Objectives Systemic lupus erythematosus (SLE; OMIM 152700) is characterised by the production of antibodies to nuclear antigens. We previously identified variants in complement receptor 2 (CR2/CD21) that were associated with decreased risk of SLE. This study aimed to identify the causal variant for this association.
Methods Genotyped and imputed genetic variants spanning CR2 were assessed for association with SLE in 15 750 case-control subjects from four ancestral groups. Allele-specific functional effects of associated variants were determined using quantitative real-time PCR, quantitative flow cytometry, electrophoretic mobility shift assay (EMSA) and chromatin immunoprecipitation (ChIP)-PCR.
Results The strongest association signal was detected at rs1876453 in intron 1 of CR2 (pmeta=4.2×10−4, OR 0.85), specifically when subjects were stratified based on the presence of dsDNA autoantibodies (case-control pmeta=7.6×10−7, OR 0.71; case-only pmeta=1.9×10−4, OR 0.75). Although allele-specific effects on B cell CR2 mRNA or protein levels were not identified, levels of complement receptor 1 (CR1/CD35) mRNA and protein were significantly higher on B cells of subjects harbouring the minor allele (p=0.0248 and p=0.0006, respectively). The minor allele altered the formation of several DNA protein complexes by EMSA, including one containing CCCTC-binding factor (CTCF), an effect that was confirmed by ChIP-PCR.
Conclusions These data suggest that rs1876453 in CR2 has long-range effects on gene regulation that decrease susceptibility to lupus. Since the minor allele at rs1876453 is preferentially associated with reduced risk of the highly specific dsDNA autoantibodies that are present in preclinical, active and severe lupus, understanding its mechanisms will have important therapeutic implications.
- Systemic Lupus Erythematosus
- Gene Polymorphism
- B cells
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Systemic lupus erythematosus (SLE (OMIM 152700)) is a heterogeneous autoimmune disease with a strong genetic component modified by environmental exposures. The complement system has been linked to its pathogenesis since low serum complement levels were first demonstrated in patients with active disease.1 ,2 Although complement activation resulting in tissue damage is an important feature of lupus, deficiencies of early classical complement pathway components are paradoxically strongly associated with lupus susceptibility. Deficiencies or altered function of complement receptors have also been associated with lupus in humans and murine models of disease.3–5 These effects have been attributed to alterations in antigen clearance, antigen processing, tolerance induction and cell activation, but the exact mechanisms remain poorly understood.
SLE is characterised by the production of class-switched autoantibodies against nuclear antigens that have undergone affinity maturation, suggesting their generation in germinal centre reactions. Complement receptor 2 (CR2/CD21) is primarily expressed on mature B cells and follicular dendritic cells, two major components of germinal centres. We first showed Cr2, which encodes both CR2 and complement receptor 1 (CR1/CD35) in the mouse, to be a candidate gene for lupus susceptibility in the NZM2410 model of lupus based on structural and functional alterations in its gene products.6 We subsequently demonstrated strong association of a common three single-nucleotide polymorphism (SNP) CR2 haplotype (rs3813946 in the 5′UTR, rs1048971 and rs17615 in exon 10) with increased risk of lupus susceptibility (p=1.0×10−5) in Caucasian and Chinese lupus simplex families with a 1.54-fold increased risk for disease development.7 We confirmed this in a case-control analysis of an independent European-derived population (p=2.3×10−2, OR 1.1 (95% CI 1.02 to 1.2))8 and also showed that a haplotype formed by the minor alleles of three SNPs in exons 10 and 11 (rs1048971, rs17615, rs4308977) was associated with decreased risk of lupus (p=1.6×10−2, OR 0.90 (95% CI 0.82 to 0.98)).8
In this study, we fine-mapped the region spanning CR2 in 15 750 subjects from four ancestral groups to identify potential causal variant(s) for these associations with lupus. Additionally, we explored the association of CR2 polymorphisms with clinical manifestations of lupus in order to generate new hypotheses regarding how CR2 contributes to disease development.
