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XLID syndrome gene Med12 promotes Ig isotype switching through chromatin modification and enhancer RNA regulation

The transcriptional coactivator Med12 regulates gene expression through its kinase module. Here, we show a kinase module–independent function of Med12 in CSR. Med12 is essential for super-enhancer activation by collaborating with p300-Jmjd6/Carm1 coactivator complexes. Med12 loss decreases H3K27 acetylation and eRNA transcription with concomitant impairment of AID-induced DNA breaks, S-S synapse formation, and 3′RR-Eμ interaction. CRISPR-dCas9–mediated enhancer activation reestablishes the epigenomic and transcriptional hallmarks of the super-enhancer and fully restores the Med12 depletion defects. Moreover, 3′RR-derived eRNAs are critical for promoting S region epigenetic regulation, synapse formation, and recruitment of Med12 and AID to the IgH locus. We find that XLID syndrome–associated Med12 mutations are defective in both 3′RR eRNA transcription and CSR, suggesting that B and neuronal cells may have cell-specific super-enhancer dysfunctions. We conclude that Med12 is essential for IgH 3′RR activation/eRNA transcription and plays a central role in AID-induced antibody gene diversification and genomic instability in B cells.


INTRODUCTION
Upon antigen encounter, mature B cells undergo immunoglobulin (Ig) class switch recombination (CSR) to allow transition of Ig isotype expression from IgM to IgG, IgA, or IgE (1). At the genetic level, the IgM constant gene is replaced by one of the downstream constant genes through Ig locus-specific DNA rearrangement induced by activation-induced deaminase (AID) (2,3). This programmed DNA arrangement involves three critical steps: (i) GLT through long intronic S regions, (ii) targeted DNA breaks in recombining S regions, and (iii) joining cleaved S region pairs by nonhomologous end joining (NHEJ)-mediated repair (4,5). AID plays a central role in these processes by inducing DNA cleavage at specific loci and promoting S-S synapse (unique cis conformation) formation to facilitate recombination (6,7). Although the requirement of AID in DNA cleavage and S-S synapse formation is well established, the precise mechanism of locus specificity and S-S tethering has yet to be fully understood.
The IgH 3′RR super-enhancer region plays an important role in AID-induced CSR (8,9) and somatic hypermutation (10) but not in recombination-activating genes (RAG)-induced V(D)J recombination (11). However, how 3′RR cis-regulatory elements influence and/or regulate AID-induced actions during CSR remains poorly understood. The most prevalent and widely accepted view suggests that the 3′RR is mainly involved in GLT (12,13), which is one of the essential prerequisites that precedes AID-induced CSR. The core 3′RR encompasses four transcriptional enhancers (hs3a, hs1.2, hs3b, and hs4), and deletion of all four decreases the GLTs, with expected decreases in CSR (9,13). These 3′RR enhancers are thought to function cooperatively, as their individual deletion does not impair Ig isotype switching. However, deletion of both hs3b and hs4 decreases CSR for all isotypes except IgG (8). In summary, the precise mechanisms underlying 3′RR-dependent CSR regulation remains unsettled despite studies demonstrating the cumulative activity of individual enhancers, such as hs1.2 and hs4, or in combination with hs3b (14).
Enhancers and super-enhancers are typically considered to be distally located gene regulatory elements that enhance transcription by long-distance interaction with gene promoters (15,16). Enhancer activation requires formation of specific protein complexes that include transcription factors (TFs), co-regulators, chromatin remodelers and modifiers, and RNA polymerase II (RNAPII) (15)(16)(17). One enhancer coactivator is the supramolecular Mediator complex, which serves as a signaling coordinator between transcriptional machinery and RNAPII through modulating subunit composition (18,19). Mediator is assembled as four subcomplexes referred to as "head," "middle," "tail," and "kinase" modules (20,21). While the head, middle, and tail modules comprise the core Mediator, the fourth module reversibly interacts with the core through its Med13 subunit. The kinase module is composed of Med12, Med13, Cdk8, and cyclin C and contributes to both negative and positive regulation of RNAPII-driven transcription (21)(22)(23).
The N-terminal leucine-rich (L) domain of Med12 is responsible for cyclin-dependent kinase 8 (CDK8) activation, representing a kinase module-dependent function of Med12 (24). Notably, while leukemia-and uterine leiomyoma (UL)-associated mutations are localized within the L domain, X-linked intellectual disability (XLID)-associated mutations, including atypical and typical FG, Lujan, Opitz-Kaveggia, or Ohdo syndrome, are distributed across the central leucine-and serine-rich (LS) domain (25). Several prostate cancer-related mutations are also located in the LS as well as proline-, glutamine-, and leucine-rich (PQL) domain (25). The PQL domain is adjacent to the LS domain and is subject to arginine methylation at several positions, which likely contributes to noncoding RNA (ncRNA) binding and protein-protein interactions (26). In addition, some PQL domain mutations may confer chemotherapeutic resistance in cancer (27). Mutations in the C-terminal odd-paired area glutamine-rich (OPA) domain of Med12 has been reported in three siblings with low IgG levels and B cell proliferation defects (28). Although Med12 mutations mentioned are thought to be crucial for disease progression, the functional significance and molecular mechanisms of these mutations remain poorly understood.
Here, we use various domain-specific Med12 mutations to determine Med12 structure-function relationships within the context of AID-induced genomic instability in mature B cells. We find that Med12 is dispensable for switch GLT but is indispensable for 3′RR activation and transcription. We also find that these Med12 functions are independent of kinase module function. Mechanistically, Med12, in collaboration with p300 and Jmjd6/coactivator-associated arginine methyltransferase 1 (Carm1) complexes, preserves signature histone epigenetic marks at 3′RR and S regions, resulting in adequate enhancer RNA (eRNA) production and unperturbed CSR. Loss of Med12 leads to both architectural and epigenomic dysregulation of the IgH locus, abrogating AID-induced DNA doublestrand breaks (DSBs) and postbreak recombination/repair processes essential for Ig isotype switching.

