Abstract
The Oct2 protein, encoded by the Pou2f2 gene, was originally predicted to act as a DNA binding transcriptional activator of immunoglobulin (Ig) in B lineage cells. This prediction flowed from the earlier observation that an 8-bp sequence, the “octamer motif,” was a highly conserved component of most Ig gene promoters and enhancers, and evidence from over-expression and reporter assays confirmed Oct2-mediated, octamer-dependent gene expression. Complexity was added to the story when Oct1, an independently encoded protein, ubiquitously expressed from the Pou2f1 gene, was characterized and found to bind to the octamer motif with almost identical specificity, and later, when the co-activator Obf1 (OCA-B, Bob.1), encoded by the Pou2af1 gene, was cloned. Obf1 joins Oct2 (and Oct1) on the DNA of a subset of octamer motifs to enhance their transactivation strength. While these proteins variously carried the mantle of determinants of Ig gene expression in B cells for many years, such a role has not been borne out for them by characterization of mice lacking functional copies of the genes, either as single or as compound mutants. Instead, we and others have shown that Oct2 and Obf1 are required for B cells to mature fully in vivo, for B cells to respond to the T cell cytokines IL5 and IL4, and for B cells to produce IL6 normally during a T cell dependent immune response. We show here that Oct2 affects Syk gene expression, thus influencing B cell receptor signaling, and that Oct2 loss blocks Slamf1 expression in vivo as a result of incomplete B cell maturation. Upon IL4 signaling, Stat6 up-regulates Obf1, indirectly via Xbp1, to enable plasma cell differentiation. Thus, Oct2 and Obf1 enable B cells to respond normally to antigen receptor signals, to express surface receptors that mediate physical interaction with T cells, or to produce and respond to cytokines that are critical drivers of B cell and T cell differentiation during a humoral immune response.
Introduction
Octamer binding protein 2, or Oct2, is encoded by the Pou2f2 gene. It was one of the first cell type-specific transcription factors identified and cloned (). As indicated by its name, it is a founding member of a family of DNA binding proteins concurrently discovered, that share a conserved bipartite DNA binding domain comprising a homeobox-like domain and a second conserved sequence entitled the POU domain, for the Pit1, Oct1/Oct2, Unc86 proteins (). Oct2 binds to a conserved consensus DNA sequence, the “octamer motif” found in the promoters and enhancers of many genes, including those encoding immunoglobulins (, ). The Obf1 protein encoded by the Pou2af1 gene, which is also known as OCA-B and Bob.1 was subsequently cloned using a yeast 1-hybrid screen for B cell proteins that physically interact with Oct1 or Oct2 (–). While Oct1/Oct2 and Obf1 share the capacity to bind to and activate genes adjacent to octamer motifs, they are selective in the genes to which they bind. The selectivity of target gene binding is determined, in part, by the sequence of the octamer motif, and whether it conforms to one of two classes of site, designated “PORE” and “MORE” motifs (). Whether binding mediates activation or repression is also influenced by the participation of cofactors [reviewed by Tantin ()], including Obf1, which can potentiate the transactivation potential of Oct1 and Oct2 (, ).
Oct2 is expressed primarily but not exclusively in the B cell lineage, where it increases with cellular activation (). Neurons, macrophages, and T cells have also been shown to express Oct2 (–). Oct2 is required for post-natal survival (), so must regulate critically important genes outside of the immune system. These will not be discussed here. The Oct2 gene is large, displays complex splicing patterns, and encodes protein isoforms with multiple essential activation domains (–). Oct2 is largely localized to the nucleus. Obf1 expression is mostly restricted to B lineage cells, where it is also highly induced upon activation (). Zwilling et al. () have reported expression in T cells, but myeloid cells do not express Obf1 (). A small protein of ~35 kDa, Obf1 is found in both the nucleus and cytoplasm, where a proportion may be tethered to the cell membrane after post-translational myristoylation (), and a potential role for membrane-associated Obf1 in B cell receptor (BCR) signaling has been proposed ().
