MKL1/2 and ELK4 co-regulate distinct serum response factor (SRF) transcription programs in macrophages
© Xie; licensee BioMed Central Ltd. 2014
Received: 10 January 2014
Accepted: 14 April 2014
Published: 23 April 2014
Serum response factor (SRF) is a widely expressed transcription factor involved in multiple regulatory programs. It is believed that SRF can toggle between disparate programs of gene expression through association with different cofactors. However, the direct evidence as to how these factors function on a genome-wide level is still lacking.
In the present study, I explored the functions of SRF and its representative cofactors, megakaryoblastic leukemia 1/2 (MKL1/2) and ETS-domain protein 4 (ELK4), during fungal infection challenge in macrophages. The knockdown study, combined with gene expression array analysis, revealed that MKL1/2 regulated SRF-dependent genes were related to actin cytoskeleton organization, while ELK4 regulated SRF-dependent genes were related to external stimulus responses. Subsequent chromatin immunoprecipitation coupled with massively parallel sequencing (ChIP-seq) suggested that many of these regulations were mediated directly in cis.
I conclude that SRF utilizes MKL1/2 to fulfill steady state cellular functions, including cytoskeletal organization, and utilizes ELK4 to facilitate acute responses to external infection. Together, these findings indicate that SRF, along with its two cofactors, are important players in both cellular homeostasis and stress responses in macrophages.
Macrophages are an important subset of innate immune cells implicated in host defense against bacterial and viral infections. Three of their major functions include phagocytosis and degradation of foreign pathogens, clearance of apoptotic or necrotic host cells, and rapid generation of effector cytokines that orchestrate immune responses. These different functions of macrophages are likely regulated by distinct transcription programs.
Serum response factor (SRF) is a member of the MADS (Mcm1, Agamous, Deficiens, SRF) transcription factor family  and is abundantly expressed in a variety of cell types. Deletion of Srf is embryonic lethal . Conditional deletion of Srf revealed its essential functions in many tissues, including skeletal, cardiac and smooth muscle cells [3, 4], neurons , and thymocytes [6, 7]. At the cellular level, these phenotypes can be attributed to impaired expression of different sets of SRF target genes. SRF-regulated immediate early genes (IEGs), such as c-fos, early growth response 1 (Egr1) and junB, are important for cell growth and proliferation [8–10], while SRF-regulated troponin, vinculin (Vcl), and SM22α participate in muscle-specific contractile functions [9, 11].
With high affinity and specificity, homodimeric SRF binds to a consensus cis-element known as a CArG box, with the sequence of CC(A/T)6GG [12, 13]. SRF regulates diverse programs of gene expression through its association with different accessory factors. The most well-studied cofactors of SRF include members of the ternary complex factor (TCF) and myocardin families  of transcription factors. The TCF family of proteins includes ELK1, ELK3 (also known as SAP2, Net) and ELK4 (also known as SAP1). TCFs respond to mitogen-activated protein kinase (MAPK) signaling initiated by serum or growth factors  and is involved in the regulation of IEGs. TCFs interact with SRF and simultaneously bind to an ETS binding site adjacent to the CArG box. Together, the CArG box and the ETS site are recognized as the serum response element (SRE) . Myocardin family members include myocardin, megakaryoblastic leukemia 1 (MKL1, also known as MAL, MRTF-A and BSAC) and MKL2 (also known as MRTF-B). Myocardin is strictly expressed in cardiac and smooth muscle cells, while MKL1 and 2 exhibit broader expression patterns . MKLs connect actin dynamics with SRF activation  and can regulate muscle-specific contractile genes in response to actin polymerization . Unlike TCFs, MKL1 and MKL2 do not bind DNA sequences directly ; instead, they associate with SRF to regulate the transcription of target genes. SRF interaction with MKLs and TCFs is mutually exclusive [20, 21], but recently, MKLs were reported to regulate the expressions of some IEGs in response to serum induction [22, 23]. However, little is known about how these two families coordinate with SRF on a genome-wide level.