Med12 is required for AID-induced DNA breaks and S-S synapse formation during CSR
To investigate the requirement of Med12 in CSR, we established a small interfering RNA (siRNA)-mediated Med12 gene knockdown (KD) (Med12 KD ) model in the murine B cell line CH12F3-2A. This cell line efficiently switches from IgM to IgA in response to stimulation with CD40L, interleukin-4 (IL-4), and transforming growth factor-β (TGF-β) (CIT) (29). Multiple siMed12 concentrations effectively inhibited CSR with a clear trend of dose dependency ( Fig. 1A and fig S1A). We subsequently used 20 pmol of siMed12 in all the experiments, as it did not affect cell proliferation. To confirm KD specificity, we designed a wild-type Med12 (WT R ) construct capable of producing Med12 transcripts resistant to degradation by siMed12 (Fig. 1B, top). Transfection of cells with the Med12 WT R construct showed a dose-dependent CSR complementation in Med12 KD cells (Fig. 1B). These results suggest that Med12 plays a critical role in CSR and may be specifically required for effective CSR.
We confirmed that Med12 deficiency did not affect switch GLT, μGLT, and αGLT or AID expression ( Fig. 1C and fig. S1A). Consistently, Med12 depletion did not affect AIDER [AID fused with estrogen receptor (ER)] expression but strongly impaired CSR in the AIDER-CH12F3-2A line (fig. S1, B and C). To examine the exact steps of CSR that are impaired following Med12 depletion, we assessed AID-induced DNA DSB formation in the S region by linker ligation-mediated polymerase chain reaction (LM-PCR) (30). Med12 depletion results in a sharp decrease in DNA DSB signals, which are restored to control levels with cotransfection of the Med12 WT R construct ( Fig. 1D and fig. S1D), suggesting that AID-induced DNA DSB formation requires Med12. Consistently, γH2AX, a marker of early DNA damage response (DDR) signaling, was also diminished at the Sμ and Sα regions in Med12 KD cells (Fig. 1E).
IgA CSR requires a unique cis conformation of the IgH locus known as the S-S synapse. This synapse brings the donor Sμ and the acceptor Sα into close proximity by looping out a large intervening sequence region. S-S synapse formation detection assays have included standard chromosome confirmation capture (3C), which enables detection of S-S proximity as a hybrid PCR product of two widely separated loci, namely, Sμ and Sα. Similarly, 3C assays can be used to detect the proximity or long-range interactions between promoters and enhancers (Eμ-3′RR) or interaction with novel loci other than IgH. In Med12 KD cells, we find that the intensity of Sμ-Sα hybrid PCR products was strongly decreased (Fig. 1F), suggesting that Med12 is required for proper S-S synapse formation during CSR. Depletion of Med12 also markedly diminished the interaction between Eμ and 3′RR, providing further evidence for the role of Med12 for both constitutive (Eμ-3′RR) and inducible (S-S) locus conformation.
As AID expression induces IgH/c-Myc translocation in addition to CSR in B lymphocytes, we next examined IgH/c-Myc translocation frequency by PCR amplifying translocated genomic DNA junctions from siControl-and siMed12-transfected cells. PCR products were subjected to Southern hybridization using c-Myc locus-specific probe (31). Med12 depletion resulted in a reduction of AIDinduced IgH/c-Myc translocations (Fig. 1G). Similarly, Med12 depletion also counteracted augmentation of IgH/c-Myc translocations by Topoisomerase 1 (Top1) deficiency.
Ligation of DSB ends between two S regions mainly occurs through the NHEJ-mediated DNA repair pathway; we next examined the impact of Med12 deficiency in an NHEJ-mediated repair assay using I-SceI meganuclease-induced DSBs (32). In this assay, a green fluorescent protein (GFP) reporter gene is expressed only after successful NHEJ between two cleaved I-SceI sites, removing an intervening thymidine kinase gene cassette. The I-SceI-expressing plasmid was cotransfected with siControl or siMed12 into the reporter cell line, H1299dA3-1. As expected, in siControl-treated cells, I-SceI expression showed 12.6% GFP CIT (+) cells, which was reduced to 3.4% in siMed12-treated cells, suggesting that DSB end joining via NHEJ requires Med12 ( fig. S1E). Together, we conclude that Med12 is vital for promoting AID-induced DNA DSBs, S-S synapse formation, and NHEJ, all of which are essential for Ig isotype switching.

S region DNA break and synapse formation are regulated by distinct domains of Med12
To understand the molecular basis of the diverse functions of Med12, we examined Med12 structure-function relationships by generating several deletion and point mutant constructs. Med12 is a large protein with four distinct domains ( Fig. 2A): an L domain, an LS domain, a PQL, and an OPA domain. We generated individual domain-specific deletions using WT R sequence as a template ( Fig. 2A). CSR complementation efficiency of these mutants was measured relative to Med12 KD cells transfected with the WT R construct. We find that the ΔL R , ΔOPA R , and ΔNLS R (nuclear localization signal) mutants display WT-level CSR complementation, whereas ΔLS R and ΔPQL R show a substantial loss of CSR activity (Fig. 2B). We find that when CSR-defective ΔLS R and ΔPQL R constructs are cotransfected, CSR is restored back to WT R levels (Fig. 2B). However, as individual LS and PQL domains were intact in the respective ΔPQL R and ΔLS R mutants, we suspect that functional cross-complementation occurs between these two domains.
To further examine this possible cross-complementation, we tested whether ΔLS R and ΔPQL R mutants can support AIDinduced DNA DSBs and S-S synapse formation by LM-PCR and 3C assays. LM-PCR results suggest that the ΔLS R mutant is severely defective in S region DSB formation in Med12 KD cells, which is consistent with this mutant's CSR deficiency (Fig. 2B). Conversely, S region DNA break signals were detected in Med12 KD cells transfected with ΔL R , ΔPQL R , ΔLS R + ΔPQL R , and ΔOPA R mutants (Fig. 2C). Notably, ΔPQL R rescued the severe DNA break defect in ΔLS R -transfected Med12 KD cells. Together, we conclude that the LS domain of Med12 plays a critical role in AID-induced S region DNA break. We next examined the contribution of the ΔLS R and ΔPQL R mutants and their coexpression (ΔLS R + ΔPQL R ) in S-S synapse formation. We find that Med12 depletion significantly reduces Sμ-Sα and Eμ-Sα interactions, while WT R transfection of Med12 KD cells restores these interactions (Fig. 2D). We find that neither ΔLS R nor ΔPQL R transfection restores Sμ-Sα or Eμ-Sα interaction in Med12 KD cells. However, we find that cotransfection of both ΔLS R and ΔPQL R rescues Sμ-Sα and Eμ-Sα interactions, suggesting that both the LS and PQL domain are required for synapse formation.
As only cotransfection of ΔLS R and ΔPQL R restored DNA break and synapse, it suggested a functional cross-complementation by the two domains, presumably through their interaction, if Med12 forms a homodimer or multimer. To examine the possibility, we performed coimmunoprecipitation (Co-IP) of differentially epitope-tagged (V5 and Flag and vice versa) LS and PQL domains, as depicted in Fig. 2E. The Co-IP result suggests that the LS and PQL domains form homodimers and also interact with each other. Moreover, the complex also pulled down p300 histone acetyltransferase (HAT), an essential interacting partner of Med12 for its function in CSR, as we revealed in the subsequent sections. Furthermore, to examine whether Med12 mutations observed in human disease have CSR defects, we tested several reported point mutations across multiple Med12 protein domains (table S1). Because the LS domain is associated with XLID, we also included two previously unknown LS domain mutations (R1138H and R1463C) that were generated during the site-directed mutagenesis process. We find that mutations in the LS (R521H, R1138H, L1224F, and R1463C) and PQL (H1729N, R1862K, and R1899K) domains show diminished CSR activity ( Fig. 2F and table S1). Point mutants that induced significant CSR defects (R1138H, R1463C, R1862K, and R1899K) were further examined for their ability to promote AID-induced DNA DSBs. LM-PCR assays show that impaired DNA DSB formation in Med12 KD cells can be restored by complementation with PQL domain mutants (R1862K and R1899K) but not by LS domain mutants (R1138H and R1463C) (Fig. 2G). Despite promoting DNA DSBs as efficiently as WT Med12, PQL mutants were CSR defective ( Fig. 2F and table S1), likely because of their recombination defects. Together, we suggest that Med12 regulates two distinct steps of CSR, namely, AID-induced DNA DSBs using its LS domain and S region synapse formation using its PQL domain.