A series of studies have shown that Oct2 and Obf1 are required for full functional and phenotypic maturation of B cells. In single knockout (KO) mice of each gene, peripheral B cells are numerically reduced and display some features of immature transitional cells (, ). The peritoneal B1 and splenic marginal zone (MZ) populations are missing in Oct2−/− mice (, ). Obf1−/− mice are viable and fertile, but show B cell developmental defects (, ), have an expanded B1 cell population (). They also lack MZ B cells () and completely fail to produce germinal centers (GCs), the sites of cognate B cell:T cell interaction and expansion, upon immunization, or infection (–). Both Oct2- and Obf1-deficient splenic B cells display aberrant responses to BCR signaling and other characteristics of immature B cells (, , ). Oct2-deficient B cells also fail to respond to lipopolysaccharide (LPS), which signals through TLR4 (). In vivo, serum immunoglobulin (Ig) levels in both mutants, particularly those that are T cell dependent, are strongly reduced (–, ). Mice doubly deficient for Oct2 and Obf1 show a stronger humoral deficiency phenotype, reflecting the distinct activities of the two factors, but still express Ig genes (). Thus, the two factors are not required, singly or in combination, for Ig gene expression by B cells.
Detailed functional studies on Oct2- and Obf1-deficient B cells in vitro and in vivo have identified a number of genes regulated by the two factors. Oct2 directly regulates the gene encoding CD36, a class B scavenger receptor family (), but only in B cells, not in macrophages or dendritic cells (–). However, no role for CD36 in B cells has been determined (). Oct2-deficent B cells have been shown to be defective in their responses to the T cell cytokine IL5 as a result of the direct regulation of the Cd125 gene encoding the IL5Rα chain (). IL5 promotes antibody-secreting cell (ASC) differentiation in mouse B cells (), and Oct2−/− B cells are defective in this process (). In another study, it was shown that both Oct2 and Obf1 contribute to the regulation of IL6 production by activated B cells, through direct effects, at least by Oct2, on the Il6 gene (). As Obf1 does not contact DNA (), it is difficult using current procedures to prove direct interaction of Obf1 with putative target gene loci. IL6 is important during T follicular helper (Tfh) cell polarization (). We have also shown, using the same quantitative tools that identified the role of Oct2 and IL5 in ASC differentiation, that Obf1 is required for T cell dependent ASC differentiation, but not isotype switching, both in vitro and in vivo ().
In addition to these established roles for Oct2 and Obf1 in B cells, we include below data from studies on other genes that we have found to be differentially regulated in Oct2- and Obf1-deficient B cells. These include the genes encoding the Syk protein, which is an important transducer of BCR signals and Slamf1, an essential mediator of cell:cell contact, especially in the context of a developing GC. Expression of Syk and Slamf1 are sensitive to Oct2 loss, through different mechanisms. We also show that Obf1 is downstream of Stat6 in the IL4 signaling pathway of B cells, with Xbp1, another Stat6 target, its direct activator. We include these data to add to our understanding of the valuable roles that Oct2 and Obf1 play in B cell responses to antigen and to T cell help.
Results
Consistent with their distinct roles in vivo, Oct2 and Obf1 have quite distinct patterns of expression in peripheral B cells, as measured by RNAseq of sorted populations from naive C57BL/6 mice (Figure 1A). Oct2 levels are highest in B1 cells of the peritoneal cavity, and decline with terminal differentiation to ASCs. In contrast, Obf1 levels peak in GC B cells, which require Obf1 for their generation, and remain high in ASC. For contrast, expression of Syk and Slamf1 in the same populations are shown in Figure 1A, as these two genes are influenced directly and indirectly, respectively, by Oct2, and will be discussed below.
Figure 1
Oct2 modulates B cell receptor signaling by fine-tuning Syk expression
A microarray screen for Oct2-dependent genes identified the tyrosine kinase Syk as a potential target gene. Characterization of the murine Syk promoter using 5′ RACE identified two alternative transcriptional initiation sites (Figure 1B) that append alternative 5′ non-coding exons to Syk mRNAs in B cells. Both transcripts encode the same protein, as the start of Syk translation lies in an exon common to the two transcripts. RNAseq data for Syk in sorted B cell populations show that the usage of exons 1 or 2 varies subtly among them (Figure 1C).
