Abstract
Chronic inflammatory insults compromise immune cell responses and ultimately contribute to pathologic outcomes. Clinically, it has been suggested that bone debris and implant particles, such as polymethylmethacrylate (PMMA), which are persistently released following implant surgery evoke heightened immune, inflammatory, and osteolytic responses that contribute to implant failure. However, the precise mechanism underlying this pathologic response remains vague. TREGS, the chief immune-suppressive cells, express the transcription factor Foxp3 and are potent inhibitors of osteoclasts. Using an intra-tibial injection model, we show that PMMA particles abrogate the osteoclast suppressive function of TREGS. Mechanistically, PMMA particles induce TREG instability evident by reduced expression of Foxp3. Importantly, intra-tibial injection of PMMA initiates an acute innate immune and inflammatory response, yet the negative impact on TREGS by PMMA remains persistent. We further show that PMMA enhance TH17 response at the expense of other T effector cells (TEFF), particularly TH1. At the molecular level, gene expression analysis showed that PMMA particles negatively regulate Nrp-1/Foxo3a axis to induce TREG instability, to dampen TREG activity and to promote phenotypic switch of TREGS to TH17 cells. Taken together, inflammatory cues and danger signals, such as bone and implant particles exacerbate inflammatory osteolysis in part through reprogramming TREGS.
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Introduction
Inflammatory osteolysis is a major complication of orthopedic joint implants1. Debris released from these implants trigger immune and inflammatory responses that promote recruitment of macrophages and osteoclasts to the injury site2. This cell- and cytokine-based pathologic response accelerates bone erosion around the implant leading to loosening and ultimately failure of implants, which poses high morbidity and mortality risks. Despite extensive efforts, the details of the biologic response to implant debris remain enigmatic and the complete repertoire by which orthopedic particles modulate cell lineages to enhance inflammation and exacerbate osteolysis remains poorly understood.
The cellular response to inflammatory triggers, including PMMA and bone particles, entails recruitment and activation of myeloid and immune cells such as macrophages, dendritic cells, granulocytes and lymphocytes. The ensuing inflammatory response is consistent with release of wear particles from implants and intensifies with increased particle burden akin to chronic response3,4,5. These particles are largely associated with inflammatory macrophages and osteoclasts at the implant-bone interface. However, the presence of multitude of other immune cell types, especially lymphocytes was also noted6,7,8,9,10. T lymphocytes mediate the adaptive phase of the immune response and are typically activated by antigen presenting cells such as dendritic cells. The most frequent subsets of these cells in inflammatory loci include T regulatory (TREG) and T helper (TH) cells. TREG cells express the transcription factor Foxp3 and elicit inhibitory activity. On the other hand, TH cells can differentiate based on their response to specific sets of factors in their microenvironment into TH1, TH17, or TH2 subtypes. Whereas TH1 and TH17 respectively secrete TNFα, IFNγ and IL-17A among many other pro-inflammatory cytokines, TH2 cells secrete primarily anti-inflammatory mediators including IL-4 and IL-1011.
The specific contribution of lymphocytes to wear debris-induced inflammatory osteolysis remains controversial. In this regard, circumstantial findings point to potential direct lymphocyte involvement as well as indirect action through secretion of pro-inflammatory and pro-osteoclastogenic factors such as RANKL, IL-17A, M-CSF or anti-osteoclastogenic factors such as IFNγ and IL-49,12,13,14,15. Notably, we have shown recently that mice harboring loss-of-function mutant foxp3 in T cells display severe osteopenia16. This finding led us to speculate that reduced immunosuppression is conceivably one of the major reprogramming of immune cells elicited by PMMA particles during the progression of inflammatory osteolysis. Hence, the goal of this study is to decipher the pathologic mechanisms by which implant debris modulate lymphocytes to exacerbate inflammatory osteolysis. To this end, we show that PMMA particles, likely through a stress mechanism, modulate T cell activation by down-regulating Foxp3 function, resulting with T cell phenotypic switch from TREG into pathogenic TH cells with enhanced NF-κB activity. Mechanistically, we provide evidence that particles down regulate expression of Nrp-1 leading to reprogramming of TREGS. This change not only renders TREGS incapable of inhibiting osteoclasts, but they secrete pro-osteoclastogenic and pro-inflammatory factors that expand the myeloid-progenitor population and enhance osteoclastogenesis.
Results
PMMA particles induce NF-κB activity and alter bone marrow cellularity toward reduced immunosuppression
We have shown previously that PMMA particles robustly activate NF-κB in myeloid cells leading to pro-inflammatory and pro-osteolytic conditions17,18. We have also shown recently that activity of NF-κB is exacerbated under conditions of TREG cell inactivity wherein the transcription factor foxp3 is mutated16. To further examine the cellular response to PMMA, we established a new experimental mouse model whereby PMMA particles or vehicle were injected directly into the proximal tibia using a 27G syringe. At different time points post injection, in vivo NF-κB reporter activity was measured. In addition, myeloid cells and lymphocytes from bone marrow and spleen were FACS sorted and quantified. Our data indicate that NF-κB luciferase activity in the whole bone marrow of PMMA-injected RelA-luc reporter mice was significantly (4 folds) elevated compared with baseline activity in control PBS-injected mice (Fig. 1a). We then used FACS analysis to examine the cellular response locally at the site of PMMA injection, namely the tibia and at adjacent femurs. The data depicted in Fig. 1 indicate that as early as two days post injection, PMMA particles induced two-fold increase in all myeloid progenitor populations examined, including lineage−c-Sca-1+c-kit+ hematopoietic stem cells (LSK HSCs) lineage−c-kit+CD34+Fcγ− common myeloid progenitors (CMPs) and lineage−c-kit+CD34+F4/80+ granulocyte-macrophage progenitors (GMPs) (Fig. 1b) while significantly reducing Foxp3+ TREG cells in tibia bone marrow (Fig. 1c) and marginally affecting cellularity in adjacent femurs (data not shown). We also examined the compartment of more committed and mature myeloid populations in the bone marrow and found frequencies of CD11b+Gr1+ granulocytic cells were elevated in PMMA injected tibias, while the frequency of CD11b+Gr1− monocytic cells was unaffected (Fig. 1d). Furthermore, these cellular changes summoned a moderately yet significantly elevated osteoclastogenic potential of whole bone marrow cells, indicating PMMA also increased osteoclast progenitors and/or their osteoclastogenic potential at the injection site (Fig. 1e,f).