The transcription regulatory kinase module of Med12 is dispensable for CSR
The N-terminal L domain of Med12 plays an important role in transcriptional regulation through its interaction with the kinase module and the core Mediator (20). The Mediator kinase module is composed of Med12, cyclin C, Cdk8/Cdk19, and Med13. This kinase module reversibly interacts with the core Mediator through Med13 and contributes to gene expression regulation ( Fig. 3A) (33). As Med12 stimulates Cdk8/19 kinase activity through cyclin C-dependent interaction, loss of Med12 or a defect at the N terminus disrupts kinase complex formation, resulting in gene expression defects (33). To test the requirement of the kinase module and the core Mediator for CSR, we treated CH12F3-2A cells by cortistatin A (CA), a potent pharmacological inhibitor of Cdk8 and its paralog Cdk19 (34). Unexpectedly, CA treatment (100 or 250 nM) did not show any inhibitory effect on CSR compared to dimethyl sulfoxide (DMSO) control ( Fig. 3B and fig. S2A). We confirmed the effectiveness of CA treatment (250 nM) by examining the expression of kinase module-regulated and CA-sensitive genes, namely, Egr1, Atf1, and Atf7 ( Fig. 3C and fig. S2B) (35). In addition, the depletion of Cdk8 by siRNA had no significant effect on CSR ( Fig. 3D and fig. S2C), despite Cdk8 mRNA being efficiently down-regulated by three independent siCdk8s ( Fig. 3E and  fig. S2C).
To further investigate kinase module-independent functions of Med12 in CSR, we modeled three Med12 mutations (L36R, Q43P, and G44S) that are associated with UL ( Fig. 3F) (36). These mutations disrupt Med12 interaction with cyclin C and Cdk8/Cdk19. Notably, each single mutation alone was sufficient to abolish the kinase module-dependent functions of Med12 (36). We confirmed the loss of Cdk8 interaction in these Med12 mutants by Co-IP (Fig. 3F). Furthermore, all three mutants fully restored CSR activity (Fig. 3G). These results are consistent with the insensitivity of CSR to CA treatment and Cdk8 depletion (Fig. 3, B and D) and further suggest kinase module-independent functions of Med12 in CSR (Fig. 3J).
Furthermore, to test the requirement of core Mediator in CSR, we knocked down Med13 and its paralog Med13like (Med13L), which is required for kinase module interaction with the core Mediator (Fig. 3A). Med13 and Med13L were depleted up to 70 to 80% by siMed13-1 and siMed13L-3, respectively. However, CSR was not significantly affected following Med13 or Med13L depletion (Fig. 3, H and I, and fig. S2, D and E). We observed a slight decrease in CSR by siMed13-2/siMed13-3 that we deemed as nonspecific, as it did not correlate with KD efficiency ( fig. S2D). Together, we conclude from these multiple lines of evidence that Med12 promotes CSR independently of its kinase module and the core Mediator (Fig. 3J).

Med12-p300 complex regulates CSR through 3′RR enhancer activation
Previous reports have largely focused on the kinase module-mediated functions of Med12, leaving the kinase module-or core Mediator-independent functions of Med12 largely unknown. A recent report suggests that Med12 regulates hematopoietic stem cell-specific super-enhancers in cooperation with the HAT p300 and independent of the Med12 kinase module (22). From this, we asked whether Med12 might analogously activate the IgH 3′RR.
To test this hypothesis, we first examined whether deposition of the hallmark enhancer marker, H3K27ac, at the IgH 3′RR super-enhancer was dependent on Med12 and p300. We find that depletion of either Med12 or p300 markedly reduces H3K27ac deposition across the enhancer clusters (hs3a, hs1.2, hs3b, hs4, hs5, hs6, and hs7) in 3′RR (Fig. 4, A to C, and fig. S3A). Because p300 is a key acetyltransferase that catalyzes H3K27 acetylation at enhancers, we tested whether p300 recruitment at the IgH 3′RR was dependent on Med12. Med12 depletion significantly reduced p300 localization at the 3′RR enhancer (Fig. 4D). In support of this finding, co-IP analysis confirms the interaction between Med12 and p300 (fig .  S3B). Furthermore, functional depletion of p300, either by siRNA or HAT catalytic inhibition by C646 inhibitor ( p300 In ), led to CSR impairment ( Fig. 4E and fig. S3, A and C) and decreased H3K27ac at the enhancer.
To confirm whether p300 loss recapitulates the Med12 loss, we investigated the three essential steps for CSR: (i) Switch GLT, (ii) DNA DSB formation, and (iii) S-S synapse formation. Unexpectedly, p300 depletion decreased S region DSBs as well as interactions between Sμ-Sα and Eμ-3′RR ( fig. S3, E to G), similar to the defects observed following Med12 depletion (Fig. 1, D and F). In addition, similar to Med12 KD (Fig. 1C), transcription of μGLT and αGLT were not perturbed following p300 depletion (fig .  S3H). However, p300 KD or its catalytic inhibition decreased DSB associated γH2AX formation in the S region ( Fig. 4F and fig. S3D). Given this observation, we examined H3K4me3 marks in the S region, as they are essential for AID-induced DNA DSBs (37-39). Depletion of Med12 or p300 resulted in a significant loss of H3K4me3 at the S region (Fig. 4, G and H). We observed a similar loss of H3K4me3 from both the Sμ and Sα regions following p300 inhibition ( fig. S3D). Co-IP experiments also showed that the Med12-p300 complex contains critical components involved in histone lysine 4 methylation, such as Ash2 and Wdr5 ( fig. S3B). Loss of either Ash2 or Wdr5 also significantly reduced S region H3K4me3 and γH2AX formation, resulting in impaired AIDinduced DSB and CSR (38). In summary, 3′RR activation through the coordinated activity of Med12 and p300 appears to be crucial for both S region chromatin remodeling and long-range S-S synapse formation. To further investigate this hypothesis, we tested whether transcription of noncoding eRNAs, another hallmark of active enhancers, was also dependent on Med12 and/or p300. We find that eRNA transcription from hs1.2 and hs4 is decreased by Med12 depletion and elevated by Med12 overexpression in Med12 KD cells (Fig. 4I). Similarly, p300 depletion or HAT activity inhibition reduces 3′RR eRNA expression (Fig. 4, J and K), suggesting that 3′RR enhancer activation is dependent on Med12 and/or p300. We conclude that Med12 plays a crucial role in recruiting p300 to the 3′RR for enhancer activation and epigenomic modulation in the S region, both of which are essential for efficient CSR (Fig. 4L). KD or p300 In on indicated transcripts relative to control. The data were normalized with endogenous β2m abundance. (L) Schematic showing the role of Med12-dependent differential epigenomic regulation at S and 3′RR regions. We propose that Med12 activates the 3′RR enhancer through p300, which marks H3 histone acetylation (black boll). The enhancer RNA (eRNA) produced from the activated enhancers regulates the AID-induced DNA break formation by regulating the histone marks γH2AX (red boll) and H3K4me3 ( purple boll) at S regions. The result summarizes the means ± SD of three independents experiments, and the statistical significance was determined by two-tailed Student's t test (P > 0.05).