The promoter upstream of exon 2 is positively regulated by Oct2. B cells sorted from Oct2−/− mice (Figure 2A) have a lower level of Syk transcripts and protein than wild type (WT) mice (Figures 2B,C). Using qPCR to distinguish Syk transcripts derived from exon 1 or exon 2, we found that those derived from exon 2 were selectively reduced in Oct2−/− B cells (Figure 2D). To confirm the influence of Oct2 on the Syk exon 2 promoter, we stably introduced an estradiol-inducible form of Oct2 () into a cloned Oct2−/− B lymphoma cell line, OM1 (). Upon treatment with estradiol, there was no effect on expression from exon 1 with either the vector only control or the inducible Oct2 construct. However, estradiol induction of Oct2 selectively enhanced Syk expression from exon 2 and culminated in markedly increased Syk mRNA levels (Figures 2E,F). A DNA sequence search revealed three perfect consensus octamer sequences in the Syk gene (Figure 1B). Chromatin immunoprecipitation (ChIP) of Oct2 on DNA from the WT B lymphoma WEHI231 showed strong enrichment of DNA from the promoter of the known Oct2 target gene Cd36 (Figure 2G). The DNA adjacent to the perfect octamer sequence upstream of exon 2 was also significantly enriched in the ChIP, but adjacent sequences in intron 1/2 were not. Thus, Oct2 can directly increase Syk levels in B cells, acting at one of two alternative promoters.
Figure 2
As mentioned above, Oct2 is required for the full functional and phenotypic maturation of B cells, such that peripheral B cells in Oct2−/− mice are numerically reduced and display some features of immature transitional cells, and the B1 and MZ populations are missing (, , ). Like transitional B cells, Oct2-deficient B cells are killed rather that activated by BCR cross-linking [Ref. (, ); see also Figure 3A]. However, Oct2−/− B cells respond normally to the survival factor Baff/BlyS, and survive to expand normally when BCR signaling occurs in the presence of Baff (Figures 3A,B and data not shown). Oct2−/− mice expressing a Bcl2 transgene still lack B1 and MZ B cells (data not shown). Thus abnormal survival properties are not responsible for the lack of these two populations in the Oct2 mutant mice.
Figure 3
We speculated that the reduced Syk levels in Oct2−/− B cells might contribute to their failure to mature in vivo and respond to BCR signals in vitro. We constructed a retroviral vector expressing Syk, and infected and cloned WT (BC1) and Oct2-deficient (OM1) lymphoma cells (Figure 3C). Boosting Syk protein levels enhanced the BCR response, as measured by calcium flux, in both WT and Oct2−/− cells (Figure 3D). Finally, using transduction of primary B cells (see Materials and Methods), we found that elevating Syk levels improved the proliferation of WT B cells, both unstimulated, and more strongly, upon BCR cross-linking, and that Oct2−/− B cells complemented with Syk retrovirus were activated to expand, rather than be killed by a BCR signal (Figure 3E). The rescue was not complete, as cell survival was still lower overall in the mutant cell cultures. This is likely to reflect technical limitations of the assay, including comparative infectivity of WT and mutant cells, and the correct timing of exogenous Syk expression in the context of the BCR signal. However, the results strongly suggest that Syk levels are limiting in Oct2−/− and, to a lesser extent, in WT B cells. We propose that Oct2 regulates Syk gene expression to enable positive selection through the BCR and therefore entrance to the mature follicular B cell pool, and it may similarly enable differentiation of B1 and MZ B cells, which are highly dependent on BCR signal strength.