Macrophages express a variety of toll-like receptors (TLRs) on their cell surface that enable recognition of molecules, known as pathogen-associated molecular patterns (PAMPs) , that are broadly expressed by pathogens, but not by the host. Zymosan, a yeast cell wall derivative, induces inflammatory responses in macrophages through binding to the dectin-1 receptor or TLR2/6 heterodimers . The function of SRF in macrophages had not been investigated until our previous studies revealed that SRF regulates both general and cell type-restricted cytoskeletal gene expression programs in these cells . Interestingly, we also found that the SRF/MADS (CArG box) motif is highly enriched in the promoters of zymosan-induced genes and that SRF indirectly modulates type I interferon signaling in macrophages . Overall, these studies suggest a possible role of SRF in the immune responses of macrophages.
With recent advances in parallel high throughput sequencing, I sought to map out the genome-wide occupancy of SRF and its cofactors, MKL1/2 and ELK4. In this study, RNA interference was used to knock down SRF, MKL1/2, and ELK4, followed by genome-wide expression profiling analysis and ChIP-seq experiments to identify the target genes and direct binding sites of these cofactors. Together, I demonstrate that the two SRF cofactor families, TCFs and MKLs, regulate distinct subsets of SRF target gene programs during fungal infection in macrophages.
SRF is required for macrophage responses to zymosan treatment
In order to identify the transcription factors that are involved in gene regulation in response to fungal infection in macrophages, I stimulated primary macrophages with zymosan for 1 h and harvested RNA for microarray analysis. Motif analysis on the promoters of genes shown by the array to be induced by zymosan identified the SRF/MADS (CArG box) motif as one of the most highly enriched motifs  (Additional file 1: Figure S1A). This is in accordance with the fact that SRF functions as an immediate responder to external stimuli such as growth factors or serum. Interestingly, Srf transcription was increased 2-fold after 1 h of zymosan treatment, but returned to baseline after 6 h of treatment (Additional file 1: Figure S1B), suggesting that SRF activation is an immediate early phase response. To evaluate if this change in mRNA expression had a functional effect, I transfected RAW264.7 cells with a reporter construct containing 3 tandem SRF-binding cis-elements (3×CArG). After 1 h of treatment with zymosan, I found an approximately three-fold increase in reporter activity (Additional file 1: Figure S1C). Next, I evaluated the impact of knocking down Srf in zymosan treated elicited mouse peritoneal macrophages by using microarray analysis . Considering that the transcription of Srf was induced quickly and that the SRF motif was enriched in the early phase of zymosan treatment, I decided to focus the rest of my study on cells treated with ligand for short periods of time. To identify SRF-dependent genes, I filtered the microarray results to isolate the set of transcripts whose expressions were reduced by more than 1.5 fold with SRF-specific siRNA after 1 h of zymosan treatment. The resulting subset contained 264 non-redundant downregulated genes and 203 upregulated genes (full list in Additional file 2: Table S1), which indicates that SRF can be induced by zymosan stimulation and that it is an important contributor to macrophage responses to external stimuli.
I validated the expression changes of some representative target genes by quantitative PCR (Q-PCR). As expected, several groups of target genes were confirmed as SRF dependent, including: (1) general actin cytoskeleton related genes such as cofilin1 (Cfl1) and Vcl, and the migration related gene, lymphocyte-specific protein 1 (Lsp1); (2) adhesion related genes like thrombospondin 1 (Thbs1); (3) genes related to stimulus responses such as Il10 and Egr3; and (4) genes related to other functions, including fms-related tyrosine kinase 1 (Flt1) and fos-like antigen 2 (Fosl2) (Figure 1B). All of these results indicate that SRF is required for intact expression of genes closely related to macrophage functions.