DNA from individuals recruited from multiple sites was processed at the Oklahoma Medical Research Foundation (OMRF; Large Lupus Association Study 2) with institutional review board approval. All patients with SLE met the 1997 American College of Rheumatology revised classification criteria.9 Clinical data were collected by chart review or testing in the OMRF Clinical Immunology laboratory. Samples for functional analyses were from healthy non-smoking 18-year-old to 60-year-old adults without family history of autoimmune disease at the University of Colorado School of Medicine.
Genotyping was performed on the OMRF Illumina iSelect platform.10 ,11 Subjects with missing genotype rate >10%, shared identical by descent >0.4 or gender mismatch were removed. Global ancestry was estimated based on the genotype of ancestry informative markers (AIMs), using principal components analysis12 and ADMIXMAP13 as described14 and genetic outliers removed. Final clean data were from European Americans (EA), African Americans (AA; 7.5% Gullahs), Asians (AS; 74.6% Koreans, 16.1% Chinese, 9.3% Japanese and Singaporeans) and Hispanics (HS) enriched for Amerindian–European admixture. 2001 EA cases and 2153 EA controls were previously analysed.8 Subjects for functional studies were genotyped using a Taqman SNP Genotyping Assay.
SNP and insertion-deletion (INDEL) genotypes of 379 Europeans, 246 Africans, 286 Asians and 181 Americans from the 1000 Genomes Project (V.3, Phase 1 integrated data, March 2012 release) were references in imputation for EA, AA, AS and HS subjects, respectively. Imputation was performed using IMPUTE 2.1.215; genotypes with information scores >0.9 and minor allele frequency (MAF)>0.01 were further analysed.
SNPs and INDELs showing biased Hardy–Weinberg equilibrium (p<0.01 in controls, p<0.0001 in cases), missing genotype rate >5% or different missing genotype rates between cases and controls (rate >2% and p<0.05) were excluded. Variants were assessed for association with SLE under a logistic regression model, and haplotypic and haplotype-based conditional association tests were performed, adjusting for gender and the first three principal components estimated using AIMs. For transancestral meta-analysis, a fixed effect model was applied if Cochran's Q statistic showed no evidence of genetic heterogeneity among ORs (p>0.05); otherwise, a random effect model was used. Analyses were performed using PLINK V.1.07.16
Peripheral blood mononuclear cells (PBMC) were isolated over Ficoll–Paque (Sigma–Aldrich). DNA was purified using the QIAamp DNA Mini Kit (QIAgen). B cells were purified using the Easy Sep Human B Cell Enrichment Kit (StemCell Technologies). RNA was processed using the RNeasy Plus Mini Kit (QIAgen). Quality check and quantification of RNA was performed using the Agilent 2100 Bioanalyzer. RNA and DNA were stored at −70°C. Epstein–Barr virus (EBV)-transformed B cell lines were generated by incubating PBMCs with supernatant from cell line GM7404A and cyclosporine A.
qPCR and quantitative flow cytometry
qPCR of primary B cell transcripts was performed using cDNA transcribed using random primers and MultiScribe reverse transcriptase (Applied Biosystems), customised CR2 primers (5′-CGAGAAGTATATTCTGTTGATCCATACAA-3′, 5′-CTAATCAATATTCCGCTGAATTCCA-3′) and probe (6FAM-AACTGGTGTGTGCCTCA-MGBNFQ), Taqman assays for CR1 (4331182) and β-actin (4352935E), and the Applied Biosystems 7500 Real-Time PCR System. Relative expression levels of CR2 and CR1, normalised to β-actin, were calculated using the comparative CT method.17
Quantitative flow cytometry was performed using Quantum Simply Cellular microbeads (Bangs Laboratories). Purified B cells were incubated with ethidium monoazide to exclude dead cells and mouse IgG to block Fc receptors and stained with biotinylated anti-human CD19 (clone HD37) followed by AF405-labelled streptavidin (Molecular Devices) and either AF488-labelled anti-human CR1 (clone 6B1.H12) or AF488-labelled anti-human CR2 (clone THB5, Harlan). Data acquired on fixed cells within 24 h using the LSR II and CellQuest software (BD Biosciences) were analysed with FlowJo (Tree Star).