Rescue of Med12 deficiency by CRISPR-dCas9-mediated 3′RR activation
We hypothesized that the loss of 3′RR activation is the underlying cause of CSR impairment following Med12 deficiency. From this, we tested whether CSR can be restored by enforced enhancer activation using a CRISPR-dead Cas9 (dCas9)-based enhancer epigenetic remodeling system (40). We used a hs1.2 and/or hs4 targeting dCas9 coupled to the core HAT domain of p300 (dCas9-p300 C ) that can catalyze H3K27 acetylation at the 3′RR enhancer ( Fig. 5A) (41). We selected the two hypersensitive sites, hs1.2 and hs4, for targeting in CH12F3-2A, as their deletion significantly impairs CSR in mouse models (42,43). Transfection of dCas9-p300 C , together with hs-specific small guide RNA (sgRNA) in Med12 KD cells, restored enhancer activity as measured by complete recovery of H3K27ac deposition and a concomitant increase in eRNA transcription (Fig. 5, B and C). Targeting dCas9-p300 C to one of the hypersensitive sites is sufficient to compensate for epigenetic deficits at the other site, possibly due to their palindromic nature and sequence similarity (44). As expected, cotransfection of dCas9-p300 C and hs-sgRNA rescued the CSR defect in Med12 KD cells nearly as efficiently as by rescue with the WT R construct (Fig. 5D; compare first two blue bars versus last two blue bars). Neither sgRNA (hs1.2/hs4) nor dCas9-p300 C transfection alone affected the CSR compensation in Med12 KD cells (Fig. 5D, gray bars).
Similarly, cotransfection of dCas9-p300 C and hs-sgRNA also restored S region DSB formation in Med12 KD cells as detected by our LM-PCR assay (Fig. 5E; compare b versus f and g). DSB signals derived from Med12 KD cells transfected with hs1.2 and hs4 sgRNA or dCas9-p300 C were considered as background (Fig. 5E,  d and e). Notably, enforced activation of 3′RR in Med12 KD cells also restored S region H3K4me3 and γH2AX marks (Fig. 5, F and G). Transfection with dCas9-p300 C and hs1.2 or hs4 sgRNA also largely restored long-range interactions between Sμ-Sα/Eμ-Sα in Med12 KD cells (Fig. 5H).
Because AID is essential to S region DNA DSB and S-S synapse formation, we also examined how enhancer reactivation affects AID recruitment to the IgH locus, a process that has previously been reported to be 3′RR dependent (10,13). In Med12 KD cells, AID was reduced at S regions and was restored to control levels upon cotransfection with dCas9-p300 C and enhancer-targeting sgRNAs (Fig. 5I). AID has also been reported to target 3′RR and was found to be distributed across the 3′RR super-enhancer region (45). Furthermore, AID-induced DNA breaks at 3′RR are responsible for locus suicide recombination (LSR), a process that removes a large sequence region containing Sμ and 3′RR and leads to impaired cell survival. LSR is considered an intrinsic mechanism to regulate B cell homeostasis and for selection of antigen-specific B cells. We observed that Med12 depletion also reduces AID recruitment at 3′RR (fig. S4A). However, it remains to be determined whether Med12 and/or 3′RR eRNA also regulate LSR (45).
Together, our findings suggest that 3′RR activation by CRISPR-dCas9-p300 C compensates for CSR defects following Med12 deficiency, likely through restoring multiple epigenetic processes in the S region, including H3K4me3 formation, DNA DSB induction, and S-S synapse formation. In summary, Med12 is an indispensable chromatin remodeling factor for IgH 3′RR activation and associated CSR.

Mechanism of Med12-dependent IgH 3′RR eRNA regulation
Here, we provide evidence that Med12-dependent 3′RR eRNA transcription is critical for CSR regulation. However, several outstanding questions remain, including how Med12 is recruited to the IgH enhancer and how the enhancer activation functions of Med12 are regulated. To address these questions, we used an ER-bound enhancer (ERE) element eRNA transcription system. In this system, eRNA transcript expression is strongly and rapidly induced following estrogen exposure (46). Recent evidence suggests that Jmjd6, a multifunctional enzyme, regulates ERE-derived eRNA transcription by recruiting Med12 and the Carm1 complex (47). Jmjd6 may also be necessary for Med12 interaction with Carm1, which, in turn, methylates Med12 at multiple arginine sites to facilitate chromatin binding.
To test the involvement of the Jmjd6/Carm1 pathway in 3′RR regulation through Med12, we first confirmed the presence of Jmjd6/Carm1 at the IgH 3′RR and that this occupancy can be depleted by using siRNA against Jmjd6 (Fig. 6A). We find by chromatin IP (ChIP) analysis that Jmjd6/Carm1 occupies the 3′RR and that this occupancy is dependent on Med12 (Fig. 6B). This finding prompted us to examine whether Jmjd6/Carm1 depletion also affects CSR and 3′RR eRNA transcription. We find that depletion of Jmjd6/Carm1 reduces CSR, and eRNA transcription from both hs1.2 and hs4 and is correlated with KD efficiencies (Fig. 6, C and  D). Furthermore, ChIP analysis revealed that reduced eRNA transcription in Jmjd6 KD cells was likely due to the loss of H3K27ac mark but not loss of Med12 at the 3′RR, as Jmjd6 depletion specifically reduced H3K27ac and p300 protein enrichment (Fig. 6, E and F). We confirmed the specificity of siJmjd6 by using an siRNA-resistant transcript (WT-jmjd6 R ) that successfully restored the siJmjd6-mediated CSR inhibition ( fig. S4D). As expected, expression of WT-Jmjd6 R but not the catalytically defective mutant (H187A-Jmjd6 R ) restored CSR in Jmjd6 KD cells ( fig. S4D), suggesting that the demethylase activity of Jmjd6 may remove repressive histone marks to preserve H3K27ac at the 3′RR. To further confirm that the observed siJmjd6-mediated CSR impairment is due to the loss of H3K27ac and eRNA at the 3′RR, we activated the enhancer by cotransfecting dCas9-p300 C and hs4-sgRNA. This activation fully restored the CSR defect in Jmjd6 KD cells (Fig. 6G), further emphasizing the importance of 3′RR activation and eRNA production for CSR.
Next, to evaluate the importance of Med12 arginine methylation in CSR and 3′RR eRNA regulation, we generated Med12 mutants (R1854K, R1871K, and R1899K) that are defective in arginine methylation by Jmjd6/Carm1 (47). CSR complementation assays showed that all three methylation mutants were defective in CSR at variable levels of deficiency (Fig. 6H). These CSR defects are comparable to defects previously reported in the Med12 ΔPQL mutant (Fig. 2, A  and B), the Med12 domain that contains critical and additional arginine methylation sites. Notably, addition of the ΔPQL mutant was also unable to restore 3′RR eRNA transcription from both the hs1.2 and hs4 enhancers in Med12 KD cells (Fig. 6I). Together, we conclude that the Jmjd6/Carm1 complex is an important posttranslational regulator of Med12, which cooperates with p300 to regulate 3′RR activation and eRNA transcription and efficient CSR (Fig. 6J).