Oct2 indirectly and selectively regulates Slamf1 expression on B cells
Slamf1 encodes CD150, a lymphocyte signaling and adhesion molecule () that is expressed in B cells and T cells and at very low levels in myeloid cells (see www.immgen.org). Our RNAseq analysis of activated B cells indicated that Slamf1 was expressed at abnormally low levels in Oct2 KO B compared to controls (Figure 4A). This was confirmed by flow cytometric analysis (Figure 4B). Resting WT and LPS-activated B cells expressed similar levels of Slamf1, but levels on Oct2-deficient B cells were much lower than controls under both conditions. Activated WT T cells up-regulated Slamf1 from resting levels. However, Slamf1 was not Oct2-dependent in resting or activated T cells, or in macrophages expanded from fetal liver, despite Oct2 normally being expressed in these cell types (, , ).
Figure 4
We next asked whether Slamf1 was a direct Oct2 target using cloned WT (WEHI231) and KO (OM1) B lymphoma lines transduced with the inducible Oct2-ER vector, as described above. As expected, the Oct2 target Cd36 gene was expressed in WEHI231 but not OM1 (Figure 4C). Estradiol treatment enhanced Cd36 levels in WEHI231, and strongly induced Cd36 expression in OM1 cells. However, Slamf1 expression, while low in the Oct2−/− line, was not increased by Oct2 induction. Therefore, Oct2 is unlikely to directly regulate Slamf1 transcription in B cells.
Examination of the pattern of expression of the Slamf1 gene during B cell development, using the Immgen database (http://www.immgen.org) and by flow cytometry of bone marrow (BM) and peripheral B cell populations indicated that Slamf1 is a marker of B cell maturation, appearing during the transition from immature (IgMhi/IgDlo) to mature (IgMlo/IgDhi) follicular B cells of the spleen (Figure 4D), with MZ B cells expressing intermediate Slamf1 levels. We conclude that loss of Oct2 blocks B cell maturation before the Slamf1+ stage, thereby indirectly regulating its expression.
It has been shown that B cells lacking Slamf1 cannot form the lasting interactions with Tfh cells that are required for GC formation (), and yet Oct2 mice do form GC upon infection and immunization (). We immunized WT and KO mice with SRBC and stained GC cells for Slamf1 9 days later. Oct2+/+ and Oct2−/−GC B cells expressed similar levels of Slamf1. This indicates that Oct2 is dispensable for Slamf1 expression, and that endogenous signals driving the GC response override the Oct2 maturation defect in vivo (Figure 4E). To explore the nature of these signals, we tested the capacity of a number of mitogens and cytokines to induce Slamf1 expression on Oct2-null B cells in vitro. Anti-μ, anti-CD40, Baff, and IL4, tested singly or in all possible combinations, failed to induce appreciable Slamf1 on Oct2−/− B cells, suggesting that other factors and cells contribute in vivo. Collectively these studies point to an Oct2-regulated differentiation step that enables efficient FoB cell maturation.
Obf1 enables T cell dependent ASC differentiation driven by IL4
We have shown that both Oct2 and Obf1 affect a B cell’s capacity to differentiate to ASC in response to particular cytokines, with Oct2 regulating the response to IL5 (), and Obf1 being essential for ASC differentiation driven by IL4 ().
We determined that Obf1 lies downstream of Stat6 in the IL4 signaling cascade (Figures 5A–C). Interestingly, while the IL4/Stat6 axis drives both isotype switching and ASC differentiation (), Obf1 is dispensable for IL4 driven switching (). In order to learn how IL4 and Stat6 regulate Obf1 expression, we performed microarray analysis on the WEHI231 B lymphoma, an IL4 responsive line. Because Stat6 exists in a latent form in the cytoplasm, and is activated by phosphorylation to enter the nucleus and act as a transcription factor (), direct Stat6 targets would be activated after IL4 signaling even in the absence of new protein synthesis. Cells therefore were treated with cyclohexamide (CHX) to inhibit translation, and 1 h later, IL4 was added. A parallel culture did not receive IL4. After another 4 h, RNA was prepared from both. Analysis using Illumina Sentrix Mouse v1.1 arrays identified a small number of genes whose expression rose two to fourfold during this short period of IL4 stimulation, genes likely to be regulated directly by Stat6. Among these were three transcriptions factors: Nfil3, Vdr, encoding the 1,25-dihydroxyvitamin D3 receptor, and Xbp1. Their induction under these conditions was validated by qPCR (Figure 5D). Interestingly, Obf1 transcription was not elevated by IL4 treatment in the presence of CHX, indicating that it is not a direct Stat6 target gene (Figure 5D).
