Introduction
Rheumatoid arthritis (RA) is a systemic chronic inflammatory disorder associated with persistent and destructive synovitis leading to cartilage and bone erosion. The underlying cause of RA is unknown; however, the pathogenesis of RA is thought to be the result of complex cell to cell interactions between amongst others, T cells, macrophages and fibroblasts. In established disease, the preponderance of IFNγ-expressing and paucity of IL-4-expressing T cells,
in situ and
ex vivo, had until recently led to the description of RA as an immune mediated inflammatory disease associated with a predominantly T helper type-1 (Th1)-like cytokine profile [
1‐
3].
More recently, effector T cells (Th17 cells), that produce interleukin-17A (IL-17) [
4,
5] and that are functionally distinct from Th1 and Th2 helper T cells, have been identified in mice and subsequently in humans [
6]. Th17 cells have an important role in the clearance of extracellular bacteria and fungi, but also appear to play a pathogenic role in several inflammatory and autoimmune diseases. In experimental animal models, IL-17-producing T cells are involved in the pathogenesis of experimental autoimmune encephalomyelitis (EAE), collagen-induced arthritis (CIA), colitis and psoriasis [
7‐
9].
In mice, the development of Th17 cells is driven by the transcription factor retinoic acid-related orphan receptor γt (RORγt). Differentiation from naïve T cells requires TGFβ, IL-1, and IL-6 [
10,
11]. In humans, the origin of Th17 cells and the factors that regulate their development remain controversial, but like murine Th17 cells, IL-1 and IL-6 are essential and it is likely that TGF-β also plays a role. Both murine and human Th17 cells require IL-23 for their expansion and survival. Th17 differentiation is not only regulated by cytokines but also by environmental and dietary factors, such as aryl hydrocarbons [
12,
13] and vitamin D
3 [
14,
15]. In addition to IL-17, Th17 cells have been shown to produce IL-21, IL-22, TNFα and IFNγ [
16].
In RA, IL-17 has been detected in synovial fluid (SF) and synovium [
17‐
21]. Its expression is associated with inflammation and joint destruction, as well as with production of IL-1β and TNFα. In addition to stimulating the production of these proinflammatory cytokines, IL-17 acts synergistically by amplifying their effects [
22,
23]. We have previously identified IL-17-producing T cells within SF and synovial tissue, and demonstrated that RA synovial fibroblasts treated with IL-17 and TNFα promote the survival and functional lifespan of neutrophils, contributing to the increased number of neutrophils observed in the rheumatoid synovial microenvironment [
23]. Based upon the combined evidence for a role of IL-17 in inflammation, targeting of IL-17 is now being tested as a new therapeutic strategy for the treatment of RA [
24].
However, relatively little is known about the phenotype, cytokine profile and frequency of Th17 cells in the synovial environment and how they relate to RA disease activity. Two reports have shown that the frequency of Th17 cells was increased in the blood of RA patients compared with healthy donors [
15,
25], whilst Shahrara
et al. demonstrated that the percentage of Th17 cells was higher in RA SF compared with normal and RA peripheral blood [
15,
25,
26]. In addition, IL-17-producing T cells were shown to be enriched in the joints of children with juvenile idiopathic arthritis [
27]. In contrast, Yamada
et al. reported fewer Th17 cells in the joints of RA patients compared to peripheral blood [
28]. In light of these conflicting data, we investigated the phenotype and frequency of IL-17-producing T cells in the blood, SF and synovial tissue of patients with RA, examining the cytokine profile of this population and correlation with disease activity.
Materials and methods
Patients
Paired blood and SF was obtained from 14 RA patients (nine female) meeting the 1987 ACR criteria [
29] with a median age of 60.5 years (interquartile range (IQR) 52 to 69.5), and a median DAS28 of 5.55 (IQR 4.41 to 6.11). Paired blood and synovium was obtained from 10 RA patients (nine female) meeting the 1987 ACR criteria [
29] with a median age of 56 years (IQR 48 to 71), and a median DAS28 of 4.75 (IQR 4.08 to 5.95) undergoing joint replacement surgery. The clinical details of patients who donated blood and SF or synovium are given in Table
1. Peripheral blood samples were obtained from an additional 20 RA patients (10 female) giving a total of 44 RA blood samples analysed. Blood from 13 healthy control (HC) donors (six female) with a median age of 56 years (IQR 51.5 to 62) was obtained. Details of the 44 RA patients for whom analysis of blood was conducted are given in Table
2. Ethical approval for this study was given by the local research ethics committee and all subjects gave written informed consent.