Depletion of 3′RR eRNAs perturbs enhancer function and impairs CSR
eRNAs are short transcripts that are transcribed unidirectionally or bidirectionally from enhancers (20). eRNAs exert a plethora of functions either in cis or trans, including regulating transcription through recruiting transcription and/or chromatin remodeling factors, regulating long-range interaction between enhancer and promoter sequences, and regulating histone modifications (48). At some enhancers, H3K27ac deposition and Mediator complex recruitment are dependent on eRNA production (48,49). From this, we attempted to clarify the role of 3′RR eRNAs in histone modification at the 3′RR and S region, as well as the role of 3′RR eRNAs in S region DSB, S-S synapse formation, DNA repair, and CSR.
To specifically deplete 3′RR eRNAs, we designed locked nucleic acid-modified antisense oligos (ASO1 and ASO2) targeting the hs4 enhancer. We chose hs4 because of its basal eRNA expression in CH12F3-2A cells, which is several folds higher than hs1.2 basal  S4B). Transfection of hs4-specific ASOs but not an unrelated control ASO strongly inhibited IgA switching in CH12F3-2A cells (Fig. 7A). Depletion of hs4-specific eRNAs by ASO1 and ASO2 was also confirmed by qRT-PCR (Fig. 7B). Neither μGLT nor αGLT transcript expression was affected by ASO1/ASO2 treatment (Fig. 7B). A similar level of CSR impairment by ASOs was also observed in the AIDER expressing CH12-F3-2A cell line, where CSR is induced through activation of an ER-fused AID by 4-hydroxytamoxifen (OHT) (tamoxifen) treatment ( fig. S4C). Next, we examined whether CSR defects are correlated with S region DSB by LM-PCR and ChIP assays. As expected, transfection of ASOs into CH12F3-2A cells markedly reduced S region DSB signals, as compared to control ASOs (Fig. 7C). Using the most potent ASO, we evaluated DNA breaks and damage response-associated histone marks at the S regions. We observed a severe defect in H3K4me3 deposition and γH2AX formation in ASO1-transfected Med12 recruits p300 at 3′RR enhancers, which, in turn, catalyzes the H3K27ac histone acetylation. Med12-p300 complex initiates the enhancer activation, which transcribed into the eRNA. The eRNA produced from the 3′RR and recruits Med12, H3K4me3 methyltransferase, and DNA break complex at S regions. In the absence of Med12, p300 does not recruit to 3′RR, resulting in inactivation of enhancers and perturbed DNA break and S-S synapse formation. The result summarizes the means ± SD of three independents experiments, and the statistical significance was determined by two-tailed Student's t test (P > 0.05).  (Fig. 7D), which was consistent with S region DSB impairment (Fig. 7C). AID association with the IgH locus decreased following ASO1 treatment (Fig. 7D) despite AID levels remaining unchanged (Fig. 7C). Notably, in addition to impaired AID-induced S region DNA breaks, long-range Sμ and Sα interactions were also disrupted (but not Eμ-3′RR) following ASO1 transfection (Fig. 7E). It is notable that 3′RR-eRNA depletion following ASO treatment also impaired the two key steps of CSR: S region DSBs and S-S synapse formation consistent with our observations following Med12 depletion. Together, our data suggest that Med12 functions in CSR are dependent on eRNA expression from the 3′RR. We find that the Med12 mutant with multiple XLID mutations (R521H/R621Q/I771T), which we named "HQT," shows significant CSR impairment and 3′RR eRNA transcription defects (Fig 7, F and  G). Such a function has never been reported for any XLID mutations; we also find loss of the Med12 PQL domain impairs CSR and 3′RR eRNA transcription (Figs. 2B and 6I). Our findings that the LS and PQL domains of Med12 regulate CSR imply that both AID-driven DNA DSBs and S-S synapse formation require 3′RR activation and more specifically eRNA transcription.
We noticed that Med12 has intrinsically disordered regions (IDRs) across the LS and PQL domains ( fig. S6A). A comparison of Predictor of Natural Disordered Regions (PONDR) analysis revealed that the feature is very similar to Med1 and Brd4 ( fig. S6A). We also confirmed that Med12 is an IDR-containing protein by precipitating IDR-specific chemical ( fig. S6C), biotinylated isoxazole or b-Isox, which also precipitated other known IDR-containing proteins, including Med1 and Brd4 (50,51). Because of the presence of IDRs, Med1 and Brd4 can undergo nuclear phase separation to form condensate at the enhancers (50,51). To investigate that this is the case for Med12, we similarly used the chemical 1,6-hexanediol (1,6-HD) to disrupt the Med12-eRNA complex, perturbing the phase separation. There was a clear dose-dependent inhibition of CSR and concomitant decrease of eRNA synthesis at the IgH 3′RR by the 1,6-HD treatment ( fig. S6B).
We propose that IgH 3′RR-derived eRNAs drive epigenomic regulation at the IgH 3′RR enhancer and the S-region, stabilizing S-S proximity and promoting AID-induced DNA DSBs and CSR through recombination-associated condensate formation, which awaits further investigation.

Med12 and AID have functional homology for DNA DSBs and S-S synapse formation during CSR
AID is an indispensable enzyme for generating the DNA DSBs and S region synapses that are required for oriented deletional recombination during CSR (6,7,52). How AID regulates the mechanistically distinct processes of S region DNA DSBs and S-S synapse formation remains poorly understood (53). While numerous AID-interacting and noninteracting CSR regulatory factors have been identified, these factors appear to play exclusive roles in DNA break, repair, or synapse formation (4,54,55). Here, we show that Med12 is a previously unknown CSR cofactor that not only promotes AID-induced DNA DSBs and synapse formation but also supports DNA repair via NHEJ (Fig. 1, D to F, and fig.  S1E). We find that Med12 shares with AID many of the key functional aspects that are essential for efficient CSR and, eventually, Ig gene diversity. As CSR is highly sensitive to Med12 protein levels, we consider Med12 levels to be a key rate-limiting factor for DNA DSBs and S region synapse formation. Our analysis of multiple Med12 mutations (table S1) shows that the LS and PQL domains are critical for efficient CSR (Fig. 2F) and likely have distinct yet overlapping functions. Loss of the LS, but not PQL domain, leads to severe impairment of DNA DSBs and DDR signals such as γH2AX formation in the S region (Figs. 1, D and E, and 2C). However, deletion of either domain leads to impaired S-S synapse formation and loss of AID occupancy at the IgH locus (Figs. 2D and 5I). Our cross-complementation and studies using Med12 mutants also suggests that, while the LS domain is crucial for AID-induced DNA DSBs, both the LS and PQL domains are necessary for S-S and Eμ-3′RR interaction (Figs. 1F and 2D). The LS and PQL domains are likely involved in Med12 dimerization or multimerization (Fig. 2E) that associates with the eRNA-protein complex to form local enhanceosome (50) or condensate ( fig. S6B).