Electrophoretic mobility shift assay
39-mer oligonucleotides (5′–GGGCCAAAAGCGAGACGGT[G/A]GGGGCAGTGCTCGACG–3′, 5′–CGTCGAGCACTGCCCC[C/T]ACCGTCTCGCTTTTGGCCC–3′) were synthesised, HPLC-purified and biotin-labelled; 25 fmol labelled oligonucleotides were incubated with 2–4 μg nuclear extracts (NE) or 50 mM potassium chloride (for unbound controls) in 4% Ficoll, 20 mM N-2-hydroxyethylpiperazine-N-2-ethane sulfonic acid (HEPES), 1 mM EDTA, 0.5 mM dithiothreitol and 1 µg poly dI:dC for 30 min on ice. For competition and blocking experiments, NE were pre-incubated with unlabelled oligonucleotide or anti-CCCTC-binding factor (CTCF) (sc-15914; Santa Cruz Biotechnology) for 10 or 30 min on ice. Reactions were electrophoresed on 6% DNA retardation gels (Life Technologies), transferred and cross-linked using ultraviolet light to nylon membranes and visualised using the Chemiluminescent Nucleic Acid Detection Module (Thermo Fisher Scientific).
Chromatin immunoprecipitation (ChIP) was performed using the Upstate Biotechnology ChIP assay kit with minor modifications.18 1.1×108 cells were incubated with 1% formaldehyde for 15 min and 0.125 M glycine added for 5 min. Washed cells were incubated in NP-40 lysis buffer and nuclei pelleted, resuspended in sodium dodecyl sulfate lysis buffer and sonicated five times on ice. Precleared soluble chromatin was incubated with anti-CTCF, an isotype control, or no antibody followed by Protein G agarose/salmon sperm DNA. qPCR was performed on immune complex-associated DNA using primers spanning rs1876453 (5′–GGAAAGTTTCTGTGCCGCGA–3′, 5′-GACAATCAGGACCAGGCGGT–3′), SYBR Green-based detection, and the Illumina Eco Real-Time PCR System. A standard curve was constructed using a chromatin input control.
qPCR of EBV-transformed cell transcripts was performed using cDNA transcribed using the Superscript VILO cDNA synthesis kit (Life Technologies), primers specific for β-actin (5′-GATGACCCAGATCATGTTTGAG-3′, 5′-GACTCCATGCCCAGGAAGGAA-3′), CTCF (5′-CAACCAGCCCAAACAGAACCAG-3′, 5′-TCCTCTTCCTCTCCCTCTGC-3′), CR2 (5′-TGCCTGTAAAACCAACTTCTC-3′, 5′-AGCAAGTAACCAGATTCACAG-3′) and CR1 (5′-TGCTAAGGACAGGTGCAGAC-3′, 5′-GGCAGACGAGGAACCAATGA-3′), SYBR Green-based detection, and the Eco Real-Time PCR System (Illumina). Transcript abundance was determined by comparison with a standard curve and normalised to β-actin.
A two-tailed unpaired Student t test detected differences between groups. Spearman rank correlation determined correlation within a group. A p value of <0.05 was considered significant. Statistics and graphs were generated using GraphPad Prism software.
