mild traumatic brain injury. Stem Cells Int. 2017, 2923182 (2017).
Tang, M. M., Lin, W. J., Pan, Y. Q. & Li, Y. C. Fibroblast growth factor 2 modulates hippocampal microglia activation in a neuroinflammation induced model of depression. Front. Cell Neurosci. 12, 255 (2018).
Lawlor, K. E. et al. Critical role for granulocyte colony-stimulating factor in inflammatory arthritis. Proc. Natl. Acad. Sci. USA 101, 11398–11403 (2004).
Kim, Y. M. et al. Airway G-CSF identifies neutrophilic inflammation and contributes to asthma progression. Eur. Respir. J. 55, 1900827 (2020).
Tsantikos, E. et al. Granulocyte-CSF links destructive inflammation and comorbidities in obstructive lung disease. J. Clin. Invest. 128, 2406–2418 (2018).
Liu, X., Albano, R. & Lobner, D. FGF-2 induces neuronal death through upregulation of system xc. Brain Res. 1547, 25–33 (2014).
Llorian-Salvador, M. & Gonzalez-Rodriguez, S. Painful understanding of VEGF. Front. Pharmacol. 9, 1267 (2018).
Matsuoka, A. et al. Bevacizumab exacerbates paclitaxel-induced neuropathy: A retrospective cohort study. PLoS ONE 11, e0168707 (2016).
Okayama, Y. & Kawakami, T. Development, migration, and survival of mast cells. Immunol Res. 34, 97–115 (2006).
Talkington, J. & Nickell, S. P. Borrelia burgdorferi spirochetes induce mast cell activation and cytokine release. Infect. Immun. 67, 1107–1115 (1999).
Bernard, Q., Wang, Z., Di Nardo, A. & Boulanger, N. Interaction of primary mast cells with Borrelia burgdorferi (sensu stricto): role in transmission and dissemination in C57BL/6 mice. Parasit. Vectors 10, 313 (2017).
Volarevic, V., Al-Qahtani, A., Arsenijevic, N., Pajovic, S. & Lukic, M. L. Interleukin-1 receptor antagonist (IL-1Ra) and IL-1Ra producing mesenchymal stem cells as modulators of diabetogenesis. Autoimmunity 43, 255–263 (2010).
Verri, W. A. Jr. et al. Hypernociceptive role of cytokines and chemokines: Targets for analgesic drug development?. Pharmacol. Ther. 112, 116–138 (2006).
Madiai, F. et al. Anti-fibroblast growth factor-2 antibodies attenuate mechanical allodynia in a rat model of neuropathic pain. J. Mol. Neurosci. 27, 315–324 (2005).
Dos Santos, G., Delay, L., Yaksh, T. L. & Corr, M. Neuraxial cytokines in pain states. Front. Immunol. 10, 3061 (2019).
Schweizerhof, M. et al. Hematopoietic colony-stimulating factors mediate tumor-nerve interactions and bone cancer pain. Nat. Med. 15, 802–807 (2009).
Jin, L., Nonaka, Y., Miyakawa, S., Fujiwara, M. & Nakamura, Y. Dual therapeutic action of a neutralizing anti-FGF2 aptamer in bone disease and bone cancer pain. Mol. Ther 24, 1974–1986 (2016).
Cohen, S. S. et al. Effects of interleukin-6 on the expression of tight junction proteins in isolated cerebral microvessels from yearling and adult sheep. NeuroImmunoModulation 20, 264–273 (2013).
Kossmann, T. et al. Interleukin-8 released into the cerebrospinal fluid after brain injury is associated with blood-brain barrier dysfunction and nerve growth factor production. J. Cereb. Blood Flow Metab. 17, 280–289 (1997).
Crossland, N. A., Alvarez, X. & Embers, M. E. Late disseminated lyme disease: Associated pathology and spirochete persistence posttreatment in rhesus macaques. Am. J. Pathol. 188, 672–682 (2018).
Qin, L. et al. Systemic LPS causes chronic neuroinflammation and progressive neurodegeneration. Glia 55, 453–462 (2007).
We thank the TNPRC Pathogen Detection and Quantification Core Laboratory for help with the multiplex ELISA assays. We thank Dr. Pete Didier for his valuable advice on brain histology. We thank the microscopy core for help with confocal imaging, and the histology core for help with tissue sectioning.
This study was supported by the Bay Area Lyme Foundation Grant 557243 and the TNPRC base Grant P51OD011104.
The authors declare no competing interests.
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Parthasarathy, G., Gadila, S.K.G. Neuropathogenicity of non-viable Borrelia burgdorferi ex vivo. Sci Rep 12, 688 (2022). https://doi.org/10.1038/s41598-021-03837-0
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