Med12-dependent IgH 3′RR super-enhancer activation is central to CSR
Consistent with Med12's function in IgH locus DNA DSBs and long-range chromatin looping, we find Med12 enrichment at the Eμ, Sμ, Sα, and 3′RR super-enhancer regions ( fig. S5, A to C) (56). However, Mediator is a 30-subunit megadalton complex with four submodules, including the Med12-containing kinase module that reversibly interacts with the core Mediator for transcriptional regulation (20). At the IgH locus, Med12 functions in CSR appear independent of its kinase function, as CSR was refractory to CDK8 depletion or catalytic inhibition of the CDK8 kinase. These findings are also consistent with competent CSR observed in Med12 mutants that are defective in CDK8 activation (Fig. 3, F and  G). Similarly, depletion of Med13/Med13L, the essential bridging component between core Mediator and the kinase module, does not affect CSR (Fig. 3H). While other associations may still exist, these kinase-independent functions of Med12 are reminiscent of Med12 functions in human pluripotent stem cells (HPSC) homeostasis (22), where Med12 helps regulate cell lineage-specific superenhancers in a kinase-independent manner.
H3K27ac and H3K4me1 on enhancer chromatin distinguish transcriptionally active enhancers from inactive and paused enhancers (57). Priming of enhancer activation occurs through the binding of pioneering TFs and subsequent loading of other TFs, coactivators, and RNAPII to generate eRNA from super-enhancers (58). Consistent with previous reports, our work suggests that Med12 maintains IgH 3′RR super-enhancer activation through p300, as Med12 depletion results in p300 recruitment defects, impaired H3K27ac deposition, and 3′RR eRNA transcription (Fig. 4, C, D, I, and J). Here, we used multiple lines of evidence to demonstrate the importance of IgH enhancer activation for CSR. These lines of evidence included (i) a Med12 deficiency complementation for CSR by CRISPR-dCas9 enhancer activation system that restored H3K27ac signature and eRNA synthesis at 3′RR (Fig. 5, B and C), (ii) recapitulating 3′RR inactivation and CSR defects observed in Med12 deficiency by p300 depletion or inhibition (Fig. 4, C, J, and K), and (iii) degradation of 3′RR eRNAs by ASO targeting shows strong CSR impairment, as well as impaired S region DNA DSBs, reduced long-range interactions, and reduced AID recruitment to the IgH locus (Fig. 7, C to E). We obtained similar results when eRNA processing was interrupted by depleting the catalytic subunit of the integrator complex (IntS11 and IntS13) ( fig.   Haque et al., Sci. Adv. 8, eadd1466 (2022) 25 November 2022 12 of 18 S4E), which regulates the length and production of eRNAs (59). Consistent with these findings, we also find enrichment of IntS11 and IntS13 at the 3′RR enhancer after stimulation with CIT for CSR ( fig. S4F). The requirement of the 3′RR super-enhancer in CSR has been well documented by numerous elegant studies in mice models and ex vivo system (9,13). However, there remains minimal information regarding the mechanisms of 3′RR activation and how this activation affects AID-induced CSR events. Recently, Zymnd8 that recognizes various histone modifications was shown to reduce RNAPII loading at the IgH super-enhancer and reduce enhancer transcription (60). Conversely, RNAPII elongation factor Spt5 may regulate 3′RR transcription by regulating RNAPII pause release (61). Transcription elongation factor (SPT5) deficiency does not disrupt Med12 or H3K27ac occupancy at the 3′RR, and a CRISPR-dCas9-VPR transcriptional activation system can rescue enhancer transcription defects but not CSR. This is likely due to Spt5 being required for AID expression and recruitment (61,62). However, we find that complementation of Med12 deficiency strictly requires an enhancer-activating CRISPR-dCas9-p300 C system, which restores H3K27ac marks at the 3′RR and restores eRNA transcription and CSR (Fig. 5, C and D). In conclusion, our results are consistent with Spt5 and Zymnd8 functioning downstream of enhancer activation by Med12.

Med12 and 3′RR eRNA-dependent epigenomic and conformational regulation
Promoters of actively transcribed gene loci are generally enriched with H3K4me3, a signature mark of accessible chromatin (63). However, at the IgH locus, actively transcribed I promoters and downstream S recombination regions are highly enriched with H3K4me3 (64-66). Down-regulation of IgH locus-specific H3K4me3 is associated with various CSR-associated defects, including impaired AID-induced S region DNA DSBs and impaired Ig isotype-specific transcription in primary B cells (37,38,67). Our work here is consistent with other studies, suggesting that the combinatorial histone code, including H3K4me3, facilitates DNA DSB complex formation at the S region (37,38,68). One of our notable findings is that Med12 deficiency causes strong down-modulation of H3K4me3 and AID-induced S region DNA DSBs. Because Med12 is in a complex with H3K4me3 writing machinery, loss of Med12 in S regions may perturb H3K4me3 complex activity, leading to impaired AID-induced DNA DSBs. Within this process, we suspect that 3′RR activation plays a critical role, as p300 depletion (or 3′RR inactivation) leads H3K4me3-impaired deposition and DNA DSB formation at S regions (Fig. 4, H and  F). This hypothesis is consistent with our finding that 3′RR activation by CRISPR-dCas9-p300 system can fully restore defects caused by Med12 depletion.
Depletion of 3′RR eRNAs, the activation markers of the IgH super-enhancer, phenocopied the DNA DSB and S-S synapse formation defects observed in Med12, p300, and AID deficiency (Fig. 7, C to E). This result suggests a direct and unique role of 3′RR eRNAs in CSR regulation. We have shown that 3′RR eRNAs can bind Med12, Wdr5, Rad21, and AID ( fig. S5D); and their depletion impairs recruitment of Med12, H3K4me3, and AID occupancy at S region, leading to DNA DSB and S-S synapse formation defects ( Fig. 7D and fig. S5C), Notably, 3′RR eRNA depletion did not affect Med12 or H3K27ac occupancy at the 3′RR ( fig. S5B), suggesting that these eRNAs predominantly contribute to CSR in a trans-manner, possibly functioning in the S regions. Consistent with this hypothesis, S region DNA DSBs and long-range Sμ-Sα but not Eμ-3′RR interactions are affected by 3′RR eRNA depletion. However, Med12 depletion leads to disruption of both chromatin loops, Sμ-Sα and Eμ-3′RR interactions (Fig. 1F), suggesting that Med12 is an essential constituent of both Sμ-Sα and Eμ-3′RR chromatin conformations. While basal levels of Med12 and 3′RR eRNAs are likely sufficient to confer Eμ-3′RR chromatin architecture, CSR induction may stabilize it further through Med12 enrichment and increased eRNA transcription. eRNA transcripts also may help Med12, AID, and other essential components localize to recombining S regions for S-S synapse formation.