Association of rs1876453 with decreased risk of lupus
To localise causal variants of the CR2 gene, we genotyped 56 SNPs in CR2 and CR1 and 347 AIMs in 15 750 unrelated case-control subjects from four ancestral groups: EA (3872 cases vs 3449 controls), AA (1676 vs 1929), AS (1265 vs 1260) and HS (1492 vs 807). Genotypes for additional variants (SNPs and INDELs) were imputed using reference data from the 1000 Genomes Project. After applying quality control measures, 138 EA, 167 AA, 102 AS and 133 HS genetic variants deeply covering a 57.6 kB region 5′ upstream of CR2 to intron 1 of CR1 were assessed for association with SLE (see online supplementary figure S1 and table S1). Only rs1876453, in intron 1 of CR2, was consistently associated with SLE in EA (MAF 0.086 in cases vs 0.099 in controls, p=0.045, OR 0.89 (95% CI 0.79 to 0.99)), AA (0.075 vs 0.086, p=0.045, OR 0.83 (95% CI 0.70 to 0.99)) and HS (0.032 vs 0.051, p=3.5×10−3, OR 0.62 (95% CI 0.46 to 0.86)). rs1876453 was not associated with SLE in AS given the low MAF in this group (0.0004 vs 0.0008, p=0.68, OR 0.60 (95% CI 0.05 to 6.74)). In transancestral meta-analysis of 75 genetic variants assessed in EA, AA, AS and HS (see online supplementary figure S1 and table S1), the strongest association signal was detected at rs1876453 (p=4.2×10−4, OR 0.85) and only this signal reached the Bonferroni-corrected significance level (p<6.7×10−4).
Increased signal associated with rs1876453 after subphenotype stratification
We next assessed the association of rs1876453 with 14 lupus subphenotypes. In case controls, the minor allele was consistently associated with decreased risk of serositis, renal disorder, haematological disorder and dsDNA autoantibodies in EA, AA and HS, of which the strongest association was detected with dsDNA autoantibodies (pEA=6.6×10−4, OR 0.73 (95% CI 0.61 to 0.88); pAA=9.7×10−3, OR 0.72 (95% CI 0.56 to 0.92); pHS=7.1×10−3, OR 0.58 (95% CI 0.39 to 0.86); pmeta=7.6×10−7, OR 0.71) (table 1). In cases only, the minor allele of rs1876453 was associated with decreased risk of dsDNA autoantibodies (pmeta=1.9×10−4, OR 0.75) and renal disorder (pmeta=1.3×10−2, OR 0.83) (table 1), but only the association with dsDNA autoantibodies remained significant after correction for multiple comparisons.
rs1876453 tags the protective EA haplotype
No other SNP in this region exhibited stronger association with dsDNA autoantibodies in EA, AA and HS than rs1876453 (figure 1A–C, see online supplementary table S2). When conditioning on rs1876453, the association signals at all other SNPs were eliminated (see online supplementary table S2). The H1 haplotype, constructed using rs1876453 and previously associated or tightly linked CR2 SNPs, was equivalent to the protective EA SLE haplotype8 and was perfectly tagged in EA by the minor allele of rs1876453 (figure 1D). In all three ancestral groups, it was associated with decreased risk of SLE (pEA=0.037, pAA=0.043 and pHS=0.042) and dsDNA autoantibodies (pEA=6.0×10−4, pAA=7.8×10−3 and pHS=0.034).
The minor allele at rs1876453 is associated with altered expression of B cell CR1
We did not detect allele-specific differences in CR2 mRNA or protein levels in primary B cells from healthy controls (figure 2A, B). However, CR1 mRNA and protein levels were significantly higher in subjects with the minor A allele (figure 2C, D). Although B cell CR1 and CR2 levels were positively correlated in both groups (major allele Spearman r=0.6342, p<0.0001; minor allele Spearman r=0.7998, p<0.0001, figure 2E), the ratio of CR1 to CR2 on B cells was higher in subjects with the minor allele (p=0.0002; figure 2F). Allele-specific differences in CR1 expression were not detected on other peripheral blood cells (see online supplementary figure S2). These data suggest that rs1876453 has long-range effects on the regulation of expression of CR1, which lies directly 3′ of CR2, that are either B cell-specific or dependent on coexpression of CR2.