PMMA particles modulate extra-medullary hematopoiesis in the spleen
To evaluate plausible systemic response to PMMA injection in the tibia, we examined NF-κB activity and hematopoiesis in the spleen. Similar to what was observed in the tibia (i.e. local response), NF-κB luciferase activity was also significantly elevated in either whole spleen cells or splenic CD4+ T cells (Fig. 2a,b). The number of spleen CD4+CD25+Foxp3+ TREG cells two days post-injection was also significantly reduced (Fig. 2c) whereas frequency of CD11b+Gr1+ cells that include but not limited to neutrophils and myeloid derived suppressive cells (MDSCs) was significantly increased (Fig. 2d). CD4+CD25+Foxp3+ TREG in the periphery including the blood and lymph nodes were also significantly decreased (Fig. S1). These findings suggest that PMMA particles elicit an acute inflammatory response that extends from pro-inflammatory marrow macrophages to systemic pro-inflammatory neutrophils, granulocytes and immunosuppressive MDSC cells. This further suggests that PMMA-induced changes in the marrow elicit systemic responses, likely cytokine-mediated signaling, to modulate immune responses in the spleen, lymph nodes and peripheral blood. Thus, this inflammatory cascade may initiate a vicious cycle that magnifies the severity of PMMA-induced osteolytic disease.
The increase of myeloid progenitors in response to PMMA is transient, while the reduction of regulatory T cells is prolonged
To further dissect the in vivo response of PMMA, we followed the changes of myeloid progenitor and regulatory T cell population in the bone marrow over time from 2 to 7 days after intra-tibial injection of PMMA. To monitor the systemic response, we extended our analyses to cellular changes in the spleen, lymph nodes and blood. We found that the significant increase of myeloid progenitor populations including LSKs, CMPs and GMPs rapidly diminished as early as 4 days post injection (Fig. 3a–c). In contrast, PMMA-induced decrease of TREG frequency remained persistent in the bone marrow and in the spleen of intra-tibially injected animals even after 7 days (Fig. 3d,e). Concomitantly, peripheral blood granulocytic neutrophils were also increased early after injection (2 days) and gradually declined back to the level similar to PBS injected animals (Fig. 3f). Finally, RelA-luciferase reporter activity, a measure of NF-κB activity, was also normalized systemically 7 days after injection, as no significant difference was found between PMMA- and PBS-injected mice in both the spleen and lymph nodes (Fig. S2a,b). However, immunostaining for Luciferase in bone sections from PMMA-injected tibias and luciferase activity of the bone marrow cells derived from PMMA injected tibias remained significantly increased (Fig. 3g,h). Consistent with the observed normalized systemic response, NF-κB activity also declined in femurs one-week post PMMA injection to adjacent tibias (Fig. 3h, marked with #). More importantly, when we performed functional assessment of osteoclast precursor numbers by ex vivo osteoclastogenesis assay, whole bone marrow cells from PMMA injected tibia and from adjacent femurs retained significantly higher osteoclastogenic potential than those from the PBS-injected controls (Fig. 3i). Since the numbers of myeloid progenitors were normal at this stage post PMMA injection, PMMA was most likely to potentiate and sensitize osteoclast progenitors versus increase their numbers at early stage. These results suggest that PMMA elicits a prolonged dampening of immunosuppression by TREGS, which may lead to unrestrained inflammatory response already triggered by significant increase in frequency of innate immune cells, e.g. macrophages. Although tibial injection resulted in temporal systemic inflammatory response, elevated NF-κB activity persisted at the injection site.
PMMA particles enhance expression of markers of pathogenic TH effector cells
The increased local and systemic inflammatory burden along with significant reduction in TREG frequency in response to PMMA exposure prompted us to further interrogate changes in T cell populations that may contribute to this pathology. In this regard, it has been shown previously that under inflammatory conditions, TREG cells may lose their immunosuppressive phenotype and assume a TH effector pathogenic phenotype19,20,21,22,23. This phenotypic switch depends on suppression or inactivation of Foxp3.
Supporting a potential pathogenic switch of TREG cells into TH effector cells, we found that 2 days post intra-tibial injection of PMMA, bone marrow derived CD4+ T effector cells possessed significantly higher percentage of Foxp3lo RORγT+ cells (Fig. 3j). Interestingly, utilizing Foxp3 GFP reporter mice in which expression of GFP and Foxp3 are coupled, not only did we observe reduced number of CD4+CD25+TREG in situ (bone marrow), extramedullary (spleen) and in periphery (blood and lymph node) upon intra-tibial injection of PMMA (Fig. S3a–d), it was also accompanied by increased mRNA expression of TH17 markers IL-17A, RORγt, RUNX1 and a large number of other inflammatory and osteoclastogenic factors including TNFα, RANKL and M-CSF (Fig. 4a–f). Similar results were also obtained from spleen TEFF cells post PMMA injection (Fig. S4a–f) particularly for RORγt/RUNX1/IL-17, but to a lesser extent for other effector/pro-inflammatory cytokines. These results show increased frequency of TEFF at the expense of TREG cells, suggesting potential T cell phenotype switching.