Table 1
Characteristics of RA patients for whom analysis of IL-17-positive CD4 T cells in paired blood and synovial fluid (top), and paired blood and synovium (bottom) was performed.
1 | +ve | +ve | <1 | MTX, HCQ | N | N | 39 | 15 | 6.20 | 1.95 | 2.52 |
2 | +ve | +ve | 2 | MTX, HCQ | N | N | 61 | 8 | 7.01 | 1.09 | 0.82 |
3 | +ve | +ve | 1 | N | N | N | 21 | 7 | 4.18 | 2.36 | 2.17 |
4 | +ve | -ve | 23 | MTX | N | N | 18 | 11 | 5.83 | 0.73 | 0.79 |
5 | +ve | -ve | 45 | MTX | N | N | 60 | 11 | 5.27 | 0.63 | 0.53 |
6 | +ve | +ve | 5 | MTX, SSZ | N | N | 69 | 93 | 5.48 | 2.34 | 2.84 |
7 | +ve | +ve | 4 | N | Y | Y | 28 | 30 | 3.51 | 3.48 | 1.17 |
8 | +ve | +ve | <1 | MTX, HCQ | N | Y | 63 | 72 | 6.14 | 1.59 | 1.44 |
9 | +ve | +ve | 5 | N | Y | Y | 32 | 12 | 5.62 | 1.30 | 7.90 |
10 | +ve | +ve | <1 | MTX | Y | N | 80 | 71 | 6.08 | 0.73 | 5.18 |
11 | -ve | +ve | 1 | N | N | N | 10 | 15 | 5.76 | 0.86 | 3.48 |
12 | +ve | +ve | 5 | MTX | Y | Y | 24 | 24 | 4.42 | 1.06 | 1.06 |
13 | -ve | -ve | 6 | HCQ | N | N | 81 | 92 | 4.39 | 0.37 | 4.45 |
14 | +ve | +ve | 1 | MTX | N | Y | 17 | 16 | 4.48 | 0.49 | 0.46 |
| | | | Treatment
| | | | % CD3+CD4+
IL17+
|
Subject
| RF
| ACPA
| Disease duration, years
| DMARD
| Anti-TNF
| Steroid
| ESR, mm/hr
| CRP, mg/l
| DAS28
(ESR)
| PBMC
| SVMC
|
1 | +ve | +ve | 16 | N | Y | N | 20 | 20 | 3.83 | 0.77 | 0.55 |
2 | +ve | +ve | 4 | N | Y | Y | 13 | 9 | 4.95 | 0.57 | 0.48 |
3 | +ve | +ve | 5 | N | Y | Y | 13 | 3 | 4.50 | 1.63 | 0.78 |
4 | -ve | +ve | 8 | MTX | Y | N | 12 | 0 | 3.57 | 1.49 | 1.08 |
5 | +ve | +ve | 20 | N | N | Y | 89 | 24 | 6.03 | 2.63 | 0.91 |
6 | +ve | +ve | 23 | N | N | Y | 45 | 57 | 5.86 | 0.08 | 0.24 |
7 | +ve | +ve | 20 | SSZ | N | N | 31 | 11 | 4.33 | 0.73 | 0.81 |
8 | +ve | +ve | 5 | N | Y | Y | 15 | 3 | 4.55 | 0.29 | 1.17 |
9 | -ve | -ve | 15 | N | Y | N | 115 | 22 | 6.19 | 1.37 | 0.99 |
10 | -ve | +ve | 1 | LEF | N | N | 10 | 15 | 5.76 | 1.65 | 0.48 |
Table 2
Summary of RA patients for whom analysis IL-17-positive CD4 T cells in the blood was conducted
RA patients (n) | 44 |
Age, years (median (IQR)) | 56 (50 to 65.5) |
Sex, female (n) | 28 |
Disease duration, years (median (IQR)) | 3.5 (1.0 to 5.5) |
RF positive (n) | 32 |
ACPA positive (n) | 30 |
ESR, mm/hr (median (IQR)) | 24 (10 to 40) |
CRP, mg/ml (median (IQR)) | 11 (<5 to 23) |
DAS28 (ESR) (median (IQR)) | 5.15 (4.01 to 6.17) |
% IL17-positive CD4 T cells (median (IQR)) | 1.08 (0.60 to 1.64) |
% IL17-positive CD45RO CD4 T cells (median (IQR)) | 1.10 (0.47 to 1.79) |
Peripheral blood and synovial fluid cell preparation
Peripheral blood mononuclear cells (PBMC) and SF mononuclear cells (SFMC) were isolated by density gradient centrifugation on Ficoll-paque™-Plus (GE Healthcare, Amersham, UK), washed twice with RPMI-1640 medium (Sigma-Aldrich, St Louis, MO, USA), counted using a Neubauer hemocytometer and resuspended at 1 × 106 cells/ml in fresh medium.