The minor allele at rs1876453 alters transcription factor binding
rs1876453 is 97 nucleotides from the 5′ end of the first intron of CR2. This ∼12 kb intron contains a conserved silencing domain that controls CR2 expression in a cell type-specific and developmentally regulated manner.19–22 The ENCyclopedia Of DNA Elements (ENCODE) database23 reports the in vivo interaction of the region surrounding rs1876453 with multiple transcription factors in B cells, including Pax5, Oct2 and CTCF (figure 3). We confirmed the formation of multiple protein-DNA complexes containing the sequence surrounding rs1876453 by electrophoretic mobility shift assay (EMSA) using NE from several cell lines (K562, erythroid, CR1+CR2−; Reh, pre-B, CR1+CR2−; Ramos, mature B, CR1+CR2+, see online supplementary figure S3). In the presence of the minor A allele at rs1876453, transcription factor binding was reduced or ablated and less cold competitor was required to out-compete protein-DNA complexes (figure 4A). Addition of an antibody to CTCF blocked the formation of complex C (figure 4B), and specific enrichment of the region surrounding rs1876453 was three-fold higher in the presence of the major allele by ChIP-PCR (p=0.0178; figure 5A–D), suggesting that CTCF binds the region surrounding rs1876453 in an allele-specific manner. CTCF abundance was comparable between the two cell lines (figure 5E), and transcript abundance of CR1 relative to CR2 was higher in the cell line homozygous for the minor allele (p=0.023; figure 5F), consistent with the data from primary B cells.
The minor allele of rs1876453, located in intron 1 of CR2, was associated with decreased risk of lupus in three of four ancestral groups studied, with the strongest association when cases were stratified based on the presence of dsDNA autoantibodies. This allele altered the formation of multiple DNA-protein complexes, including one containing CTCF, which has been termed the master regulator of chromatin organisation. Furthermore, it was associated with increased B cell expression of CR1, suggesting long-range effects of rs1876453 on gene regulation and providing a plausible mechanism by which it may alter lupus susceptibility.
We previously identified the SLE-associated haplotype tagged by the minor allele of rs1876453 (H1 as shown in figure 1D) in EA,8 and show here that it is found also in AA and HS (figure 1D). Although it is difficult to prove that a SNP is causal based on association testing, our transancestral study, which analysed a high density of SNP markers and capitalised on the weak linkage disequilibrium around rs1876453 in AA (figure 1B), provides compelling evidence that rs1876453 rather than the previously identified SNPs (rs3813946, rs1048971, rs17615 and rs4308977) or SNPs tightly linked to rs1876453 in EA (rs17258955 and rs61821130 in intron 1, rs61735651 in exon 14 and rs7549152 in intron 15) best explains the association signal. Modest association signals of rs1876453 increased after stratification of subjects based on specific clinical manifestations of lupus, with the strongest signals in the case-control analysis when subjects were stratified based on the presence of dsDNA autoantibodies. Although increased signals were seen with other clinical manifestations, only dsDNA autoantibodies were significantly associated in both case-control and case-only analyses, suggesting that rs1876453 has a preferential effect on the production or presence of dsDNA autoantibodies. The mechanism underlying this dsDNA specificity is unclear, and characterising it will lead to a greater understanding of the etiopathogenesis of lupus, since dsDNA autoantibodies are highly specific for SLE (reviewed in refs24 ,25), and can predict onset and exacerbation of disease.26–28 Anti-dsDNA antibody levels in the serum of genotyped patients with SLE did not correlate with rs1876453 genotype (data not shown), but therapy and other disease-related factors may obscure an association. Future studies with longitudinal analyses of patients will address this more stringently.
rs1876453 is located in a transcriptional regulatory region defined by DNase hypersensitivity and containing histone marks associated with active enhancers (H3K27ac, H3K4me1 and H3K4me3) (figure 3). We demonstrated that the minor allele at rs1876453 alters the formation of multiple protein-DNA complexes (figure 4A) and that CTCF is a component of one of these complexes (figures 4B and 5). CTCF, a highly conserved and ubiquitously expressed zinc finger protein, is a master regulator of genome spatial organisation that mediates chromatin loops within the genome.29 By binding to insulators and boundary elements, it demarcates chromatin into regulatory regions and blocks communication between promoters and enhancers to regulate gene expression. CTCF interacted with the region surrounding rs1876453 in both lymphoblastoid B cell lines and primary B cells,23 with peak occupancy directly over rs1876453 (figure 3), and our data demonstrate an allele-dependent effect on its binding in vivo (figure 5) with less binding of CTCF to the minor A allele, which is associated with higher CR1 expression and is protective, and more binding to the major G risk allele, which is associated with lower CR1 expression. These data suggest that CTCF may have a repressive effect on CR1 transcription when bound to this locus. Efforts to identify the other transcription factors differentially binding this region as a result of the allele at rs1876453 are currently underway.