Figure 5
As Obf1 RNA is elevated by IL4 treatment in B cells in the absence of CHX (Figure 5B), we hypothesized that one of the three transcription factors directly regulated by Stat6 might drive Obf1 expression. We therefore constructed ER fusion vectors for each to determine their effects on Obf1 expression. The Xbp1-ER expression vector contained the mature, processed, and active form of this factor (). Clones of each line were cultured for 24 h unstimulated, with estradiol to induce each fusion protein, or with IL4. IL4 caused an increase in Obf1 RNA levels in all cases, as expected. However, estradiol induction only increased Obf1 levels significantly in the Xbp-ER expressing cell line (Figure 5E). Finally, primary splenic B cells from Xbp1+/+, heterozygous and conditional KO mice were stimulated for 48 h with CD40 ligand and IL4, and protein extracts prepared. Western blots showed that Xbp1-null B cells express markedly less Obf1 than the controls (Figure 5F). These data indicate that Nfil3 and Vdr do not influence Obf1 expression, but that Xbp1 has the capacity to directly activate the Obf1 gene in response to IL4/Stat6 signaling in B cells.
Discussion
The data we present here adds to a growing view of Oct2 and Obf1 as essential contributors to the sensing capacity of B cells (Figure 6). These two factors enhance the cell’s ability to deliver a BCR signal to drive maturation, or to sense a foreign antigen and become activated. We show here that Oct2 may do so by fine-tuning Syk levels. Since Oct2 loss blocks peripheral B cell maturation, such that MZ B cells are missing and mature FoB reduced, Oct2 may play its most important role prior to a divergence point of Fo and MZ B cells (). The immature Slamf1−, BaffR+, CD23+, CD21+, IgMhi, Dlo, HSAhi phenotype of Oct2−/− B cells does not neatly fit into the phenotypic transition of immature to mature B cells (), and may represent a normally transient phase of B cell maturation. Obf1 is required for normal B cell maturation and MZ B cell development (), but as Obf1 does not influence Syk expression, it is likely that the two factors act through unique subsets of target genes for this aspect of B cell development. Indeed, it has been reported that Obf1 positively regulates SpiB gene expression (), and that SpiB is required for normal B cell maturation and BCR signaling, through regulation of c-rel (, ).
Figure 6
T cell dependent antibody responses depend upon Oct2 and Obf1 in several ways. Both Oct2 and Obf1 are required for B cells to produce normal levels of IL6, a cytokine important in Tfh maturation in the context of a Slamf1-mediated B cell:Tfh cell interaction (, , ). These molecular interactions enable the initiation of a fruitful T cell-dependent humoral immune response. For example, IL6 produced by activated B cells early in the GC response reinforces the early dendritic cell signal that initiates Tfh differentiation, and IL21 produced by the nascent Tfh enhances both Tfh function and B cell differentiation into GC B cells and ASC (–). Slamf1, which is indirectly dependent upon Oct2, is required to prolong the B:Tfh interaction while these important signals are exchanged. Subsequently, Oct2 and Obf1 enable B cells to respond to other Th cell cytokines that drive ASC differentiation. Oct2 regulates Cd125 expression (), and so expression of the high affinity receptor for IL5, an ASC differentiation factor (). Obf1 is required for a normal B cell response to IL4, a growth, survival, isotype switching and differentiation factor for B and plasma cells [(, ) and this study].