GO analysis of the genes upregulated by SRF knockdown under zymosan treated conditions resulted in the identification of more generic terms such as “cellular process”, “nucleosome assembly” and “regulation of metabolic process” (Figure 1A, full results in Additional file 3: Table S2, Part II). Besides regulating the transcription of target genes, SRF is known to regulate some miRNAs [31–33] associated with altered expression of mRNAs and proteins. The genes upregulated upon SRF knockdown could potentially be downstream targets of SRF through the regulation of miRNAs. Using Ingenuity Pathway Analysis, I compiled a list of 10 overrepresented miRNAs for the 203 upregulated genes, which included miR-16-5p, miR-489, miR-205-5p, miR-101, miR-291a-3p, miR-204-5p, miR-33, miR-615-3p, miR-424-3p and miR-10a-5p. Although there is no current literature linking any of these miRNAs to SRF, it would be interesting to test, in future studies, whether these miRNAs are actually novel targets of SRF.
MKL1/2 and ELK4 regulate different subsets of genes in zymosan treated macrophages
Previous studies of SRF in muscle cells suggested that SRF participates in different regulatory programs by associating with different transcription cofactors. This mechanism enables SRF to toggle between regulating cell proliferation and growth and orchestrating actin cytoskeletal and contractile homeostasis. I next sought to investigate accessary factors utilized for SRF function in response to zymosan stimulation in macrophages. I focused on two well-known SRF associated cofactor families: the myocardin and TCF families of transcription cofactors.
MKL1 and MKL2, share many redundant functions  and are both highly expressed in primary macrophages. Unlike Srf, mRNA levels of Mkl1 and Mkl2 stay constant after zymosan treatment (Additional file 4: Figure S2A). Because of their many redundancies, I used an siRNA pool targeting both Mkl1 and Mkl2 to knock down their expressions simultaneously to better assess their role in macrophages (Additional file 4: Figure S2A, MKL1/2 will denote both MKL1 and MKL2 in the following text). Elk4 is the dominantly expressed member of the TCF family in primary macrophages (Additional file 4: Figure S2B). Similar to Mkl1/2, Elk4 expression does not change during zymosan treatment (Additional file 4: Figure S2B). Transfection of macrophages with Elk4-specific siRNAs significantly reduced Elk4 expression compared with control siRNA transfected samples (Additional file 4: Figure S2C). I also confirmed that the knockdown effect is specific for Elk4 and that mRNA expression for Elk1 and Elk3 were unaffected (Additional file 4: Figure S2C). Following confirmation of the siRNA knockdown efficiencies, I performed gene expression array analysis on my samples to compare the gene expression changes in Mkl1/2 and Elk4 knockdown cells versus control siRNA transfected cells after zymosan treatment for 1 h.
Using 1.5 fold reduction as a cutoff, I identified a total of 309 genes that were MKL1/2 dependent (full list in Additional file 5: Table S3) and 265 genes that were ELK4 dependent (full list in Additional file 6: Table S4). These results indicate that the absence of these cofactors would have an impact on zymosan induced gene expression in macrophages.
By comparing the 265 ELK4 target genes with the 264 SRF target genes, I identified 24 genes that were dependent on both ELK4 and SRF for their expression (Figure 2A). GO analysis of these 24 genes identified two significantly enriched terms: “response to external stimulus” and “regulation of transcription from RNA polymerase II promoter”. This result indicates that ELK4 is involved in a different aspect of SRF function than MKL1/2. The fact that ELK4 dependent genes are enriched for the GO term related to stress responses in gene ontology analysis is consistent with our finding that besides the SRF motif, the ELK4 motif is also highly enriched in the promoters of zymosan-induced genes in primary macrophages (Additional file 1: Figure S1A). Since the majority of ELK4 dependent target genes are not dependent on SRF for expression, ELK4 may have some SRF independent functions in macrophages. Similar GO analysis on the SRF independent ELK4 target genes showed the term “cellular process” shifted to the top, followed by “response to stress” and “cell division”, etc. (Figure 2C).