In vivo effect of PMMA on Treg can be recapitulated ex vivo
It is reasonable to postulate that the negative impact of PMMA on TREGS is mediated by secondary mechanisms as it mostly requires the engagement of T-cell receptor (TCR) signaling and antigen presentation by innate immune cells such as dendritic cells and macrophages24. However, mechano-transduction of T cells has been recently conceptualized and investigated25 and therefore, PMMA may also target TREG (and TEFF) in a direct manner. To gain further insights into the effect of PMMA on T cells including both TREGs and TEFF (direct vs. indirect mechanism), we conducted ex vivo cultures of whole bone marrow (WBM), whole spleen (WSpl) and whole lymph node (WLN) cells. Freshly isolated cells were cultured overnight in the presence of PMMA. These heterogeneous cultures were then stimulated with pan stimulator PMA/ionomycin for 5 hrs. Non-PMMA treated and -PMA/ionomycin stimulated cultured served as controls. Interestingly, in cultures from all 3 sources, percentage of CD3+CD4+CD25+ TREG was reduced by overnight treatment of PMMA, regardless of PMA/ionomycin stimulation (Fig. 4g–i). Reduction of TREGS was significantly greater in the WBM than in the WSpl and WLN cultures. Furthermore, percentage of IL-17A expressing cells in the CD3+CD4+CD25− TEFF population was significantly increased in WBM culture by PMMA treatment (Fig. 4j). WSpl derived TEFF cells also exhibited a trend of increased frequency of IL-17A+ population in the presence of PMMA (Fig. 4k), while the percentage of IL-17A+ T effector cells in the WLN culture was unaltered (Fig. 4l). Because WBMs and WSpls constitute significant proportion of myeloid cells (of the innate immune system; >40% for WBM and >5% for WSpl) compared to WLNs that is considered negligible proportion of myeloid cells (<1%), these data strongly suggest that secondary mechanisms (i.e. myeloid/T-cell interaction) most likely play a larger role in the effect of PMMA on TREG and TEFF cells.
PMMA particles impair the osteoclast suppressive function of TREGS
To explore the potential mechanisms by which PMMA affects TREG cell phenotype, we conducted co-culture and transwell studies (Fig. 5). CD4+CD25+ TREG cells were isolated by MACS and either co-cultured with BMMs or cultured in transwells with BMMs at the bottom of the plate. RANKL was added to BMMs to promote osteoclastogenesis followed by stimulating some wells with PMMA particles. Half of TREGS were treated with PMMA particles and the other half were left untreated. Additionally, 2,000U of human recombinant IL-2 was also supplemented to support immune suppressive function of all CD4+CD25+ TREG cells. As expected, adding TREG cells to BMMs in co-culture drastically inhibited RANKL stimulated osteoclastogenesis (Figs 5a and S5; compare corresponding panels I, II and III in both figures). Interestingly, whereas TREGs in co-culture with BMMs sufficiently interfered with PMMA-exacerbated osteoclastogenesis (Figs 5a and S5; corresponding panel IV), pre-treatment of TREGS with PMMA particles prior to co-culture with BMMs impaired TREGS anti-osteoclastogeneic function (Figs 5a and S5, panels V and VI compared with panel III). This impaired TREG function was detected in both co-culture and transwell (Fig. 5a, panels VIII and IX) conditions. Notably, when PMMA was added to the BMM compartment, TREGS were only partially able to inhibit the exacerbated osteoclastogenesis (Fig. 5a; panels IV and VIII). Interestingly, when we monitored mRNA expression of pro-inflammatory cytokines to assess reprogramming of TREGS, we observed a 12-fold increase of IL-17A expression in the TREG co-cultured with BMM stimulated with PMMA (Fig. 5b). On the other hand, we did not see significant changes of IL-17A expression or other inflammatory cytokines in the TREG cultured in transwells with BMMs undergoing PMMA exacerbated osteoclastogenesis (Fig. 5c and data not shown). These observations suggest that TREG cells, while partially affected by direct contact with PMMA, they require direct cell- cell contact with BMMs to achieve potent anti-osteoclastogenic potential. The data also suggest that TREGS secreted factors appear to play a role in their anti-osteoclastogenic function, albeit to a lesser degree than direct cell-cell contact. Most importantly, the data suggest that PMMA particles, through their action on TREGS, alter the phenotype of these cells from suppressors to IL-17A expressing T cells, suggesting a phenotypic switch.
PMMA particles impede the TREG anti-osteoclastogenic function by reprogramming TREGS through inhibition of neuropilin-1
To further delineate the mechanism affected by direct impact on T cells, qRT-PCR analysis was performed to survey mRNA expressions of genes that are important for the immune suppressive function of TREG and/or stability of TREG. To this end, we observed slight upregulation of Icos and GITR, and no change for Eos and CTLA4 in the presence of PMMA (Fig. S6a–f). We also did not see any changes of CTLA4 expression in TREG cells among all culture conditions (Fig. S5g,h). However, among the markers tested, only neuropillin-1 (Nrp-1) was downregulated in the TREG cells under all culture conditions with PMMA (Fig. 5d–f). Most notably, loss of Nrp-1 expression (resulting from exposure to PMMA) or by shRNA (Figs 5d and S5) rendered TREGS incapable of inhibiting osteoclastogenesis (Figs 5g and S5). Most interestingly, retroviral expression of Nrp-1 in TREGS halted the negative effect of PMMA on these cells and strongly stabilized and augmented their anti-osteoclastogenic function (Fig. 5h,i). These observations suggest that stable expression of Nrp-1 and its downstream signaling, stabilizes TREGS and supports its immunosuppressive function. The data further suggest that danger signals, such as PMMA particles, cause diminution of Nrp-1, which triggers TREG to undergo phenotypic switch to TEFF (i.e. exTREG), and exacerbate osteoclastogenesis.