Involvement of 3′RR eRNAs in CSR-specific condensate formation
Recent studies have shown super-enhancers exist as phase-separated condensates, defined as a three-dimensional reservoir holding large-scale regulatory factors and RNAs (50,51). Associated eRNAs have been implicated in stimulus-dependent (e.g., E2/epidermal growth factor) (59,69) dynamic phase separation during enhancer-promoter looping where they interact with many factors present in super-enhancers, including Med1, cohesins, YY1, p300/CBP, and BRD4 (48,70). Depletion of eRNAs from associated enhancers affected either the recruitment or function of the chromatin conformation regulatory factor, leading to disruption of enhancer-promoter chromatin looping and/or enhanceosome formation (50,51,70). Our work also shows that depletion of 3′RR eRNA significantly affects recruitment of Med12, AID, and possibly still unknown components to the S region. PONDR analysis ( fig. S6A) suggests that Med12 has IDRs, as observed in Med1 and Brd4, both of which promote enhancer condensate formation. We also confirm that Med12, like Med1 and Brd4, can be precipitated by IDR-specific chemical b-Isox ( fig. S6C) (71). In addition, eRNA transcription and CSR are both sensitive to 1,6-HD treatment, a known method for perturbing eRNA-dependent enhancer ribonucleoprotein complex formation and chromatin architecture ( fig. S6B) (50).
From this, we suspect that 3′RR-derived eRNAs can act as a matrix or recruiting medium so DNA break-recombination complexes can assemble locally. While some of these defects have been previously observed in a 3′RR mouse model, the underlying mechanisms remain unclear. Our work here provides a plausible explanation for how enhancer activation and transcription can coordinate two seemingly dissimilar processes simultaneously, AIDinduced DNA DSBs and S-S synapse formation.

Implications for Med12 and dysregulated CSR in XLID syndrome
Here, we have shown that mutations located near the N terminus of Med12 and those affecting Med12 kinase module (36) functions do not affect CSR. Conversely, several LS domain-and PQL domainassociated Med12 mutations show significant impairments in CSR (table S1). Both atypical and FG-type XLID mutations showed a marked impairment of CSR with impaired 3′RR activation/transcription (Fig. 7, F and G). It remains unknown whether patients with these XLID mutations (72,73)  of eRNAs (Figs. 6I and 7G), the markers of active 3′RR super-enhancers. Although Med12 mutations have been linked to various cancer types and congenital disorders with intellectual disability, the underlying functional defects and mechanisms of these disorders remains poorly understood (table S1) (25). Defined and coordinated regulation of super-enhancers is essential for cell lineage and cell identity (22,74,75). From this, it is conceivable that Med12 defects lead to dysregulation of normal or cell lineage-specific super-enhancer functions, which ultimately give rise to neurologic disorders and/or tumors (74,76). Furthermore, many neurodevelopmental and/or intellectually disability genes are linked to DNA damage repair and the NHEJ pathway (77,78). Because NHEJ pathway is essential for both V(D)J and CSR, DNA repair defects are often a common cause of both neuronal and B cell defects. We show that Med12 deficiency may impair NHEJ; however, additional work will be needed to determine the mechanism.

Methylated Med12 initiates enhancer activation
It remains unclear how Med12 coordinates these molecular activities. It is possible that Med12's functions in CSR are regulated by interacting with other ncRNAs, specifically eRNAs and long noncoding RNAs (unpublished) and/or through arginine C-terminal methylation to regulate protein-protein or protein-RNA interactions. Carm1 methylates multiple arginine residues at the C terminus of the Med12 PQL domain. Carm1-dependent Med12 methylation sensitizes breast cancer cells to chemotherapy, and mutations at these methylation sites impair Med12 binding at the p21 locus (27). Recent work has shown Jmjd6 regulates Med12 methylation through Carm1, which promotes Med12 binding to estrogen receptors alpha (ERa)-bound active enhancers and regulates Med12 function (47). Our results partially support this model, as we find that depletion of the demethylation/methylation complex (Jmjd6/ Carm1) also reduces eRNA transcription and CSR (Fig. 6, C and D). We find that Med12 is required for recruiting the Jmjd6/ Carm1 complex to the IgH 3′RR locus, while Jmjd6/Carm1 is dispensable for Med12 recruitment (Fig. 6F). Furthermore, depletion of the demethylase Jmjd6 results in failures of enhancer activation (Fig. 6E). From this, we suspect that the methylation status of Med12 is crucial for enhancer activation ( possibly through methylation-dependent recruitment of other coactivators/histone modifiers such as p300) to the IgH 3′RR locus, while methylation status does not affect Med12 chromatin binding. This hypothesis is strongly supported by evidence that Carm1 methylates Med12 at R1899, which is then recognized by coactivator TDRD3, leading to further interactions with activating ncRNAs for estrogen-regulated gene transcription (26). Crucially, we find that R1899 mutant Med12 also has diminished CSR activity (Fig. 2F). We did not find any significant difference in eRNA transcription in individual Med12 methylation defective mutants, whereas deletion of the entire PQL domain of Med12 leads to defective eRNA regulation (Fig. 6I), suggesting that combinatorial methylation is likely required for enhancer activation, a conclusion that is consistent with a previously published report (47). The mouse Jmjd6 (NM_001363363) cDNA was obtained as described above and cloned into the Hind III/Bam HI (Takara) sites of the pCMV10 vector. The 3xFlag epitope was tagged at N-terminal. To generate siJmjd6-resistant Jmjd6 transcripts (Jmjd6-WT R ), the siJmjd6 targeting sequence is modified by multiple mutageneses without altering the amino acid code. The primers sequence has been provided in the table S2.

Western blotting
For immunoblotting, total cell lysate was prepared by lysing 2 × 10 6 cells by the RiboCluster Profiler Kit (MBL, RN1001) supplemented with EDTA-free protease inhibitor cocktail (Roche) and ribonuclease (RNase) inhibitor (Sigma-Aldrich). After lysis for 5 min at 4°C, cells were centrifuged (135,000g) for 5 min, and supernatants were collected in separate tube. The obtained clear lysate was mixed with

Immunoprecipitation
For each IP, Protein G Dynabeads (Invitrogen, 1003D) were preincubated with antibody of interest (5 μg) with rotation at room temperature for 1 hour. Beads were collected and washed 2× with wash buffer provided in a RiboCluster Profiler Kit (MBL, RN1001) before overnight incubation with lysate. After the incubation, beads were washed 3×, and equal ratio of 2× SDS and wash buffer were added before gel electrophoresis. For V5 IP, agarose anti-V5 tag antibody (ab1229) was used as per the manufacturer's instructions and processed as described above.

ChIP-qPCR
The ChIP assay was performed using the ChIP-IT Express Kit (Active Motif, 53008) according to the manufacturer's instructions.
In brief, 5 × 10 6 cells were fixed in the presence of 1% formaldehyde for 5 min at room temperature. The reaction was stopped by the addition of 0.125 M glycine. A soluble chromatin fraction containing fragmented DNA of 500 to 2000 base pairs was obtained after cell lysis and sonication. ChIP was performed by incubating the cleared lysate with 3 μg of antibodies. The immunoprecipitated DNA was analyzed by real-time PCR, and the data were normalized first to the amount of input and then to the maximum value in each dataset, as described previously (38). The ChIP antibodies and primers used are listed in table S2.