CR1 expression was increased in B cells of subjects harbouring the minor allele at rs1876453 at both the mRNA and protein level (figure 2). Eukaryotic transcription is tightly controlled by regulatory elements that, though perhaps distant from their target genes, can be brought into close proximity with the general transcriptional machinery at transcription start sites through the formation of chromatin loops.30 Therefore, altered CTCF binding at intron 1 of CR2 may directly affect CR1 transcription via alterations in the chromatin looping that regulates these genetic regions. Alternatively, CR1 expression may be modified indirectly by regulatory RNA generated from intronic CR2 sequences. The minor allele at rs1876453 introduces a cryptic splice acceptor site (consensus value (CV) 71.05, CV variation of mutant from wild type 68.75%) and is predicted to break splice enhancer and silencer motifs (Human Splicing Finder31). Although there are no known microRNA sequences in the first intron of CR2, several expressed sequence tags have been aligned to this region in B cells32 and the ENCODE project has determined that it is actively transcribed (figure 3).
CR1 binds C3b and C4b activation fragments and is physically associated with CR2 on B cells.33 Although it has an independent negative regulatory role in B cell receptor (BCR)-mediated B cell activation,34 it also acts as a cofactor for the Factor I-mediated cleavage of C4b to iC4b and of C3b to iC3b and C3dg. iC3b and C3dg are specific ligands for CR235 that either augment or inhibit signalling through the BCR in mature B cells,36 ,37 depending on ligand valency. Strength of BCR signalling may also affect tolerance induction in transitional B cells.38 Therefore, we hypothesise that increased expression of CR1 associated with rs1876453, in individuals susceptible to lupus, may tolerise transitional or arrest mature dsDNA-specific B cells that encounter complement-coated apoptotic debris and, as a consequence, modify the initiation or course of lupus.
In sum, we show that the minor allele at rs1876453 reduces risk of lupus and that this effect is due, in part, to increased expression of CR1 on B cells. Since this allele alters binding of transcription factors with long-range effects, allelic variation at this SNP may modify expression of additional genes involved in lupus pathogenesis. Given the common association of rs1876453 across ancestral groups, further investigation of its mechanisms and effects has broad implications for the management of patients with this disease.
We thank the volunteers who participated in this study; Agnessa Gadiliya, Carissa Homme, Najuk Jain and Lauren Kuhlman (University of Colorado School of Medicine, Aurora, Colorado, USA) for recruiting subjects, processing samples and technical assistance; Krista Bean (OMRF, Oklahoma City, Oklahoma, USA) for assistance with data analysis; Dr Henry Marsh and Celldex Therapeutics, Boston, Massachusetts, USA for providing the anti-CR1 monoclonal antibody 6B1.H12; Dr Ellen Vitetta from University of Texas-Southwestern, Dallas, Texas, USA for providing the anti-CD19 monoclonal antibody HD37; and Drs V. Michael Holers, Tasha E Fingerlin, and Richard A Spritz (University of Colorado School of Medicine, Aurora, Colorado, USA) for helpful discussions. The BIOLUPUS network is composed of Johan Frostegård, MD, PhD (Huddinge, Sweden), Lennart Truedsson, MD, PhD (Lund, Sweden), Enrique de Ramón, MD PhD (Málaga, Spain), José M Sabio, MD, PhD (Granada, Spain), María