Discussion
In this study we show that intra-tibial injection of PMMA particles increases the frequency of premature myeloid progenitors LSKs, granulocytic CD11b+Gr1+ cells and reduce frequency of CD4+CD25+ TREG cells. We further show that NF-κB reporter activity is significantly increased in vivo concurrent with inhibition of Foxp3 and elevated expression of TH17 transcription factors Runx1 and RORγt, leading to over production of inflammatory and osteoclastogenic factors such as TNFα, RANKL, M-CSF and IL-17A. These observations suggest that PMMA particles specifically attenuate TREG suppressive activity by inhibiting Foxp3 and switching the T cell phenotype from immunosuppressive to pathogenic.
In previous work, we have shown that PMMA particles exacerbate osteoclastogenesis in whole bone marrow cultures. Thus, it is reasonable to suggest that PMMA particles elicit an inflammatory microenvironment that alters hematopoiesis, highlighted by increased frequency of primitive progenitors such as LSKs. Concurrently PMMA particles induce conditions favorable for suppressing TREGS and promoting pathogenic TH17 cell through down regulation of Foxp3. Taken together, the sum of these changes lead to higher inflammatory and osteoclastogenic burdens. Indeed, Foxp3 is indispensable for TREG suppressive function. Mechanistically, Bettelli et al.26 found that Foxp3 associates with NFAT and NF-κB proteins and hinders their transcriptional activity. In fact, we and others have shown that myeloid and T cells derived from scurfy mice, which harbor inactive mutant Foxp3, exhibit high levels of NFAT and NF-κB activity, supporting the notion that Foxp3-expressing TREG cells suppress effector T helper cells16. In this study, using foxp3-GFP reporter mice, we provide direct evidence supporting TREG phenotype switch in response to the PMMA inflammatory signals. Specifically, we observe reduced number of CD4+CD25+ TREG in situ (bone marrow), extramedullary (spleen) and in periphery (blood and lymph node) upon intra-tibial injection of PMMA, concurrent with increased mRNA expression of TH17 markers RORγt, and IL-17A. Consistent with the paradigm that Foxp3 provides a transcriptional switch in T cell differentiation, it has been shown that T helper cells, specifically TH17, may originate from Foxp3+ TREG cells20. According to this study, inflammatory conditions render Foxp3 unstable leading to trans-differentiation of TREG cells that just lost Foxp3 expression, so-called exFoxp3, into TH17 pathogenic cells. It was further shown that this cell phenotype conversion was mediated by IL-6 and was associated with increased expression of IL-23R, RANKL, and Chemokine Receptor 6 (CCR6). More importantly, these exFoxp3 TH17 pathogenic cells were primarily located at sites on inflammation in arthritic joints. Our data suggest that PMMA particles destabilize TREGS through diminution of Foxp3.
Previous studies have shown that inflammatory conditions, such as synovial joint inflammation, destabilized foxp3 in TREGS leading to impaired cell function27, increased TH17 effector cells and unleashed the activity of the proinflammatory transcription factors NFAT and NF-κB. Multiple mechanisms are involved in the control of TREG stability28. These include PI3 kinase/Foxo29, Nrp-1/semaphorin-4a/Foxo3a30, GITR signaling31 and USP21 deubiquitinase32. Moreover, several other genes also participate in the balance between TREG and TH17 cells such as Foxo3a/TSC133,34, TCR and cytokine signaling integrated by Itk35, Tpl236, Eos37, TNF/TNFR238, Notch39, cooperated signaling between TCR and CD28/CTLA440. Interestingly, when we survey expression of these genes to determine the potential targets of PMMA-mediated TREG instability, we found that Nrp-1 expression was significantly downregulated. Thus, the mechanism underlying TREG reprogramming (e.g. reduced foxp3 expression) appears to involve down regulation of Nrp-1 via undefined stress or danger-like apparatus. As a result, NF-κB activity is elevated leading to induction of pro-inflammatory and osteoclastogenic factors including TNF, IL-17A, RANKL and M-CSF. This ultimately leads to increased osteoclastogenic burden through increased myeloid progenitor numbers and increased CD11b+Gr1+ myeloid cells. Furthermore, since Nrp-1 is a cell-surface protein/receptor, it is reasonable to speculate that PMMA particles interact with Nrp-1 and elicit mechano-transduction signals. In fact, our data indicate that primed spleen CD4+CD25+ TREG (stimulation with anti-CD3/CD28 beads for 72 hours) exhibited decreased Foxp3 protein expression in the presence of PMMA. Moreover, CD4+CD25− TEFF culture under the same conditions with much lower concentration of supplemented IL-2 (30U rather than 2,000) possessed higher RORγt+ population. Perhaps the most compelling evidence supporting this phenomenon is our finding that restoring expression of Nrp-1 via viral transduction stabilized the suppressive phenotype of TREGS and render these cells irresponsive to the inflammatory impact of PMMA particles. These data suggest that PMMA, beyond its conventional role in innate immunity (targeting macrophages; the precursors of osteoclasts), could directly impact the adaptive immunity with unknown mechanisms that require further investigation.
It is well documented that the CTLA4 is required for inhibition of osteoclastogenesis by TREG through direct cell- cell contact, at least in vitro. This TREG-osteoclast interaction is mediated by CTLA4 expressed by TREG and CD80/86 expressed by osteoclast. Not only CD80/86 osteoclast can escape inhibition by TREG, more convincingly CD80/86 deficient mice are osteopenic and exhibit increased osteoclast differentiation ex vivo. That said, we did not see any change in mRNA expression of CTLA4 in TREG co-cultured with BMM undergoing PMMA-exacerbated osteoclastogenesis. Ultimately, functional tests will be required with crucial reagents such as CTLA4-Fc to rule out whether PMMA can affect CTLA4-mediated (or GITR, PD-1 etc.) osteoclastogenesis suppression by TREG. It is important to note that murine CD4+CD8+FoxP3+ TREGS inhibit osteoclastogenesis in a cell contact-dependent manner with minor contribution by circulating anti-inflammatory cytokines41. In contrast, human FoxP3+TREGS induce alternative activation and inhibit osteoclast differentiation from peripheral blood monocytes independent of cell contact, yet in a TGFβ and IL-4-dependnet manner42,43. Although varying experimental conditions may contribute to this discrepancy, it would be of interest to simultaneously determine Nrp1 expression and function in these two systems.