RNA IP
For RNA IP (RIP) assay, 1 × 10 7 cells were collected, washed with cold phosphate-buffered saline, and lysed by lysis buffer (RiboCluster Profiler Kit, MBL, RN1001) supplemented with dithiothreitol, RNase inhibitor (Sigma-Aldrich), and EDTA-free protease inhibitor cocktail (Roche) as described by the manufacturer. The subsequential RIP was performed using the Magna RIP kit (Merck Millipore, 17-700) according to the manufacturer's instruction with slight modifications. After overnight RIP, the TRIzol (Ambion) was directly added to the washed magnetic beads containing RNAs, and the total RNA was extracted using the standard RNA isolation protocol. The purity and concentration of RNA were analyzed by NanoDrop or Agilent Bioanalyzer 2100.

RNA isolation, RT, and RT-qPCR
RNA was isolated from control or treated cells using the TRIzol (Ambion), followed by DNase I treatment (Sigma-Aldrich, AMPD1). One microgram of purified RNA was used as template for cDNA synthesis using SuperScript IV (Invitrogen, 18090050) with random primers (Invitrogen, N8080127). Real-time PCR (Applied Biosystems, 7900HT Fast Real-Time PCR System) was performed using SYBR Green Master Mix (Applied Biosystems) and mRNA-specific primers listed in table S2. The 2 −∆∆Ct method was used to quantify the data using either Gapdh or β2 microglobulin (β2m) housekeeping transcript for normalization.

LM-PCR and 3C assay
For double-stranded DNA break estimation, CIT (+)-stimulated 1 × 10 6 cells per sample were collected as described above, fixed in low-melt agarose plugs, and processed for linker ligation as described previously (30). Briefly, linker ligation reaction was performed overnight at 16°C, and to inactivate the reaction, samples were heated at 70°C for 10 min. Threefold serial dilutions of linker ligated DNA were amplified by KOD FX Neo polymerase (Toyobo) using an Sμ-specific primer (forward) and a linker-specific primer (reverse). To confirm the amplification of Sμ-specific DSBs, Southern blot analysis of the PCR products was performed using a DIG-labeled Sμ probe. Similarly, PCR of the GAPDH locus from each sample served as a normalization control. The 3C assay was performed as described previously (6,54). Briefly, 7 × 10 6 cells were collected, washed, and cross-linked for 5 min at room temperature with 1% formaldehyde. After crosslinking, the cells were subjected to nuclear lysis. The cross-linked chromatin was digested overnight with Hind III and later ligated with T4 polymerase DNA ligase (Takara). The ligated chromatin was treated with proteinase K and reverse cross-linked; furthermore, the DNA was purified by phenol/chloroform extraction protocol. PCRs were performed using the primers described in table S2.

IgH/c-Myc translocation and NHEJ assay
For translocation assay, genomic DNA has been isolated from 48 hours of CIT-stimulated samples and was PCR amplified at IgH/c-Myc translocation junctions using the Expand Long Template PCR system as described previously (31). The PCR products were separated by electrophoresis on ethidium bromide containing 1% agarose gels and subjected to Southern blotting with a Myc-specific probe.
The NHEJ assay was performed as described previously (32). In brief, The I-SceI-expressing plasmid ( pCBASce) alone or with siMed12 (designed against human Med12) or control was cotransfected into NHEJ reporter cell lines using Lipofectamine 2000 (Invitrogen). Transfected cells were harvested after 48 hours for FACS analysis. The NHEJ reporter cell line H1299dA3-1 was a gift from T. Kohno at the National Cancer Center Research Institute, Tokyo. The primers and siRNAs sequence were shown in table S2.

Inhibitors
CA was a gift from M. D. Shair (Harvard University) and D. J. Taatjes (University of Colorado Boulder). The dissolved CA in DMSO was provided as a stock concentration of 1 mM and was stored at −80°C for further use. The final concentrations of 100 and 250 nM were used in the experiments. The DMSO concentrations of 0.0001 and 0.00025% (without CA) were used as a vehicle control.
The P300 HAT inhibitor, C646 (Sigma-Aldrich, 328968-36-1), was dissolved in DMSO, and the 5 μM concentration was used for related experiments. The lists of antibodies, primers, and stealth siRNAs used in this study are shown in table S2.

CRISPR and sgRNAs cloning CRISPRa
To activate the 3′RR IgH enhancer, we exploited the CRISPRa technology (40). The sgRNA (hs1.2 and hs4) sequence was obtained from previously published report (61). Briefly, oligonucleotides were annealed in the following reaction: 10 μM guide sequence oligo, 10 μM reverse complement oligo, and 50 mM NaCl in tris-EDTA buffer with the cycling parameters of 95°C for 2 min and then ramp down to 25°C at 5°C/min. The annealed oligos were cloned into the sgRNA vector ( pLH-spsgRNA2, Addgene, 64114) Haque  using a Golden Gate Assembly strategy including 100 ng of circular sgRNA vector plasmid, 0.2 μM annealed oligos, 20 U of Bbs I restriction enzyme, 750 U of T7 DNA ligase (Enzymatics, L6020L), and 1× T7 ligase buffer with the cycling parameters of 37°C for 5 min, followed by 60°C for 5 min. Insertion of sgRNA was validated by Sanger sequencing (Genetic Analyzer, 3130xl). The pcDNA-dCas9-p300 C was purchased from Addgene (no. 61357). Briefly, 500 ng of dCas9-p300 C expression vector and 500 ng of individual gRNA expression vectors were transfected in Med12 KD cells, and cells were incubated for 48 hours. After the incubation, the cells were CIT (+)-stimulated for another 48 hours before collecting the cells used for subsequent analysis.

CRISPRi
To knockdown the endogenous Integrator complex components (IntS11 and IntS13), sgRNA sequences (two sets for each) were designed from (http://crispor.tefor.net/). The obtained sgRNA oligonucleotide were annealed as described above and cloned in pSPgRNA purchased from Addgene (no. 47108) using the Bbs I cloning site. The vector dCas9-KRAB-MeCP2 was purchased from Addgene (no. 11082). Briefly, 500 ng of dCas9 expression vector and 500 ng of equimolar pooled sets of gRNAs were transfected, and cells were incubated for 24 hours. After the incubation, the cells were CIT (+) stimulated for another 24 hours before collecting the cells used for subsequent analysis.
b-Isox-mediated precipitation b-Isox-mediated protein precipitation was performed as described previously (79). The b-Isox was purchased (Sigma-Aldrich, T51161), dissolved in DMSO, and added to the cell lysates at 100 or 250 μM final concentrations. The reaction solutions were incubated at 4°C for 1 hour and then centrifuged at 14,000 rpm for 15 min. The pellets were washed twice with the wash buffer and resuspended in 2× SDS sample loading buffer. After SDS-PAGE, protein was detected by Western blotting using indicated antibodies. The antibodies used in this study are listed in table S2.

Statistical analysis
Error bars represent SDs from either independent experiments or independent samples. All statistical analyses were performed using GraphPad Prism, and the information about statistical methods is specified in figure legends. The numbers of independent experiments or biological replicate samples and P values [not significant (n.s.), *P < 0.05] are provided in individual figures. P < 0.05 was considered statistically significant.

Supplementary Materials
This PDF file includes: Supplementary Text Figs. S1 to S6 Table S1 References Other Supplementary Material for this manuscript includes the following: Table S2 View/request a protocol for this paper from Bio-protocol.