Except for the specific case of Obf1 and a subset of VL genes (), there is no evidence that Oct2 or Obf1 are required for Ig gene expression or for antibody secretion in ASC generated from single or double KO mice (, , ). Interestingly, however, we show here that Xbp1, which is highly expressed in ASC and known to be required for ASC function [(–) and our unpublished data], can directly activate Obf1. Shen and Hendershot () have also shown in ASC that Obf1 is a direct target of Xbp1. Accordingly, Obf1 expression is elevated in normal ASC compared to B cells, unlike Oct2 expression, which declines with differentiation (Figure 1). Xbp1, normally associated with the unfolded protein response in ASC, is an IL4 response gene in B cells. We confirm here that Obf1 is an Xbp1 target gene in FoB cells, and that IL4 and Stat6 directly induce Xbp1. Iwakoshi et al. () have earlier shown that, in the context of ASC differentiation, IL4 strongly induces Xbp1 expression and Stat6 is required. Thus, the selective ASC differentiation defect in Obf1 null B cells under T cell-dependent conditions may reflect an important Stat6-Xbp1-Obf1 axis.
Instead of direct influences on Ig gene expression, poor humoral immune responses in Oct2 or Obf1 mutant mice more likely reflects a paucity of differentiated peripheral B cell populations and weak to absent influences of T cells on these B cells. Oct2 and Obf1 are most highly expressed in GC B cells, with Obf1 being essential for their differentiation, but Oct2 dispensable (). In both mutants, the B cells defects are cell intrinsic. Outstanding questions remain: what are the genes that Oct2 and Obf1 regulate to ensure full peripheral maturation and competent BCR signaling? What are the Obf1 regulated genes that are essential for GC development under all circumstances tested so far, including immunization, infection, and autoimmunity (, , )? While these critical Obf1 target(s) are not yet known, candidates such as Bcl6 (or its co-repressor MTA3), Bach2, Irf4 and CXCR5, all critical for normal GC formation or maintenance [see Ref. ()], can be excluded, as they are not influenced by Obf1 loss (our unpublished data). Ongoing genome-wide RNA expression analysis, coupled with ChIPseq, will enable detailed characterization of the full Oct2 and Obf1 gene regulatory networks, and their shared and unique responsibilities in delivering effective B cell immunity.
Materials and Methods
Cell lines, cell culture, and retroviral transduction
B lymphoma cell lines used here were all generated in house: WEHI231 (), BC1, and OM1 (). Primary splenic B and T cells were purified using anti-B220 or anti-CD4 microbeads (Miltenyi), as described (). Oct2+/+ and Oct2−/−macrophages were expanded in vitro from E13 fetal liver using M-CSF, as described (). Retroviral transduction in all cases used the pMX-pie vector and was preformed using spin infection as described (, ). For lymphoma lines, cells were cloned post-infection as single GFP+ cells in puromycin-supplemented medium.
For the retroviral complementation experiment of Figure 3E, primary splenic B220+ cells were stimulated for 24 h with CpG [1 μM oligonucleotide CpG 1668 (sequence 5′-TCCATGA CGTTCCTGATGCT-3′), fully phosphothioated GeneWorks] to promote cell cycling and enable retroviral infection. After overnight culture, cells were washed and resuspended in medium at 0.5 × 106 cells/ml, without CpG but containing anti-μ [10 μg/ml AffiniPure F(ab′)2 fragment, goat anti mouse Jackson Laboratories] and/or Baff (250 ng/ml a kind gift from Jürg Tschopp). Cell survival in transduced (GFP+) cells was assessed after a further 48 h by flow cytometry, propidium iodide exclusion, and cell counting using internal microbead controls.
Retroviruses expressing transcription factors fused to the human estrogen receptor (hER) dimerization domain were generated by amplification of each factor’s ORF, and sequencing each amplified product to ensure it was mutation-free and in frame with the hER. Production of ER fusion proteins of the correct size was confirmed by western blots of infected or transfected cells. Anti-CD40 (clone FGK4.5) was prepared in house and used at 10 μg/ml. β-Estradiol (Sigma) was used at 10 μM, cycloheximide at 50 μM.
Mice
Oct2−/−, Obf1−/−, and Stat6−/− mice have been described previously (, ) Xbp1fl/flCd19Cre/+mice, where Xbp1 is conditionally deleted in the B cell lineage, were generated by Hetz et al. () and further described in Taubenheim et al. (). All mice were maintained on a C57BL/6 background, and all experiments conformed to the relevant regulatory standards of the Animal Ethics Committee of the Walter and Eliza Hall Institute of Medical Research (AEC Projects 2010.010 and 2013.014).