Taken together, these findings support the view that MKL1/2 and ELK4 are involved in distinct functions of SRF in zymosan treated macrophages. Specifically, MKL1/2 is involved in actin cytoskeleton organization, ELK4 contributes to establishing responses to external stresses, and both sides constitute important functions of SRF in macrophages. Moreover, I found that both MKL1/2 and ELK4 have roles that are independent of SRF and that they may perform these roles independently or in coordination with other transcription factors. Additional work will be necessary to explore how SRF and these cofactors work on the genome directly and also to identify other potential cofactors.
MKL1/2 and ELK4 dependent target genes show different responses to zymosan induction
I also verified the ELK4 dependence of a subset of stimulus response genes, including Egr1, c-fos, Il10, and Egr3 (Figure 3B). The expression of these four genes can be induced as much as 100 fold by zymosan, in contrast to actin related genes. Although not revealed by microarray evaluation, I found by Q-PCR that knocking down MKL1/2 also impaired the expression of some stimulus response genes such as Egr3 and Il10 (Additional file 4: Figure S2E).
Generation of a BLRP-MKL1-BirA stable cell line for ChIP-seq analysis in RAW264.7 macrophages
While knockdown experiments combined with mRNA expression analysis helped to identify the genes whose expressions are dependent on SRF, MKL1/2 and ELK4, it could not tell me whether these dependencies are through direct transcriptional regulation or through a secondary effect. It has been reported (and our expression data confirms) that SRF regulates the expression of itself [34, 35] and that this effect is dependent on both MKL and TCF cofactors [14, 18, 36]. Thus, it is possible that knocking down MKL1/2 and ELK4 could cause reduced expressions of some target genes through reducing the expression of Srf. As shown in Figure 3C, knocking down MKL1/2 reduced the expression of Srf more than 50%, under both basal and zymosan treated conditions (p < 0.001 and p = 0.017, respectively). Knocking down ELK4 showed a similar effect (p = 0.036 and 0.013, respectively). This result is consistent with previous reports that there is an MKL and TCF-dependent positive feedback loop for SRF-dependent autoregulation [14, 18, 36].
To identify the direct targets of SRF and its cofactors on a genome-wide level, I performed ChIP followed by high throughput sequencing of the enriched DNA fragments (ChIP-seq). MKL1 and MKL2 do not bind DNA sequences directly ; instead, they associate with SRF to regulate the transcription of target genes. As the binding affinity of MKL1/2 to the DNA fragment is relatively weak, conventional ChIP assay with MKL1 antibody failed to provide sufficient enrichment on known target genes in macrophages (data not shown). To this end, I generated a BLRP-tagged MKL1 expression vector and transfected it into RAW264.7 cells to generate a stable cell line exogenously expressing BLRP-MKL1 (BLRP-MKL1-BirA stable cell line). A TEV-based ChIP strategy was then performed for MKL1 using this stable cell line, followed by sequencing analysis. I note here that SRF and ELK4 directly bind DNA, so ChIP-seq using commercial antibodies against endogenous proteins were possible in the MKL1 overexpressed BirA stable cell line.
Stable clones with highly expressed BLRP-MKL1 were identified and selected by RT-qPCR with primers targeting the BLRP sequence (Additional file 7: Figure S3A). Blrp expression was approximately 4000 times higher in the stable cell line compared to parental BirA cells and the Blrp mRNA can be further induced as much as 10 fold following 1 h of zymosan treatment. MKL1 expression levels in this stable clone were twice as high as in the BirA parental cell line under basal conditions and were induced 7.5 fold after 1 h of zymosan treatment (Additional file 7: Figure S3A). The high expression of MKL1 protein was also confirmed by western blot (Additional file 7: Figure S3B).