F González-Escribano, PhD (Sevilla, Spain), Javier Martin, MD, PhD (Granada, Spain), Norberto Ortego-Centeno (Granada, Spain), José Luis Callejas MD (Granada, Spain), Julio Sánchez-Román, MD (Sevilla, Spain), Sandra D'Alfonso, PhD (Novara, Italy), Sergio Migliarese MD (Napoli, Italy), Gian-Domenico Sebastiani MD (Rome, Italy), Mauro Galeazzi MD (Siena, Italy), Torsten Witte, MD, PhD (Hannover, Germany), Bernard R Lauwerys, MD, PhD (Louvain, Belgium), Emoke Endreffy, PhD (Szeged, Hungary), László Kovács, MD, PhD (Szeged, Hungary), Carlos Vasconcelos, MD, PhD (Porto, Portugal) and Berta Martins da Silva, PhD (Porto, Portugal). The members of GENLES Network are Hugo R Scherbarth, Pilar C Marino, Estela L Motta, Susana Gamron, Cristina Drenkard, Emilia Menso, Alberto Allievi, Guillermo A Tate, Jose L Presas, Simon A Palatnik, Marcelo Abdala, Mariela Bearzotti, Alejandro Alvarellos, Francisco Caeiro, Ana Bertoli, Sergio Paira, Susana Roverano, Cesar E Graf, Estela Bertero, Cesar Caprarulo, Griselda Buchanan, Carolina Guillerón, Sebastian Grimaudo, Jorge Manni, Luis J Catoggio, Enrique R Soriano, Carlos D Santos, Cristina Prigione, Fernando A Ramos, Sandra M. Navarro, Guillermo A Berbotto, Marisa Jorfen, Elisa J Romero, Mercedes A Garcia, Juan C Marcos, Ana I Marcos, Carlos E Perandones, Alicia Eimon, Sanatorio Parque and Cristina G. Battagliotti in Argentina; Eduardo Acevedo and Mariano Cucho in Perú; Ignacio García de la Torre, Mario Cardiel Ríos, José Francisco Moctezuma and Marco Maradiaga Ceceña in Mexico.
The UCSC Genes Track from ENCODE was produced at UCSC using a computational pipeline developed by Jim Kent, Chuck Sugnet, Melissa Cline and Mark Diekhans. It is based on data from NCBI RefSeq, UniProt (including TrEMBL and TrEMBL-NEW), CCDS and GenBank, as well as data from Rfam and the Todd Lowe lab. The UCSC Uniform DNaseI HS Track was created by the ‘Open Chromatin’ (Duke/UNC/UT-A) ENCODE group: Duke University Institute for Genome Sciences & Policy (IGSP): Alan Boyle, Lingyun Song, and Greg Crawford, University of North Carolina at Chapel Hill: Paul Giresi, Jason Lieb, and Terry Furey, Universty of Texas at Austin: Zheng Liu, Ryan McDaniell, Bum-Kyu Lee and Vishy Iyer. European Bioinformatics Institute: Paul Flicek, Damian Keefe, and Ewan Birney, and University of Cambridge, Department of Oncology and CR-UK Cambridge Research Institute (CRI): Stefan Graf with support from NHGRI and by the University of Washington (UW) ENCODE group (contact: Richard Sandstrom). The Layered H3K4Me3, H3K4Me1 and H3K27Ac Tracks show data from the Bernstein Lab at the Broad Institute. The Transcription Factor ChIP-seq Track shows data from the Myers Lab at the Hudson Alpha Institute for Biotechnology, the labs of Michael Snyder, Mark Gerstein and Sherman Weissman at Yale University, Peggy Farnham at UC Davis, Kevin Struhl at Harvard, Kevin White at The University of Chicago, and Vishy Iyer at The University of Texas Austin. The Broad Histone Track shows data generated at the Broad Institute and in the Bernstein lab at the Massachusetts General Hospital/Harvard Medical School, with data generation and analysis supported by funds from the NHGRI, the Burroughs Wellcome Fund, Massachusetts General Hospital and the Broad Institute (Contact: Noam Shoresh). The Transcription Track shows data from the Wold Lab at Caltech.
Handling editor Tore K Kvien
JZ, BMG and RLT contributed equally.
Memberships for the BIOLUPUS and GENLES Networks are available in the Acknowledgements section.