Synovial tissue dissociation
RA synovium was cut into small pieces and washed in RPMI-1640 medium. The tissue suspension was transferred into a Stomacher® 400 Circulator Bag (Seward Ltd, Worthing, UK), heat sealed, placed in a Stomacher® 400 circulator (Seward Ltd) and run at 230 rpm for five minutes. The contents of the bag were removed and passed through a BD Falcon 70 mm nylon cell strainer. The filtered cell suspension was then layered onto ficoll and synovial tissue mononuclear cells (SVMC) isolated from the buffy coat following centrifugation as above.
Flow cytometric analysis
Monoclonal antibodies (mAb) and reagents used for flow cytometric analysis were phycoerythrin (PE)-conjugated anti-IL-17A mAb (eBioscience, San Diego, CA, USA), anti-IL-4 mAb (BD Biosciences, Franklin Lakes, NJ, USA), anti-CD4 mAb (Immunotools, Friesoythe, Germany); fluorescein isocyanate (FITC)-conjugated anti-interferon-γ mAb (Invitrogen, Paisley, UK), anti-IL-6 mAb (eBioscience), anti-TNFα mAb (BD Biosciences), anti-IL-10 mAb (eBioscience), anti-CD4 mAb (Immunotools), anti-CD45RO mAb (Dako, Fort Collins, CO, USA), anti-IL-23R mAb (R&D Systems, Abingdon, UK); allophycoerythrin (APC)-conjugated anti-IL-22 mAb (R&D Systems), anti-CD45RA mAb (Southern Biotech, Birmingham, AL, USA), anti-CD8 mAb (Biolegend, San Diego, CA, USA); pacific blue (PcB)-conjugated anti-CD4 mAb (eBioscience); PE-Cy7-conjugated anti-CD3 mAb (eBioscience); PE-Cy647-conjugated anti-CD14 mAb (Immunotools). Stained cells were run on a Cyan flow cytometer (Dako), and the data analysed using Summit v4.3 software (Dako).
Intracellular staining of cytokines
Mononuclear cells were stimulated with 100 ng/ml of phorbol myristate acetate (PMA) (Sigma-Aldrich) and 1 μg/ml of ionomycin (Sigma-Aldrich) for three hours together with 2 μg/ml of brefeldin A (Sigma-Aldrich). This time-point was identified prior to this study, in a time-course experiment, as the optimum for intracellular cytokine measurement of IL-17 and IFNγ (the prime discriminators between Th1/Th17 cells) (data not shown). After surface staining, intracellular staining was performed using a Caltag fixation and permeabilisation kit (Invitrogen) according to manufacturer's instructions.
Statistical analysis
Correlations were examined using Spearman rank test. For comparisons of unpaired and paired samples, the Mann-Whitney U test and Wilcoxon signed rank test were used respectively, with two-tailed P-values. Medians and interquartile ranges (IQR) are reported. P-values less than 0.05 were considered significant.
Discussion
There is considerable evidence, from both animal and human studies, that IL-17 plays a role in inflammatory arthritis [
17‐
21,
34]. Mechanistically, IL-17 promotes osteoclastogenesis, partly through upregulation of RANKL expression [
35], and also synergises with other inflammatory cytokines, such as TNFα and IL-1, to amplify their effects [
22,
23]. These observations have led to the development of new therapeutic strategies aimed at targeting IL-17 or suppressing Th17 cells [
24]. However, recent studies of the frequency of Th17 cells in RA patients have yielded conflicting data. Furthermore, the profile of cytokines produced by these cells
ex vivo and their relationship with disease activity has not been well defined. Some studies have only examined this population in the blood of RA patients [
25], whilst only two studies have examined these cells in SF or synovium [
26,
28].
