Objective We sought clinically relevant predictive biomarkers present in CD4 T-cells, or in serum, that identified those patients with undifferentiated arthritis (UA) who subsequently develop rheumatoid arthritis (RA).
Methods Total RNA was isolated from highly purified peripheral blood CD4 T cells of 173 early arthritis clinic patients. Paired serum samples were also stored. Microarray analysis of RNA samples was performed and differential transcript expression among 111 ‘training cohort’ patients confirmed using real-time quantitative PCR. Machine learning approaches tested the utility of a classification model among an independent validation cohort presenting with UA (62 patients). Cytokine measurements were performed using a highly sensitive electrochemiluminescence detection system.
Results A 12-gene transcriptional ‘signature’ identified RA patients in the training cohort and predicted the subsequent development of RA among UA patients in the validation cohort (sensitivity 68%, specificity 70%). STAT3-inducible genes were over-represented in the signature, particularly in anti-citrullinated peptide antibody-negative disease, providing a risk metric of similar predictive value to the Leiden score in seronegative UA (sensitivity 85%, specificity 75%). Baseline levels of serum interleukin 6 (IL-6) (which signals via STAT3) were highest in anti-citrullinated peptide antibodies-negative RA and distinguished this subgroup from non-RA inflammatory synovitis (corrected p<0.05).Paired serum IL-6 measurements correlated strongly with STAT3-inducible gene expression.
Conclusion The authors have identified IL-6-mediated STAT-3 signalling in CD4 T cells during the earliest clinical phase of RA, which is most prominent in seronegative disease. While highlighting potential biomarker(s) for early RA, the role of this pathway in disease pathogenesis awaits clarification.
This paper is freely available online under the BMJ Journals unlocked scheme, see http://ard.bmj.com/info/unlocked.dtl
Statistics from Altmetric.com
If you wish to reuse any or all of this article please use the link below which will take you to the Copyright Clearance Center’s RightsLink service. You will be able to get a quick price and instant permission to reuse the content in many different ways.
The importance of prompt disease-modifying therapy in early rheumatoid arthritis (RA) is now established.1 ,2 Yet about 40% of patients with new-onset inflammatory arthritis present with disease that is unclassifiable at inception, having a so-called undifferentiated arthritis (UA).3 Timely intervention for the subset of these UA patients who subsequently develop RA therefore remains problematic. The issue is highlighted by the publication of updated RA classification criteria4 and a validated ‘prediction rule’ that foretells risk of UA progression to RA.5 Such approaches rely heavily on autoantibody status, emphasising the specificity of circulating anti-citrullinated peptide antibodies (ACPA) for RA.6 Consequently, the diagnosis of ACPA-negative RA remains challenging in the early arthritis clinic (EAC), being frequently delayed despite application of the prediction rule.7
The potential for the whole-genome transcription profiling to yield clinically relevant prognostic ‘gene signatures’ in autoimmune disease has been demonstrated.8 ,9 Applying a similar, prospective approach to the discovery of predictive biomarkers in UA should complement existing diagnostic algorithms, while providing new insights into disease pathogenesis.10 However, the use of peripheral blood (PB) mononuclear cells for transcriptional analysis may result in data that are biased by relative subset abundance.11 To address this, protocols for rapid ex vivo positive selection of cell subsets for the purpose of transcription profiling have been validated.12 Although no single cell-type is exclusively implicated in RA, many of its established and emerging genetic associations implicate the CD4 T cell.13 We therefore hypothesised that the PB CD4 T-cell transcriptome would provide a useful substrate for both biomarker discovery and a pathophysiological understanding of RA induction.
Materials and methods
A complete description of experimental and bioinformatics approaches are given in the online supplementary text.
Patients with recent onset arthritis, naïve to disease-modifying anti-rheumatic drugs and corticosteroids, were recruited between September 2006 and December 2008. An initial working clinical diagnosis was updated by the consulting rheumatologist at consecutive clinic visits for the duration of the study—median 28 months and >12 months in all cases. RA was diagnosed only where 1987 American College of Rheumatology classification criteria14 were fulfilled; UA was defined as a ‘suspected inflammatory arthritis where RA remained a possibility, but where established classification criteria for any rheumatological condition remained unmet’ (see online supplementary text and supplementary table S1). Individuals whose arthritis remained undifferentiated at the end of the study were excluded. Patients gave written informed consent before inclusion into the study, which was approved by the local regional ethics committee.