Global localization of SRF, MKL1 and ELK4 in macrophages
Motif analysis of the 5025 nearest genes associated with SRF peaks by oPOSSUM recovered many transcription factor binding sites (TFBSs). As expected, SRF and ELK4 were among the top hits, together with GABPA, NFκB, Staf, TEAD1, NFYA, RELA, CREB1, STAT1 and RREB1 (Figure 4B). Some of the overrepresented TFs have been reported as cofactors of SRF already, including NFκB, TEAD1, NFYA and RELA [38–42]. My study also revealed additional potential cofactors of SRF, such as GABPA, Staf, CREB1, STAT1 and RREB1. The most highly enriched motif for MKL1 bound genes was SRF, followed by MEF2A, NFκB, STAT1, IRF1, MIZF, FOXF2, GABPA, NFYA, RELA and CREB1 (Figure 4B). Most of the overrepresented TFBSs of MKL1 peaks coincided with those of SRF (including NFκB, STAT1, GABPA, NFYA, RELA and CREB1), suggesting that MKL1 might be involved in the same complex with SRF and other cofactors. However, there is also the possibility that MKL1 might interact with the novel cofactors, independently of SRF, to regulate specific target genes.
For ELK4 bound genes, ELK4 and SRF motifs were significantly enriched, together with NFYA and GABPA (Figure 4B). NFYA has been predicted to interact with both ELK4 and ELK1 . GABPA, another ETS-domain transcription factor, has been reported to show a substantial overlap in promoter occupancy with ELK1 and ELK4 . The association of ELK4 with both NFYA and GABPA motifs suggests that, besides SRF, these factors could be new partners of ELK4 in macrophages and should be experimentally validated in future work.
Classification of SRF peaks with respect to the locations of genes revealed that a large fraction of SRF peaks were located in intergenic regions (37.1%) and introns (32.4%). Approximately 27.4% of the peaks were located in the vicinity of promoters (+/- 1000 bp of a transcription start site) and only 3.0% in exons (Figure 4C). This distribution pattern is consistent with our previous SRF ChIP-seq studies in quiescent primary macrophages . A large fraction of the peaks seen in primary macrophages (923 peaks, 73.1% of the total SRF bound peaks) were also identified in my SRF ChIP-seq in BLRP-MKL1-BirA cells. Genomic annotation of MKL1 binding sites indicated a distribution pattern similar to SRF peaks. 39.7% of the MKL1 peaks were located in intergenic regions, 30.5% in introns, 26.8% in promoters and a very small fraction in exons (3.0%) (Figure 4C). However, the genomic distribution of ELK4 binding sites differed significantly from that of SRF and MKL1. Approximately 42.4% of the ELK4 peaks were located in promoters, 32.1% in intergenic regions, 21.2% in introns and a very small fraction in exons (4.4%) (Figure 4C). This data indicates that ELK4, unlike SRF and MKL1, may function primarily through promoter-proximal regions.
The fact that there is a difference in the number of SRF ChIP-seq peaks in intergenic regions versus those of ELK4, indicates that SRF participates in some unique transcription regulation mechanisms independent of its well-known cofactor, ELK4. There are two possible explanations for this phenomenon. First, SRF could function at distal enhancers for its regulated genes. This possibility was verified by our previous study showing that SRF binds together with PU.1 at distal sites to regulate cell-type specific cytoskeletal genes using an enhancer-based strategy . Second, since many non-coding RNAs (ncRNAs) are found in intergenic regions, it is possible that SRF regulates the expression of ncRNAs. To test this notion, I examined if there are annotated ncRNA loci within 20 kb of the 1827 SRF intergenic binding sites. My in silico analysis showed that a significant portion (10.89%) of the intergenic peaks were associated with annotated ncRNAs (Figure 4D). A total of 316 unique ncRNAs (Additional file 11: Table S8) were associated with intergenic SRF peaks, indicating the possibility of regulation of these ncRNAs by SRF. A majority of the ncRNAs (84.49%, 267) identified are classified as long non-coding RNAs (lncRNAs), while 44 are miRNAs (Figure 4E). In support of the possibility of SRF regulation of ncRNAs, the previously reported SRF target miRNAs, miR-1 and miR-133, were on the miRNA list generated by my in silico analysis.