Antibodies
For westerns, antibodies used were specific for Oct2 (clone 9A2, in house), Obf1 (clone 6F10, in house) Stat6 (S-20), Syk (N-19), and actin (I-19) all from Santa Cruz and Xbp1 (Ab37152-100, Abcam). For flow cytometry, antibodies used were specific for B220 (RA3-6B2), IgD (11-26c.2a), fas/CD95 (Jo2), all from BD Pharmingen Slamf1/CD150 (TC15-12 F12.2, Biolegend), and GL7 (eBioscience). Calcium flux was assessed cytometrically as described (78).
Microarrays
Illumina Sentrix Mouse v1.1 arrays were probed with RNA prepared from independent B lymphoma cell lines: to identify Oct2-dependent genes, two independent clones of OM1 cells stably transduced with a control vector or one expressing an estradiol-inducible Oct-ER fusion protein were treated in vitro for 6 or 48 h with estradiol prior to RNA preparation. For Obf1 targets, two clones of the Obf1−/− BM1 lymphoma line (78), transduced with vector control or an Obf1-ER expression vector, were induced in a similar manner and RNA prepared and analyzed.
RNA sequencing
Peripheral B cell populations were sorted from naïve or immunized C57Bl/6 mice as described in the legend to Figure 1. Two independent biological replicates were prepared for each population, except for spleen and BM ASC. Because of the paucity of ASC in these tissues, cells were pooled from three to four individuals before sorting. Two such pools were processed independently for sequencing. Normalized expression levels are shown in the graphs. As more than 70% of reads in RNA from ASC map to the Ig loci, all Ig reads were excluded from the data, for all populations, before normalization to generate the values shown in Figure 1A. Specifically, all reads from the IgH locus on chromosome 12, NC_000078.6 (positions 113,258,768–116,009,954), all reads from the Igλ locus on chromosome 16, NC_000082.6 (positions 19,026,858–19,260,844), and all reads from the Igκ locus on chromosome 6, NC_000072.6 (positions 67,555,636–70,726,754) were excluded. For Figure 2B, Oct2+/+ and Oct2−/−B cells were sorted, as in Figure 2A, from spleen of two independent mice of each genotype and activated for 48 h before RNA extraction and preparation for sequencing. As these conditions do not induce ASC differentiation, Ig sequence reads were not excluded from analysis of these samples.
Primers
The starts of Syk transcription in primary B cells were determined directly using FirstChoice® RLM-RACE (Ambion) and nested Syk gene specific primers specific for the first Syk coding exon: 5′-GTAGGTCAGGTGGTTGGCGCTGTCCACAGC-3′ and 5′-CCCGCCATGTCTGCACCCCTTCAGAGTTC-3′.
For exon-specific
SykqPCR, these primers were used:
5′Syk exon 1: 5′-CAGTGACTGCGGCTGAGCGCGGACC-3′
5′Syk exon 2: 5′-CAGCAGGAAACCTCCACTTGCTCTCC-3′
Common 3′ Syk primer: 5′-CCATGTCTGCACCCCTTCAGAGTTC-3′.
For
SykChIP PCR, these primers were used:
Exon 2: fwd 5′-GCCTAGGCCACGATGGTCAAAGGAGG-3′ and
rev 5′-GGAGAGCAAGTGGAGGTTTCCTGCTG-3′.
Upstream of exon 2: fwd 5′-CCATTGGTGGGCCCTCAGCTTGGTTC-3′ and
rev 5′-GACCAGAGAAGAAATGGCCTCAGAAGACAGG-3′.
Chromatin immunoprecipitation was conducted as previously described (), using high titer, polyclonal anti-Oct2 rabbit serum generated in house.