CD4 T-cell RNA processing and array analysis
Whole blood drawn between 13:00 and 16:30 was stored at room temperature for ≤4 h before processing. After monocyte depletion by immuno-rosetting, an automated magnetic bead-based positive selection protocol was used to isolate CD4 cells (Stemcell Technologies, Vancouver, Canada). Using this approach, a median CD4 T-cell purity of 98.9% was achieved (range 95–99.7%), which was determined using flow cytometry (see online supplementary figure S1). Total CD4 T-cell RNA was immediately extracted, then quality controlled using an Agilent 2100 Bioanalyzer (Agilent, Santa Clara, California, USA). The median RNA integrity number15 of samples used was 9.4. cRNA generated from 250 ng total RNA (Illumina TotalPrep RNA Amplification Kit) was hybridised to the Illumina Whole Genome 6v3 BeadChip (Illumina, San Diego, California, USA), representing 48 804 known genes and expressed sequence tags. Array data were processed using Illumina BeadStudio software, then it was normalised, batch corrected,16 filtered and quality controlled as described (online supplementary text and figure S2).
To define differential expression a fold-change cut-off of 1.2 between comparator groups was combined with a significance level cut-off of p<0.05 (Welch's t-test), corrected for multiple testing using the false-discovery-rate method of Benjamini et al.17 Genes thereby identified were used to train a support vector machine (SVM) classification model based on known outcomes among a ‘training’ sample set.18 The model's accuracy as a prediction tool was then assessed among an independent ‘validation’ sample set. To obtain larger lists of differentially expressed genes for biological pathway analysis, significance thresholds were relaxed through the omission of multiple-test-correction and Ingenuity Pathways Analysis software (Ingenuity Systems, Redwood City, California, USA) was then employed.
Serum cytokine measurement
Between 13:00 and 16:30, baseline serum was drawn and frozen at −80°C until use. Serum interleukin 6 (IL-6), soluble IL-6 receptor (sIL6R), tumour necrosis factor α (TNFα), leptin and granulocyte colony stimulating factor concentrations were measured using a highly sensitive electrochemiluminescence immunosorbance detection system (Meso Scale Discovery, Gaithersberg, Maryland, USA), assays having been validated as outlined (online supplementary text and figure S3).
Quantitative real-time PCR
CD4 T cell total RNA samples were reverse transcribed using superscript II reverse transcriptase and random hexamers, according to the manufacturer's instructions (Invitrogen, Carsbad, California, USA). Real-time PCR reactions were performed as part of a custom-made TaqMan Low Density Array (7900HT real-time PCR system, Applied Biosystems, Foster City, California, USA). Raw data were normalised and expressed relative to the housekeeping gene β-actin as 2−ΔCt values.19
Parametric and non-parametric analyses of variance, Mann–Whitney U tests, Pearson's correlation coefficients, intra-class correlations, multivariate analyses and the construction of receiver operator characteristic (ROC) curves were performed, as described, using SPSS version.15.0 (SPSS, Chicago, Illinois, USA). The derivation of Leiden prediction rules5 and transcriptional ‘risk metrics’ for ACPA-negative RA is outlined in the online supplementary text.
A total of 173 patient samples were retrospectively selected for microarray analysis. One hundred and eleven of these originated from patients assigned definitive diagnoses at inception, confirmed at a median 28 months follow-up (minimum 1 year); an RA versus non-RA discriminatory ‘signature’ was derived from this ‘training cohort’ alone. The remaining 62 samples, all representing UA patients, formed an independent ‘validation cohort’ for testing the utility of the ‘signature’ according to diagnostic outcomes as they evolved during the same follow-up period. As expected, the characteristics of the UA cohort (age, acute phase response, joint counts, etc.) fell between the equivalent measurements in the RA and control sample sets within the training cohort (table 1). For subsequent pathway analysis, all 173 samples were pooled before being divided into four categories based on diagnostic outcome at the end of the study (see online supplementary table S2).
RA transcription ‘signature’ most accurate in ACPA-negative UA
Using a significance threshold robust to multiple test correction (false-discovery-rate p<0.05),17 12 genes were shown to be differentially expressed (>1.2-fold) in PB CD4 T cells between 47 ‘training cohort’ EAC patients with a confirmed diagnosis of RA, and 64 who could be assigned non-RA diagnoses (table 2). An extended list, obtainable by omitting multiple-test correction, appears as online supplementary gene-list 1. Supervised hierarchical cluster analysis of the resultant dataset (111 samples, 12 genes), demonstrated a clear tendency for EAC patients diagnosed with RA to cluster together based on this transcription profile (figure 1A). Quantitative real-time PCR (qRT-PCR)was used to analyse expression of seven of the differentially expressed genes in a subset of 73 samples (for baseline characteristics of this subset, see online supplementary table S4). Despite the reduced power to detect change in this smaller dataset, robust differential expression was confirmed for six of the seven genes (table 2).