Our co-culture experiments show that while TREGS potently inhibit osteoclastogenesis, exposure of TREGS to PMMA particles impair their anti-osteoclastogeneic function. Moreover, under co-culture conditions, PMMA particles induce robust expression of proinflammatory cytokines by TREG cells, suggesting that macrophage-TREG contact is crucial for this response. This observation, which is highlighted by secretion of IL-17A and TNFα by exTREG cells, is reminiscent of TREG phenotype switching and assuming an effector function. On the other hand, marginal osteoclast inhibition by TREGS in transwell conditions, suggest that PMMA particles may marginally induce secretion of soluble factors by macrophages that adversely influence secretion of repressors factors by TREG cells. These observations are consistent with the established paradigm wherein TH17 serve as osteoclastogenic TH cell type linking T cell activation with bone resorption through the interleukin IL23-IL17 axis44. Further delineation of the subsets of pathological effector T cells induced by orthopedic particles vs. rheumatoid diseases may have significant therapeutic implications.
In sum, our findings show that, in addition to its well documented direct effect on osteoclasts, PMMA particles also induce inflammatory osteolysis by modulating TREG cells. Specifically, we suggest that PMMA particles, by yet to be defined mechanism, down regulate Nrp-1 leading to reduced foxp3 and subsequent reprogramming TREGS into TH17 pathogenic cells. These cells express pro-inflammatory and osteoclastogenic factors that directly expand the osteoclast progenitor population and exacerbate osteoclastogenesis. Our findings identify the Nrp-1 pathway as a potential therapeutic target to combat inflammatory osteolysis.
Materials and Methods
Study design and statistical analysis
Data is expressed as mean ± SD of at least three independent experiments. Typically, each experimental design includes triplicates of each condition. *p < 0.05; **p < 0.005 using Student t-test. Our experimental design is based on reaching 0.05 significance and effect size of 25%. With desired difference of 80%, we calculated sample size as 6 mice per group. Experiments were conducted with male and female mice at equal proportions. There are no reported osteolytic differences between mouse sexes.
Mice
Approval for using animals was obtained from Washington University School of Medicine Institutional Animal Care and Use Committee in accordance with NIH guidelines prior to performing this study. Mice were housed at the Washington University School of Medicine barrier facility. NF-κB reporter (NGL) mice were purchased from Jackson Laboratories to monitor in vivo NF-κB activity longitudinally during disease progression as well as ex vivo studies including cultures of macrophages/monocytes, proinflammatory T helper cells and co-cultures. Foxp3-GFP reporter mice were kindly provided by Dr. John DiPersio’s lab (Washington University) and were originally from Jackson Laboratories (Bar Harbor, ME USA). The Foxp3 reporter mice were used to perform hematological diagnosis by flow cytometry for TREG cells, myeloid populations and progenitors after manipulation.
Chemicals and reagents
PMMA particles (Polyscience) were sterilized before injection by washing with 70% EtOH for three times followed by 3 times in PBS and finally resuspended in PBS (0.2 mg/ml for in vitro studies and 20 ul per injection of 5 mg/ml in vivo). All FACS antibodies, buffers and reagents were purchased from either BD Biosciences, eBioScience/Thermo Fisher or BioLegend.
Flow cytometry
To analyze myeloid progenitor in the bone marrow, freshly flushed WBM cells were sequentially stained with PE conjugated anti-CD34 and Brilliant Blue 421 conjugated anti-CD16/32 antibodies for 30 minutes on ice, and biotin conjugate lineage antibody cocktail (anti-CD2, -CD3ε -IL7R, -Ter119 and –B220) and PerCP Cy5.5 anti-CD11b, PE Cy7 anti-CD115 (c-fms), Alexa 700 anti-Ly6G and APC H7 anti-CD117 (c-kit) antibodies for additional 30 minutes. After washed with FACS buffer, antibody labeled cells were stained with Brilliant Blue 510 conjugated streptavidin for 20 minutes before analyzed on flow cytometer. To phenotype T cells, whole bone marrow (WBM) or whole spleen (WSpl) cells were stained with PE anti-CD4, PerCP Cy5.5 anti-CD44, APC anti-CD62L, PE Cy7 anti-CD3ε, APC e780 anti-CD8a and Brilliant Blue 421 anti-CD25 for 30 minutes on ice.
Intra-tibial injection mouse model to test acute/short-term cellular response to PMMA
Mice were anesthetized with 100 μl of ketamine/xylazine cocktail per 10 grams of body weight. Skin above the knee cap was wetted with 70% EtOH to sterilize and visualize the injection site. To allocate the growth plate of tibia, patellar ligament was used as a landmark. 27G needle was inserted above the patellar ligament until encountering resistance. Drill motion was applied to the needle until the growth plate was penetrated. 20 μl of PBS or PMMA solution (5 mg/ml) was released into the bone marrow cavity slowly to avoid back flash.
Cell Isolation and culture
Bone marrow macrophages/monocytes (BMMs)
Bone marrow cells were harvested from femurs and tibias. After cell numbers were determined by hemacytometer counts, cells were cultured in DMEM supplemented with 10% FBS and 10% CMG that contained M-CSF.
CD4+CD25+TREG
CD4+CD25+ cells were isolated from mouse spleens by MACS according to manufacturer’s protocol. After isolation, purity was checked by FACS before cultured with RPMI 1640 medium supplemented with 10% FBS, sodium pyruvate, non-essential amino acids, glutamine, 10 mM HEPES and 50 μM β-mercaptoethanol. To activate TREG at phtsiological level, Dynabeads were added at bead-to-cell ratio of 2:1 and 2,000 U of recombinant IL-2 was also supplemented.