We found no significant difference in the frequency of IL-17-producing CD4 T cells in the blood of RA patients and healthy controls. This contrasts with data from the study of Shen
et al. (which looked at blood from 12 RA patients) but is consistent with data from Yamada
et al. (which looked at blood from 123 RA patients and mononuclear cells isolated from the joints of 12 patients) [
25,
28]. The study by Shen
et al., whilst primarily focussed on Th17 cells in ankylosing spondylitis, demonstrated an increased frequency of IL-17-producing CD4 T cells in RA patients blood compared to healthy controls which correlated with both CRP and swollen joint counts (SJC). We would suggest that the larger sample sizes in our study (blood examined from 44 RA patients) and the study of Yamada
et al. may provide a broader representation of what is recognised to be a very heterogeneous disease.
Our observation of a small but significant increase in the frequency of IL-17-producing CD4 T cells in SF compared to peripheral blood of RA patients, and the same for the frequency of memory CD4 T cells (CD45RO-positive) producing IL-17, are consistent with data from Shahrara
et al. [
26] but differ from the findings of Yamada
et al. [
28]. It should be noted however that Yamada
et al. studied cells from the joints of only 12 RA patients and data from synovial fluid (
n = 8) and synovial tissue (
n = 4) were grouped together for analysis; this may be relevant in the context of our observation that the percentage of Th17 cells was lower in synovial tissue than in the blood of RA patients whereas the reverse was seen when synovial fluid was compared with blood.
Our data also demonstrate that there is marked variability in the frequency of IL-17-positive CD4 T cells in SF between RA patients. The underlying cause for this remains unclear but drug therapy may be a contributing factor. As discussed, Yamada
et al. reported that patients taking prednisolone or MTX had a higher frequency of IL-17-producing CD4 T cells, but could not attribute this directly to treatment [
28]. In our study we did not observe this phenomenon. Most patients in this study were receiving treatment with a non-steroidal anti-inflammatory drug, a disease modifying anti-rheumatic drug, a biologic agent or a combination of these (Table
1). We assessed the relationships between therapy and frequencies of IL-17-positive CD4 T cells but found no significant relationships. As it is not yet known how current therapeutic regimes affect the frequency of IL-17-producing CD4 T cells, it is possible that medication, in addition to other factors, such as disease duration and seropositivity, may contribute to the heterogeneity in frequency of IL-17-producing CD4 T cells amongst patients studied here. In the context of medication, appropriately designed longitudinal studies would be needed to address the impact of drug therapy on IL-17 producing cell populations.
IL-17-producing T cells were originally misclassified under the Th1 umbrella. Since the characterisation of Th17 cells, it has been identified that some IL-17-producing T cells coexpress IFNγ. This IFNγ-positive IL-17-positive subset is particularly enriched in the gut of patients with Crohn's disease [
36]. Here we found that the majority of IL-17-producing CD4 T cells in the blood and SF of patients with RA also coexpress IFNγ. However, in the SF we observe a greater frequency of IFNγ-positive IL-17-negative CD4 T cells compared with blood, suggesting that Th1 cells and not Th17 cells predominate in the established RA joint. The relative paucity of IL-17-positive CD4 T cells in either the SF or synovium is at odds with the high levels of IL-17 detected in RA SF [
17‐
21]. One explanation may lie with the use of a non-physiological stimulus
in vitro, such as PMA/ionomycin; stimuli in the RA joint, such as antigen or cytokines, may drive a different cytokine response
in vivo. Ziolkowska
et al. demonstrated that RA PBMC produced significantly more IL-17 than SFMC when challenged with PMA/ionomycin
in vitro, however, stimulation with IL-15 induced greater IL-17 production from SFMC than PBMC [
21]. It is thus possible that the inflammatory environment of the rheumatoid synovium drives Th17 cells to produce IL-17 in a cytokine-dependent manner. In addition, the concept that CD4 T cells may not be the only source of IL-17 in the joint is being increasingly recognised. Mast cells have recently been identified as a source of IL-17 in RA synovium and are potent producers of IL-17 upon stimulation with TNFα, immune complexes and LPS [
37].
IL-22 has been characterised as one of the effector cytokines secreted by Th17 cells [
9,
30,
31], but it is also produced by Th1 cells [
38]. Although this novel cytokine belongs to the IL-10 family, it is proinflammatory in function [
39]. In animal models such as CIA, IL-22 is proinflammatory, whilst IL-22(-/-) mice are less susceptible to CIA than wild-type mice [
32]. In human studies, IL-22 has been proposed to play a role in the pathogenesis of autoimmune inflammatory diseases, such as psoriasis [
40] and Crohn's disease [
41,
42]. In RA, expression of IL-22 was found to be upregulated in synovium and capable of inducing synovial fibroblast proliferation and chemokine production [
33]. Here, we found that IL-17-producing CD4 T cells in the SF coexpressed very little IL-22. Furthermore, we identified an IL-22-producing CD4 T cell population distinct from IL-17-producing CD4 T cells, but this population was not elevated in the blood of RA patients compared to healthy controls nor was it enriched in RA SF. This CD4 T cell subset may be similar to that recently reported to secrete IL-22 but not IL-17 and to be involved in the skin pathophysiology of psoriasis [
43,
44]. The paucity of IL-22-producing CD4 T cells in SF lends support to the notion that the primary source of IL-22 in the joint is not T cells but rather synovial fibroblasts and/or macrophages as reported by Ikeuchi
et al. [
33].