To derive a metric denoting risk of progression to RA, the sum of normalised expression values for the 12-gene RA ‘signature’ was calculated for each individual in the training cohort (see online supplementary text). A ROC curve was constructed for this risk metric, the area under which (0.85; SEM=0.04) suggested promising discriminatory utility (figure 1B). A SVM based on the training cohort dataset was then applied to classify members of the validation cohort, correctly identifying UA patients who developed RA with a sensitivity, specificity, positive and negative likelihood ratio (0.68, 95% CI 0.48 to 0.83); 0.70, 95% CI0.60 to 0.87); 2.2, 95% CI 1.2 to 3.8) and 0.4 95% CI 0.2 to 0.8), respectively. However, we observed that of the 13 ACPA-positive UA patients, 12 progressed to RA, indicating that autoantibody status alone was a more sensitive predictor of RA in this subset. By contrast, when applied exclusively to the ACPA-negative subset of the UA validation cohort (n=49), the SVM classification model provided a sensitivity of 0.85 (95% CI 0.58 to 0.96) and a specificity of 0.75 (0.59-0.86) for progression to RA, thereby performing best in this diagnostically most challenging patient group. Hierarchical clustering of the ACPA-negative UA samples based on their 12-gene RA ‘signature’ expression profiles further illustrates molecular similarities within the ACPA-negative RA outcome group (figure 1C).
Gene signature adds value to existing tools in diagnosing ACPA-negative UA
Next, we tested the value of our 12-gene signature in comparison with the existing ‘Leiden prediction rule’ as a predictor of RA among UA patients.5 While the discriminatory utility achieved by the prediction rule in our UA cohort was comparable with that previously reported (n=62; AU ROC curve=0.86; SEM=0.05, data not shown), its performance diminished among the ACPA-negative sub-cohort (n=49; AU ROC curve=0.74; SEM=0.08; figure 1D). Employing a 12-gene risk metric, as described above, equivalent discriminatory utility was found in this sub-cohort (AU ROC curve=0.78; SEM=0.08, data not shown). However, by deriving a modified risk metric, which combined all features of the Leiden prediction rule with our 12-gene risk metric (see online supplementary text and table S5), and applying it to the independent ACPA-negative UA cohort, we could improve the utility of the prediction rule for seronegative UA patients (AU ROC=0.84; SEM=0.06; figure 1D).
STAT3 transcription profile is most prominent in ACPA-negative RA
All 173 patients studied were now grouped into four categories based on outcome diagnosis alone: ACPA-positive RA, ACPA-negative RA, inflammatory non-RA controls and osteoarthritis(OA); their demographic and clinical characteristics are presented for comparison (online supplementary table S2). Three lists of differentially expressed genes were then generated by comparing each of the ‘inflammatory’ groups (which themselves exhibited comparable acute phase responses) with the OA group (>1.2-fold change; uncorrected p<0.05; online supplementary gene-lists 2–4). The three lists were overlapped on a Venn diagram (figure 2).
A highly significant over-representation of genes involved in the cell cycle was identified in association with ACPA-positive RA (24/43; p<1.0×10−5); figure 2; online supplementary gene-list 5). In addition, genes involved in the regulation of apoptosis were over-represented in ACPA-negative RA patients, and RA was, in general, characterised by genes with functional roles in T cell differentiation (figure 2 online supplementary gene-lists 5–8). Importantly, within the highly significant 12-gene RA ‘signature,’ several genes (PIM1, SOCS3, SBNO2, BCL3 and MUC1) were noted to be STAT3-inducible based on literature sources.20,–,25 The majority of these were more markedly differentially expressed in ACPA-negative than ACPA-positive RA (figures 3A,B and online supplementary figures S4A–C). Additional STAT3-inducible genes (MYC, IL2RA)20 ,26 ,27 exhibited similar expression patterns, and there was a trend for STAT3 to be upregulated in ACPA-negative compared with ACPA-positive RA (online supplementary figures S4D–F). Moreover, a reciprocal pattern of expression across outcome groups was observed for the dominant negative helix-loop-helix protein-encoding gene inhibitor of DNA-binding 3 (ID3) (online supplementary figure S4G), consistent with its putative regulatory role in STAT3 signalling.28 MYC and ID3, although absent from the discriminatory RA signature under the stringent significance thresholds used, were however robustly differentially expressed between RA and non-RA patients within the training cohort (table 2). Finally, in relation to both the 12-gene signature and the extended list of genes exclusively deregulated in ACPA-negative RA (online supplementary gene list 6), overlap with independently predicted STAT3-inducible gene sets (see online supplementary text and supplementary gene list 9) confirmed a preponderance of STAT3-inducible genes (hypergeometric p-values <0.005 in both cases; see online supplementary text) – which was not seen for genes deregulated only in ACPA-positive RA (p=0.19).