CD4+CD25− T effector cells
CD4+CD25− cells were obtained during CD4+CD25+TREG cell isolation. TEFF cell culture was supplemented with 30U IL-1 and anti-CD3/CD28 Dynabeads at bead-to-cell ratio of 1:1 for activation and expansion.
Spleen and lymph nodes
To isolate single cells from the spleen or inguinal lymph nodes, tissues were carefully dissected, placed in ice-cold FACS buffer, grinded using the back end of a 3-ml syringe before passing through a sterile 70 micro filter. After red blood cell lysis, mononucleated cells were then subjected to either FACS analysis, MACS isolation for CD4+ T cells or TREGS, or luciferase activity assay.
BMM-TREG co-culture and transwell culture for osteoclastogenesis assay
BMMs were prepared as aforementioned. In vitro expanded TREG cells were generated by culturing MACS-isolated splenic naïve CD4+ T cells in TREG cell differentiation media (R&D Systems), either with or without the presence of PMMA particles for 2 days before directly added onto BMMs for co-culture or into transwell inserts on top of BMMs for transwell culture at BMM-TREG ratio of 5:1 or 10:1.
Luciferase assay
Luciferase assay was conducted according to the manufacturer’s protocol (Promega). Briefly, freshly isolated or MACS purified cells were lysed in passive cell lysis buffer After protein concentration was determined by BCA assay, 20 μg of protein was used from each lysate with Luciferase Assay Reagent to measure the light produced by a luminometer.
Nrp-1 knockdown
The lentiviral sgRNA vectors and sequences for targeting Nrp-1 were designed by the Genome Center at Washington University. The lentiviral sgRNA bearing a scrambled, non-specific sequence was used as control. To generate lentiviral particles, each vector was co-transfected into HEK cells together with packaging and helper vectors, replenished with fresh media on the next day. Conditioned media containing lentiviral particles was collected after 2 days, concentrated, and stored at −80 upon use. To transduce T cells, 3 million spleen derived mouse naive CD4+ T cells were incubated with 300 ul concentrated lentiviral stock in the presence of 10 ug/ml polybrene overnight, washed and replenished with TREG cell differentiation media, in the presence or absence of PMMA particles for 2 days before proceeding to co-culture experiment with BMMs.
Nrp-1 expression (Gain of function)
To achieve expression of Nrp-1 in Tregs, retroviral vector (namely PINCO) carrying mouse wildtype Nrp-1 gene was purchased from Addgene (https://www.addgene.org/browse/gene/18186/). To generate retroviral particles, 5 ug of each PINCO vector plasmid was transfected into 4 millions of PLAT-E cells plated on p100 TC dish 1 day prior. After 8 hours, transfected PLAT-E cells were replenished with RPMI media supplemented with 10% FBS and 50 uM b-ME. Supernatants were then collected after 48 hours of culture and served as retroviral stocks, which were kept on ice until use. To transduce TREGS, 1 millions of freshly MACS-isolated naïve CD4+ T cells from mouse spleen were incubated overnight with 3 ml of retroviral stock supplemented with reagents from the TREG Cell Differentiation Kit (R&D Systems) and 10ug/ml of polybrene. Transduced naïve CD4+ T cells were then washed and replenished with TREG differentiation media and cultured for 2 additional days before subjected to co-culture with osteoclast progenitors for in vitro osteoclastogenesis assay. To condition PINCO-Nrp1 transduced TREGS, 0.1 mg/ml PMMA particles were added to culture.
Gene expression analysis by RT-qPCR
Cells isolated by MACS or harvested freshly from cultures were lysed in Trizol reagent. Total RNAs were isolated and cDNA synthesis was performed according to the manufacturers’ protocol. 20 μl of each cDNA sample was diluted by 10-fold with Tris-EDTA buffer and 4 μl of diluted cDNA sample was used for 10 μl qPCR reaction with SYBR Green PCR mix. Primers for assessing cytokine expressions (IL-10, IL-17A, M-CSF, RANKL and TNFα) were described previously (Chen et al. 2015). Other primer sequences are listed as follows – For CTLA4, forward primer 5′-GCTTCCTAGATTACCCCTTCTGC-3′, reverse primer 5′-CGGGCATGGTTCTGGATCA-3′; for Dbc1, forward primer 5′-GTATCTCAGTGCAGCCCTCC-3′, reverse primer 5′-AACGGGCAAACTCCCTGTAT-3′; for Eos, forward primer 5′-TCTGGACCACGTCATGTTCAC-3′, reverse primer 5′-ACGATGTGGGAAGAGAACTCATA-3′; for Foxp3, forward primer 5′-ATTGAGGGTGGGTGTCAGGA-3′, reverse primer 5′-ACAGCATGGGTCTGTCTTCTC-3′; for GATA3, forward primer 5′-CCATTACCACCTATCCGCCC-3′, reverse primer 5′-TTCACACACTCCCTGCCTTC-3′, for GITR, forward primer 5′-CCACTGCCCACTGAGCAATAC, reverse primer 5′-GTAAAACTGCGGTAAGTGAGGG-3′; for Helios, forward primer 5′-GAGCCGTGAGGATGAGATCAG-3′; reverse primer 5′-CTCCCTCGCCTTGAAGGTC-3′; for Icos, forward primer 5′-ATGAAGCCGTACTTCTGCCG-3′, reverse primer 5′-CGCATTTTTAACTGCTGGACAG-3′; for Nrp-1, forward primer 5′-GACAAATGTGGCGGGACCATA-3′, reverse primer 5′-TGGATTAGCCATTCACACTTCTC-3′; for RUNX1, forward primer 5′-CAGGCAGGACGAATCACACT-3′, reverse primer 5′- CTCGTGCTGGCATCTCTCAT-3′; for RORγT, forward primer 5′-TACCCTACTGAGGAGGACAGG, reverse primer 5′-AATGGGGCAGTTCTGCTGAC-3′; for Tbet, forward primer 5′-GTCTGGGAAGCTGAGAGTCG-3′, reverse primer 5′-ACATTCGCCGTCCTTGCTTA-3′, for Tpl2, forward primer 5′-ATGGAGTACATGAGCACTGGA-3′, reverse primer 5′-GGCTCTTCACTTGCATAAAGGTT-3′; for Ubc 13, forward primer 5′-ACAAGAGCAGAGGCCGAAC′3′, reverse primer 5′-GCAAACGCTGGGTTTCCTTG-3′.