IL-22 production by Th17 cells has been shown to be dependent upon IL-23 [
38,
45,
46], thus our observation, which corroborates that of Shen
et al. [
25], that very few IL-17-producing CD4 T cells express IL-23R provides a potential explanation for the paucity of IL-22-positive IL-17-positive CD4 T cells we observed. Considering the importance of IL-23 to the development and maintenance of Th17 cells, it is striking that over 90% and 85% of IL-17-producing CD4 T cells in the SF and blood respectively did not express IL-23R. However, our data are consistent with recent evidence showing that bioactive IL-23 (p19/p40) was barely detectable in joints of patients with RA [
47].
In contrast to the pattern of IL-22 expression, the majority of IL-17-producing CD4 T cells in SF coexpressed TNFα; these double positive cells were significantly elevated in SF compared to blood. Although the percentage of IL-17-producing CD4 T cells coexpressing TNFα is very small compared to that of TNFα-producing CD4 T cells found in the SF, this may be relevant in terms of therapy. One of the mechanisms by which monoclonal antibodies against TNFα mediate their therapeutic effects, in addition to TNFα blockade, may be through induction of apoptosis in monocytes and T cells by outside to inside signalling through transmembrane TNFα [
48‐
50]. Membrane expression of TNFα on IL-17-producing CD4 T cells would make these cells a potential target of monoclonal antibodies and may help to explain the beneficial effects of these therapies.
Upon identification of the IL-17/IL-23 axis, Th17 cells were viewed as a driving force in the pathogenesis of several autoimmune diseases previously associated with a Th1 predominance. In the case of multiple sclerosis evidence has supported this shift in paradigm [
51,
52]. However in RA, evidence is less clear. There is no doubt that cytokines associated with the Th17 lineage, such as IL-17, IL-6, IL-1β, IL-22, can be found within the RA joint [
20,
33], and as demonstrated here, there is evidence for a small but significant enrichment of Th17 cells within RA SF. In our study, however, we have only examined established RA and many patients had longstanding severe disease; thus 60% (6 of 10) of patients from whom synovial tissue was obtained and 29% (4 of 14) from whom synovial fluid was obtained were on anti-TNF agents. Recent data from Colin
et al. and previous data from our group suggest that the situation may be different in the early phase of RA [
15,
20]. Further studies are required to define the role of Th17 cells in the early phase of disease. The absence of an enrichment of Th17 cells in the synovial tissue of established RA patients is paradoxical to the role this cytokine is reported to play in the pathogenesis of RA [
17‐
21]. This leaves the possibilities that Th17 cells located outside the synovium, such as the juxta-articular bone marrow, may be an additional source of IL-17, that other cells in the synovium, including mast cells [
37] may also produce IL-17 or that the experimental techniques used to reveal IL-17 production
ex vivo do not reveal the true potential of T cells in the rheumatoid joint to produce IL-17. Future work will need to address these issues.
Competing interests
KR, DST and CDB hold an unrestricted research grant from UCB for work on the pathobiology of RA which supported the work described in this report. KR, ADF and CDB hold an unrestricted research grant from Cellzome for work on the pathobiology of RA. KR and CDB hold an unrestricted research grant from Pfizer for work on the pathobiology of RA. SR is employed by UCB.
Authors' contributions
LDC conducted the majority of the experimental study, performed the statistical analysis and drafted the manuscript. AF was involved in the design of the study, consenting and collecting patient samples, coordinating patient samples with the Royal Orthopaedic Hospital, and helped with drafting the manuscript. EH and KH assisted in conducting the experimental study. AT was involved in the design of the study, consenting and collecting patient samples. SR was involved in the design and conception of the study. DST was involved in the design of the study and helped with drafting the manuscript. CB and KR were involved in the design and conception of the study, consenting and collecting patient samples and helped with drafting the manuscript. All authors read and approved the final manuscript.