Serum IL-6 is highest in ACPA-negative RA and independently predicts CD4 STAT3-inducible gene expression
Since one classical mechanism of STAT3 phosphorylation is via gp130 co-receptor ligation,29 we hypothesised that increased systemic levels of a key gp130 ligand and pro-inflammatory cytokine, IL-6, may be responsible for the STAT3-mediated transcriptional programme in early RA patients. Baseline serum IL-6 was measured in 131 of the 173 EAC patients which were subsequently grouped according to their ultimate diagnosis (ACPA-negative RA, ACPA-positive RA, non-RA inflammatory arthropathy or OA). IL-6 levels were low overall (generally <100 pg/ml), but were highest in the ACPA-negative RA group (figure 3C). Indeed, unlike the generic marker of systemic inflammation C reactive protein (CRP), baseline IL-6 discriminated ACPA-negative RA from non-RA inflammatory arthritides (figures 3C,D). Furthermore, among individuals for whom paired and contemporaneous serum IL-6 and PB CD4 T-cell RNA samples were available, clear correlations between IL-6 and the normalised expression of STAT3-inducible genes were seen (figures 4A–D; also online supplementary figures S5A–D); for example, serum IL-6 measurements correlated with normalised SOCS3 expression: Pearson's R=0.57, p<0.001 (figure 4A). Multivariate analysis confirmed that IL-6, but not CRP or TNFα (which does not signal via STAT3), independently predicted PB CD4 T cell SOCS3 expression (β=0.53; p<0.001; see online supplementary table S6) excluding a more general influence of inflammation.
Given that only 30–50% of PB CD4 T cells are thought to express membrane-bound IL6R,30 we also measured sIL6R (as a surrogate of IL-6R trans-signalling)31 and two other gp130 ligands, granulocyte colony stimulating factor and leptin, both of which have been implicated in RA pathogenesis.32 ,33 However, levels in sera from a subset of 80 study patients correlated with neither the diagnostic outcome nor the STAT3 gene expression. Finally, IL-10 and IL-17, which are both STAT3 activators,34 were undetectable in the vast majority of sera (data not shown).
STAT3-inducible, RA-associated expression signature is activated by IL-6 in primary CD4 T cells of healthy donors in vitro
To confirm that the observed deregulated expression of STAT3 target genes among early RA patients was downstream of IL-6 signalling, primary human CD4 T cells were incubated in vitro with recombinant human IL-6 and the expression of relevant target genes measured at 1 and 6 h (see online supplementary text and figures S6–S7). Robust upregulation of SOCS3, PIM1, BCL3 and MYC was observed consistently 1 h after the addition of IL-6. A similar trend was seen for SBNO2, which became significant in the presence of recombinant soluble human IL-6 receptor. Conversely and consistent with prior observations, a distinct trend towards repression of ID3 was seen in response to IL-6 plus sIL6R.
We present a unique analysis of the CD4 T-cell transcriptome in a well-characterised inception cohort of early arthritis patients attending a routine EAC in UK. As a potential diagnostic tool, it is significant that our 12-gene ‘RA expression signature’ (table 2) performed best among the diagnostically challenging ACPA-negative UA patient group. Intriguingly, these findings support the involvement of CD4 T cells in both ACPA positive and negative disease.
The signature's sensitivity and specificity (0.85 and 0.75) for predicting subsequent RA in seronegative UA patients equate to a positive likelihood ratio of 3.4, indicating that a prior probability of 25% for RA progression among this cohort (13 of the 49 patients progressed to RA) doubles to 53% for an individual who has been assigned a positive SVM classification.35 Moreover, of the 13 ACPA-negative UA patients who progressed to RA in our cohort, 8 fell into an ‘intermediate’ risk category for RA progression according to the validated Leiden prediction score.5 Encouragingly, all but one of these patients were correctly classified based on their 12-gene expression profile. Our proposal that this approach might add value to existing algorithms for the diagnosis of ACPA-negative UA is further supported by the construction of ROC curves comparing the Leiden prediction rule with a modified risk metric that incorporates features of our gene signature (figure 1D).