Immunohistochemistry
At the end of experiments, mouse long bones were harvested and fixed in 10% neutral buffered formalin for 24 hours followed by decalcification in Immunocal (StatLab, McKinney, TX) for 3 days. Tissues were then processed, embedded into paraffin, and sectioned 5 mm thick. For immunohistochemistry, sections were de-paraffinized and rehydrated using xylene followed by ethanol gradient. Antigen retrieval was performed by incubating samples at 60 degrees celsius in Citrate buffer (pH 6.0) followed by quenching of endogenous peroxidase activity with 3% H2O2. Sections were blocked using DAKO solution with background reducing components. Sections were incubated overnight with a 1:200 dilution of anti-Luciferase (Novus), anti-Nrp1 (Novus) or anti-FoxP3 (Novus) antibody. Sections were rinsed in phosphate-buffered saline (PBS) followed by a 1:1000 dilution of biotinylated secondary antibody for one hour. Post-secondary antibody incubation, the sections were incubated with stereptavidin-HRP (2 ug/ml) for 20 min. After extensive washing with PBS, sections were developed using Impact DAB kit (Vector Biolabs).
References
Abu-Amer, Y., Darwech, I. & Clohisy, J. C. Aseptic loosening of total joint replacements: mechanisms underlying osteolysis and potential therapies. Arthritis Res Ther 9(Suppl 1), S6 (2007).
Cobelli, N., Scharf, B., Crisi, G. M., Hardin, J. & Santambrogio, L. Mediators of the inflammatory response to joint replacement devices. Nat Rev Rheumatol 7, 600–608 (2011).
Schmalzried, T. P., Jasty, M. & Harris, W. H. Periprosthetic bone loss in total hip arthroplasty. Polyethylene wear debris and the concept of the effective joint space. J Bone Joint Surg Am 74, 849–863 (1992).
Hirakawa, K., Bauer, T. W., Stulberg, B. N. & Wilde, A. H. Comparison and quantitation of wear debris of failed total hip and total knee arthroplasty. Journal of biomedical materials research 31, 257–263 (1996).
Margevicius, K. J., Bauer, T. W., McMahon, J. T., Brown, S. A. & Merritt, K. Isolation and characterization of debris in membranes around total joint prostheses. J Bone Joint Surg Am 76, 1664–1675 (1994).
al-Saffar, N. & Revell, P. A. Pathology of the bone-implant interfaces. J Long Term Eff Med Implants 9, 319–347 (1999).
Revell, P. A., al-Saffar, N. & Kobayashi, A. Biological reaction to debris in relation to joint prostheses. Proc Inst Mech Eng H 211, 187–197 (1997).
Landgraeber, S., Jager, M., Jacobs, J. J. & Hallab, N. J. The pathology of orthopedic implant failure is mediated by innate immune system cytokines. Mediators Inflamm 2014, 185150 (2014).
Pearson, M. J. et al. The effects of cobalt-chromium-molybdenum wear debris in vitro on serum cytokine profiles and T cell repertoire. Biomaterials 67, 232–239 (2015).
Hopf, F. et al. CD3+ lymphocytosis in the peri-implant membrane of 222 loosened joint endoprostheses depends on the tribological pairing. Acta Orthop 88, 642–648 (2017).
DuPage, M. & Bluestone, J. A. Harnessing the plasticity of CD4(+) T cells to treat immune-mediated disease. Nat Rev Immunol 16, 149–163 (2016).
Sandhu, J., Waddell, J. E., Henry, M. & Boynton, E. L. The role of T cells in polyethylene particulate induced inflammation. J Rheumatol 25, 1794–1799 (1998).
Childs, L. M., Goater, J. J., O'Keefe, R. J. & Schwarz, E. M. Effect of anti-tumor necrosis factor-alpha gene therapy on wear debris-induced osteolysis. J Bone Joint Surg Am 83-a, 1789–1797 (2001).
Taki, N. et al. Polyethylene and titanium particles induce osteolysis by similar, lymphocyte-independent, mechanisms. J Orthop Res 23, 376–383 (2005).
Lin, T. H. et al. Exposure of polyethylene particles induces interferon-gamma expression in a natural killer T lymphocyte and dendritic cell coculture system in vitro: a preliminary study. Journal of biomedical materials research. Part A 103, 71–75 (2015).
Chen, T. H., Swarnkar, G., Mbalaviele, G. & Abu-Amer, Y. Myeloid lineage skewing due to exacerbated NF-kappaB signaling facilitates osteopenia in Scurfy mice. Cell Death Dis 6, e1723 (2015).
Clohisy, J. C., Hirayama, T., Frazier, E., Han, S. K. & Abu-Amer, Y. NF-kB signaling blockade abolishes implant particle-induced osteoclastogenesis. J Orthop Res 22, 13–20 (2004).
Clohisy, J. C., Yamanaka, Y., Faccio, R. & Abu-Amer, Y. Inhibition of IKK activation, through sequestering NEMO, blocks PMMA-induced osteoclastogenesis and calvarial inflammatory osteolysis. J Orthop Res 24, 1358–1365 (2006).
Li, L., Patsoukis, N., Petkova, V. & Boussiotis, V. A. Runx1 and Runx3 are involved in the generation and function of highly suppressive IL-17-producing T regulatory cells. PLoS One 7, e45115 (2012).