MKL1 and ELK4 are dedicated to different transcription programs in macrophages
By using KEGG pathway analysis for the SRF, MKL1, and ELK4 bound genes, I found that MKL1 and ELK4 associated genes contribute to different pathways related to SRF. For example, SRF and MKL1 associated genes showed overlapping and enriched pathways of “focal adhesion” and “adherens junction”. In contrast, SRF associated genes were enriched in the “MAPK signaling pathway” with ELK4 associated genes. The KEGG term of “pathways in cancer” was commonly seen in the analysis of all of the 3 groups of target genes (Figure 6B, full results in Additional file 13: Table S10, Parts I, II and III). These functional differences can be illustrated by different target genes regulated by the two different cofactors. Actb is an example of a “focal adhesion” KEGG pathway molecule and Egr1 is a representative “MAPK signaling pathway” molecule. Each of these genes are independently regulated by MKL1 and ELK4 as indicated by genome browser images. As shown in Figure 6C, Actb is an MKL1-dependent and ELK4-independent SRF target gene. In contrast, Egr1 is bound by ELK4 and SRF, but not MKL1.
In this study, I analyzed the role of SRF, and representative members of its cofactor families in macrophages, in the context of zymosan stimulation. Using a knockdown strategy coupled with gene expression array analysis, I identified target genes whose expressions were dependent on the intact expression of SRF, MKL1/2 and ELK4, respectively. Chromatin immunoprecipitation combined with high-throughput sequencing allowed the identification of direct target genes of SRF, MKL1 and ELK4. Taken together, my results indicate that MKL1 and ELK4 contribute to distinct aspects of SRF functions in macrophages.
Here, I show that SRF mediates a response to zymosan stimulation in primary macrophages. The transcription of Srf was increased by zymosan treatment in an early phase, similar to other highly characterized immediate early genes in the literature such as c-fos and Jun. Identification of the SRF binding element, the CArG box, as one of the most highly enriched motifs in the promoters of zymosan induced genes suggests that SRF may play important roles in zymosan responses in macrophages. Using knockdown analysis combined with gene profiling, I identified different target gene sets for SRF and members of two well-known families of SRF accessory cofactors: the myocardin family members, MKL1/2, and the TCF family member, ELK4. With regard to the effects of knocking down SRF, I found that different gene sets with macrophage specific functions were targets of SRF, including genes related to migration, phagocytosis, adhesion and responses to stimuli. In agreement with previous studies performed in other cell types, MKL1/2 regulates the expression of many genes related to actin cytoskeleton organization in macrophages. These genes showed high basal expression and little to no induction in response to zymosan treatment. In contrast, I found that ELK4 target genes are overrepresented in the GO term of “response to stress”. I validated some representative ELK4 target genes and found that the expressions of these genes were highly induced by zymosan treatment and that their inductions were heavily dependent on intact ELK4 expression. Taken together, it’s proposed that MKL1/2 and ELK4 contribute to different functions in the quiescent state compared to the context of an inflammatory response. Moreover, the microarray data revealed that both MKL1/2 and ELK4 have some SRF independent functions and that these functions may involve other novel cofactors.
One of the limitations of microarray analysis is that it is difficult to differentiate the direct target genes from the secondary ones. For example, Srf expression itself can be affected by knocking down MKL1/2 or ELK4. I also noticed that some ELK4 dependent target genes showed decreased expression with MKL1/2 loss, which is probably a secondary effect of SRF expression downregulation. Therefore, I performed ChIP-seq analysis to further identify direct target genes of SRF and its cofactors and to explore novel partners of the three transcription factors.