Primers for other qPCR were:
Stat6: fwd 5′-CTGCTGGGCCGAGGCTTCACATTT-3′
rev 5′-TCAGGGGCCATTCCAAGATCATAAGGT-3′
CD36: fwd 5′-GGAGGCATTCTCATGCCAGTCGGAGAC-3′
rev 5′-CAAAACTGTCTGTACACAGTGGTGCCTG-3′
Slamf1: fwd 5′-GGGAGCTATCCAGATCACCTG-3′
rev 5′-CGTTCTCCTCCACGCTCAC-3′
Cd23: fwd 5′-GACACTGCAATTCAGAATGTCTCTCATG-3′
rev 5′-GCTTCTGTTCAGCTTGGAGTTCTTGCAAG-3′
Nflil3: fwd 5′-CTCACGGACCAGGGAGCAGAACCACG-3′
rev 5′-CAGGTCTTAAGGACTTCAGCCTCTCATCC-3′
Obf1: fwd 5′-CGGTGTTGACCTATGCTTCTCCACC-3′
rev 5′-GAGGGGCGCCTGGTGCTCGGGACCC-3′
Vdr: fwd 5′-CGCTATGACCTGTGAAGGCTGCAAGGG-3′
rev 5′-GCCAATGTCCACGCAGCGTTTGAGCC-3′
Xbp1: fwd 5′-AGCAGCAAGTGGTGGATTTG-3′
rev 5′-CCAAGCGTGTTCTTAACTCCT-3′
Hmbs (for normalization): fwd 5′-GACCTGGTTGTTCACTCCCTGAAG-3′
rev 5′-GACAACAGCATCACAAGGGTTTTC-3′
Chromatin immunoprecipitation PCR and qPCR were performed on triplicate samples in all cases, and the data presented as means ± SD. Statistical significance was determined using the unpaired Student’s t-test.
Immunization
Mice stably reconstituted with Oct2+/+ or Oct2−/−fetal liver were immunized i.p with 2 × 109 sheep red blood cells (Applied Biological Product Management, Australia) in 100 μl of PBS and sacrificed after 9 days.
Statements
Author contributions
Lynn Corcoran performed many of the experiments and wrote the manuscript; Dianne Emslie and Tobias Kratina together performed all of the qPCR and protein analyses; Wei Shi performed all bioinformatics analysis for the RNAseq experiments; Susanne Hirsch performed the Slamf1 studies; Nadine Taubenheim contributed to the Xbp1 studies; Stephane Chevrier led most of the flow cytometric analyses.
Acknowledgments
We thank Drs. Laurie Glimcher for conditional Xbp1 mutant mice and Patrick Matthias for Obf1 mice, Gordon Smythe for bioinformatics assistance and Stephen Nutt for critical comments on the manuscript. Jennifer Vasiliadis and Louise Inglis provided expert animal care. This work was made possible through Victorian State Government Operational Infrastructure Support and Australian Government NHMRC IRIIS and research grants from the NHMRC (#637306 and #575500).
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
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Summary
Keywords
Oct2, Obf1, Syk, Slamf1, B:T collaboration, cytokines
Citation
Corcoran L, Emslie D, Kratina T, Shi W, Hirsch S, Taubenheim N and Chevrier S (2014) Oct2 and Obf1 as Facilitators of B:T Cell Collaboration during a Humoral Immune Response. Front. Immunol. 5:108. doi: 10.3389/fimmu.2014.00108
Received
24 December 2013
Accepted
03 March 2014
Published
20 March 2014
Volume
5 - 2014
Edited by
Ananda L. Roy, Tufts University School of Medicine, USA
Reviewed by
Mikael Sigvardsson, Linköping University, Sweden; Bruce David Mazer, Montreal Children’s Hospital, Canada
Copyright
© 2014 Corcoran, Emslie, Kratina, Shi, Hirsch, Taubenheim and Chevrier.
This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Lynn Corcoran, Walter and Eliza Hall Institute of Medical Research, 1G Royal Parade, Melbourne, VIC 3052, Australia e-mail: corcoran@wehi.edu.au
†Present address: Stephane Chevrier, Institute of Molecular Life Sciences, University of Zurich, Zurich, Switzerland
This article was submitted to B Cell Biology, a section of the journal Frontiers in Immunology.
Disclaimer
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article or claim that may be made by its manufacturer is not guaranteed or endorsed by the publisher.