Our data indicate that PB CD4 T cells in early RA are characterised by a predominant upregulation of biological pathways involved in cell cycle progression (ACPA-positive) and survival, death and apoptosis (ACPA-negative) (figure 2; also online supplementary gene lists 5–6). Pathway analysis also suggested that T-cell development and differentiation were deregulated in both RA serotypes (online supplementary gene list 7). These findings concur with previous observations of impaired T-cell homeostasis in RA, characterised by increased turnover, telomere shortening and immunosenescence.36 ,37 Given the well-characterised importance of the STAT3 signalling pathway in both oncogenesis and T-cell survival, it was notable that five genes from our statistically robust 12-gene RA signature are downstream of STAT3 signalling.20,–,25 The degree to which these genes sub-cluster according to the expression pattern among individuals in both the training and validation cohorts (figure 1A,C) presumably reflects their co-regulation by STAT3. Their upregulation was generally most pronounced in ACPA-negative RA (figure 3A,B; also online supplementary figure S4A–C), explaining why the predictive utility of the 12-gene signature was optimal in this disease subset.
Our observation that increased serum IL-6 levels among EAC attendees may predict a diagnosis of RA versus alternative arthritides is consistent with findings of previous biomarker studies,38 ,39 but ours is the first demonstration of a particular association with ACPA-negative disease (figure 3C). Striking correlations were seen between PB CD4 T-cell expression of several STAT3-inducible genes and paired, contemporaneous serum IL-6 concentrations, which were independent of alternative acute phase markers (figures 4A–D; also online supplementary figures S5A–D and table S6). STAT3 phosphorylation and downstream transcription is initiated by ligation of the cell-surface gp130 co-receptor by a range of ligands, including IL-6.40 We measured IL-6 in particular because of its recognised role as a pro-inflammatory cytokine in RA,41 and we excluded similar relationships with sIL6R (a surrogate of IL-6R trans-signalling) and other relevant substrates of STAT3 signalling. Therefore, the STAT3-inducible gene expression signature that we have identified does appear to be downstream of IL-6 signalling. The capacity of IL-6 alone to induce the STAT-3-regulated elements of our early RA gene expression signature in primary CD4 T cells was confirmed in vitro (online supplementary figures S6 and S7).
In conclusion, our data provide strong evidence for the induction of an IL-6-mediated STAT3 transcription programme in PB CD4 T cells of early RA patients, which is most prominent in ACPA-negative individuals and which contributes to a gene expression ‘signature’ that may have diagnostic utility. Furthermore, our findings could pave the way for a novel treatment paradigm, whereby emerging drugs targeting the IL-6-gp130-STAT3 ‘axis’42 ,43 find a rational niche as first choice agents in the management of ACPA-negative RA. Studies, such as ours, should ultimately contribute to the realisation of true ‘personalised medicine’ in early inflammatory arthritis, in which complex heterogeneity is stratified into pathophysiologically and therapeutically relevant subsets, with clear benefits in terms of clinical outcome and cost.
AGP's work was supported by a clinical research fellowship from the Arthritis Research Campaign, UK. This work was supported by the UK NIHR Biomedical Research Centre for Ageing and Age-Related Disease Award to the Newcastle upon Tyne Hospitals NHS Foundation Trust. Clinical and translational research in the Musculoskeletal Research Group is supported by the Northumberland, Tyne and Wear Comprehensive Local Research Network. The authors would like to thank the clinical staff at The Freeman Hospital who co-operated with the recruitment phase of the study, and, of course, the many patient volunteers who contributed so willingly.
This web only file has been produced by the BMJ Publishing Group from an electronic file supplied by the author(s) and has not been edited for content.
Files in this Data Supplement:
- Web Only Data - This web only file has been produced by the BMJ Publishing Group from an electronic file supplied by the author(s) and has not been edited for content.
- Web Only Data - This web only file has been produced by the BMJ Publishing Group from an electronic file supplied by the author(s) and has not been edited for content.
Funding This study was supported by Arthritis Research UK (grant number 17983).
Competing interests None.
Ethics approval Ethics approval was provided by the Newcastle and North Tyneside Local Research Ethics Committee.
Provenance and peer review Not commissioned; externally peer reviewed.
Data sharing statement Raw and processed microarray data used in this study is available via Gene Expression Omnibus at: http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?token=bviftkociimgsnk&acc=GSE20098.