Komatsu, N. et al. Pathogenic conversion of Foxp3+ T cells into TH17 cells in autoimmune arthritis. Nat Med 20, 62–68 (2014).
Yu, F., Sharma, S., Edwards, J., Feigenbaum, L. & Zhu, J. Dynamic expression of transcription factors T-bet and GATA-3 by regulatory T cells maintains immunotolerance. Nat Immunol 16, 197–206 (2015).
Kluger, M. A. et al. RORgammat(+)Foxp3(+) Cells are an Independent Bifunctional Regulatory T Cell Lineage and Mediate Crescentic GN. J Am Soc Nephrol 27, 454–465 (2016).
van der Veeken, J. et al. Memory of Inflammation in Regulatory T Cells. Cell 166, 977–990 (2016).
Perry, J. S. & Hsieh, C. S. Development of T-cell tolerance utilizes both cell-autonomous and cooperative presentation of self-antigen. Immunol Rev 271, 141–155 (2016).
Ma, Z. & Finkel, T. H. T cell receptor triggering by force. Trends in immunology 31, 1–6 (2010).
Bettelli, E., Dastrange, M. & Oukka, M. Foxp3 interacts with nuclear factor of activated T cells and NF-ΰB to repress cytokine gene expression and effector functions of T helper cells. Proceedings of the National Academy of Sciences of the United States of America 102, 5138–5143 (2005).
Nie, H. et al. Phosphorylation of FOXP3 controls regulatory T cell function and is inhibited by TNF-alpha in rheumatoid arthritis. Nat Med 19, 322–328 (2013).
Overacre, A. E. & Vignali, D. A. T(reg) stability: to be or not to be. Curr Opin Immunol 39, 39–43 (2016).
Merkenschlager, M. & von Boehmer, H. PI3 kinase signalling blocks Foxp3 expression by sequestering Foxo factors. J Exp Med 207, 1347–1350 (2010).
Delgoffe, G. M. et al. Stability and function of regulatory T cells is maintained by a neuropilin-1-semaphorin-4a axis. Nature 501, 252–256 (2013).
Ephrem, A. et al. Modulation of Treg cells/T effector function by GITR signaling is context-dependent. Eur J Immunol 43, 2421–2429 (2013).
Li, Y. et al. USP21 prevents the generation of T-helper-1-like Treg cells. Nat Commun 7, 13559 (2016).
Khatri, S., Yepiskoposyan, H., Gallo, C. A., Tandon, P. & Plas, D. R. FOXO3a regulates glycolysis via transcriptional control of tumor suppressor TSC1. J Biol Chem 285, 15960–15965 (2010).
Park, Y. et al. TSC1 regulates the balance between effector and regulatory T cells. J Clin Invest 123, 5165–5178 (2013).
Gomez-Rodriguez, J. et al. Itk-mediated integration of T cell receptor and cytokine signaling regulates the balance between Th17 and regulatory T cells. J Exp Med 211, 529–543 (2014).
Xiao, Y. et al. TPL2 mediates autoimmune inflammation through activation of the TAK1 axis of IL-17 signaling. J Exp Med 211, 1689–1702 (2014).
Rieder, S. A. et al. Eos Is Redundant for Regulatory T Cell Function but Plays an Important Role in IL-2 and Th17 Production by CD4+ Conventional T Cells. J Immunol 195, 553–563 (2015).
Miller, P. G., Bonn, M. B. & McKarns, S. C. Transmembrane TNF-TNFR2 Impairs Th17 Differentiation by Promoting Il2 Expression. J Immunol 195, 2633–2647 (2015).
Coutaz, M. et al. Notch regulates Th17 differentiation and controls trafficking of IL-17 and metabolic regulators within Th17 cells in a context-dependent manner. Sci Rep 6, 39117 (2016).
Holt, M. P., Punkosdy, G. A., Glass, D. D. & Shevach, E. M. TCR Signaling and CD28/CTLA-4 Signaling Cooperatively Modulate T Regulatory Cell Homeostasis. J Immunol 198, 1503–1511 (2017).
Zaiss, M. M. et al. Treg cells suppress osteoclast formation: a new link between the immune system and bone. Arthritis Rheum 56, 4104–4112 (2007).
Tiemessen, M. M. et al. CD4+ CD25+ Foxp3+ regulatory T cells induce alternative activation of human monocytes/macrophages. Proc Natl Acad Sci USA 104, 19446–19451 (2007).
Kim, Y. G. et al. Human CD4+ CD25+ regulatory T cells inhibit the differentiation of osteoclasts from peripheral blood mononuclear cells. Biochem Biophys Res Commun 357, 1046–1052 (2007).
Sato, K. et al. Th17 functions as an osteoclastogenic helper T cell subset that links T cell activation and bone destruction. J Exp Med 203, 2673–2682 (2006).
Acknowledgements
This work was supported by NIH/NIAMS R01-AR049192, R01-AR054326, R01-AR072623, (to YA), Biomedical grant #86200 from Shriners Hospital for Children (YA), P30 AR057235 NIH Core Center for Musculoskeletal Biology and Medicine (to YA) and NIH/NIAMS R01-AR064755 and R01-AR068972 (to GM).
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Y.A. conceived, developed and supervised the project and finalized the manuscript. T.C. performed experiments, presented and analyzed data, participated in development of the project and significantly contributed to manuscript writing. G.S., M.A. and participated in performing experiments and data analysis. G.M. participated in experimental design, data analysis and manuscript preparation.
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Chen, T.HP., Arra, M., Mbalaviele, G. et al. Inflammatory Responses Reprogram TREGS Through Impairment of Neuropilin-1. Sci Rep 9, 10429 (2019). https://doi.org/10.1038/s41598-019-46934-x
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DOI: https://doi.org/10.1038/s41598-019-46934-x
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