Contributors JCE, RPK, EEB, BPT, HW and SAB: selected SNPs for the association study, and PMG, KMS, JAK, KMK, CDL and JBH: were responsible for the design of the large lupus association study. MEA-R, GSA, J-MA, S-CB, SAB, EEB, LAC, JCE, BIF, PMG, GSG, JMG, JBH, COJ, JAJ, DK, DLK, RPK, H-SL, JTM, KMS, TBN, MAP, RR-G, JDR, RHS, AMS, BPT, LMV and TJV: assisted in the collection and characterisation of the SLE cases and controls. AJA, KMK and PMG: performed the genotyping. SBG, AHW, MEC, JTZ, MCM, KMK and CDL: performed quality control and ancestry analyses. JZ: performed association analyses and imputation under the guidance of BPT, BMG, RLT, GAY, KML and HLN: performed functional studies under the guidance of DU, LJA, and SAB, JZ, BMG, RLT, DU, BPT and SAB: prepared the manuscript. All authors approved the final draft.
Funding The quality of the RNA samples prepared from healthy human subjects was evaluated in the University of Colorado Cancer Center Microarray Core, which is supported by the NIH/NCI Cancer Core Support Grant (P30 CA046934). Flow cytometry was carried out in the Barbara Davis Center Flow Cytometry Core Facility, which was supported by National Institutes of Health (NIH) grant P30 DK57516. This work was also supported by the US National Institutes of Health [R01AI070983 (S.A.B, B.P.T., D.U.), K24AI078004 (S.A.B.), T32AR07534 (B.M.G.), K24AR002138 (R.R.G.), LRPAI071651 (T.B.N.), K08AI083790 (T.B.N.), N01AR062277 (J.B.H.), P01AI083194 (J.B.H.), P01AR049084 (R.P.K., J.B.H., J.C.E., E.E.B., G.S.A., J.D.R., R.R.G., and M.A.P.), P20RR020143 (J.B.H.), P30AR048311 (E.E.B.), P30AR053483 (J.A.J and J.M.G.), P30AR055385 (E.E.B.), P30GM103510 (J.A.J.), P60AR030692 (R.R.G.), P60AR062755 (D.L.K.), P60AR053308 (L.A.C.), R01AI063274 (P.M.G.), R01AR033062 (R.P.K.), R01AR042460 (J.B.H.), R01AR043274 (K.M.S.), R01AR43727 (M.A.P.), R01AR043814 (B.P.T.), R01AR051545 (A.M.S.), R01AR057172 (C.O.J.), R01CA141700 (M.E.A.R.), R21AI070304 (S.A.B.), R37AI024717 (J.B.H.), RC1AR058621 (M.E.A.R.), U01AI101934 (J.A.J. and J.M.G.), U19AI082714 (J.A.J. and J.M.G.), U54RR023417 (J.D.R.), UL1RR024999 (T.B.N.), UL1RR025014 (A.M.S.), UL1RR025741 (R.R.G.), UL1RR025777 (R.P.K. and J.C.E.), UL1RR029882 (D.L.K.), and UL1TR000004 (L.A.C.)], the Alliance for Lupus Research (S.A.B., B.P.T., D.U., K.M.S., T.B.N., L.A.C. and C.O.J.), the Lupus Research Institute (B.P.T., T.B.N.), the US Department of Veterans Affairs (Merit Awards; J.B.H., G.S.G.), the US Department of Defense (PR094002, J.B.H.), the Arthritis National Research Foundation (Eng Tan Scholar Award; J.Z. and T.B.N.), the Arthritis Foundation (A.M.S., and P.M.G.), the Korea Healthcare Technology R&D Project, Ministry for Health and Welfare, Republic of Korea (A121983; S.C.B.), the European Science Foundation RNP (BIOLUPUS Research Network), the Wellcome Trust (T.J.V.), Arthritis Research UK (T.J.V.), a Kirkland Scholar Award (L.A.C.), and the Wake Forest School of Medicine Center for Public Health Genomics (C.D.L.). The funders had no role in study design, data collection, analysis and interpretation, writing of the report or decision to submit the paper for publication.
Competing interests None.
Ethics approval IRB at University of Colorado School of Medicine and multiple institutions.
Provenance and peer review Not commissioned; externally peer reviewed.