Motif analysis of the SRF bound peaks identified in my ChIP-seq experiment revealed a set of transcription factors that could be cofactors of SRF besides ELK4. Some of these factors have already been reported as cofactors of SRF. For example, SRF acts in conjunction with TEAD1 for cardiac muscle gene regulation [38, 42], the interaction of SRF and NFYA has been verified in vitro, and the interaction of SRF and NFκB has been observed on the IL-2R enhancer in T lymphocytes . In addition, the NFκB subunit, p65 (also known as RELA), synergizes with SRF to activate an SRE containing reporter . My study also revealed several additional potential cofactors of SRF, including GABPA, Staf, CREB1, STAT1 and RREB1. An independent ChIP-seq study in Jurkat T cells found that a large fraction of SRF peaks occur within 100 bp of GABP peaks, suggesting that SRF may interact physically with GABP . Although CREB has not been reported as directly interacting with SRF, CREB binding protein (CBP) has been found constitutively bound to the SRE on the c-fos promoter . RREB1 and SRF were also both predicted to interact with the same factor, MEF2 . These references provide some evidence for my hypothesis that SRF may interact with cofactors outside of the myocardin and TCF families.
Our previous ChIP-seq study of SRF in primary macrophages indicated a critical role of SRF in promoting hematopoietic-cell-restricted gene expression through binding at distal enhancers, while modulation of generally expressed genes occurred at promoters . A large fraction of the SRF peaks in primary quiescent macrophages also showed up in my ChIP-seq experiment in the BLRP-MKL1-BirA cells. Moreover, I also found that SRF-binding sites are not restricted to promoter regions, but are preferentially located in intergenic regions of the mouse genome. Through mapping of the intergenic peaks to the mouse genome, I found that 10.89% of the peaks were associated with annotated ncRNAs, of which, lncRNAs constitute the major fraction. A list of miRNAs were also associated with intergenic SRF peaks, including the known SRF targets, miR-1 and miR-133 . While MKL1 has a genomic distribution pattern similar to SRF, as previously reported , ELK4 showed a relatively larger fraction of occupancy on promoters. In particular, GABPA and NFYA motifs were found to be enriched on ELK4 bound gene promoters, suggesting a possible partnership of the two transcription factors with ELK4.
In addition to validating the MKL1 and ELK4 binding sites from my ChIP-seq experiment, I also assessed the binding of these factors in the context of zymosan stimulation. With regard to mRNA expression, MKL1 dependent genes showed high basal expression and little to no induction in response to zymosan treatment. By ChIP-qPCR, I found that MKL1 binding to the promoters of its target genes was increased after zymosan treatment. Considering the higher expression of MKL1 after zymosan treatment in the BLRP-MKL1-BirA stable cells, this enhanced occupancy may reflect an increased expression of BLRP-MKL1 protein. In contrast, ELK4 target gene mRNA levels can be highly induced by zymosan treatment. However, in the basal state, ELK4 is already bound to target genes poised for zymosan induction. I speculate that additional events, such as post-translational modification of the SRF-cofactor complex, occur upon zymosan treatment to promote the function of ELK4-SRF at these loci. Kasza, et al. reported similar results in which ELK1 and SRF were both found on the ZC3H12A promoter and that their binding was also not increased upon IL-1β stimulation . These results indicate that transcription factor recruitment may not be a key regulatory event in response to inflammatory stimuli.
In summary, this is the first study to examine the functions of SRF and its key cofactors simultaneously on a genome-wide level through both ChIP-sequencing and transcriptome analysis. The overall view of the genome-wide locations of SRF, MKL1 and ELK4 has been constructed and the results suggest that SRF utilizes MKL1 to fulfill steady state cellular functions, including cytoskeletal organization, and utilizes ELK4 to facilitate acute responses to external infection. Previous studies of SRF largely focused on skeletal, cardiac and smooth muscle cells and neurons. This project sheds light on the functions of SRF, MKL1 and ELK4 in macrophages, indicating their potential roles for both cellular homeostasis and stress responses in immune cells.
Cell culture and transient transfection
Thioglycollate (BD biosciences) -elicited, peritoneal macrophages were prepared as previously described  from 6–8 week old, male, C57BL/6 mice (Harlan). For RNAi experiments, 0.75 million primary macrophages were transfected with nonspecific (NS) control or SMARTpool siRNAs (100 nM, Dharmacon) directed against Srf, Mkl1, Mkl2 and Elk4 using the Deliver X transfection reagent (Panomics) according to the manufacturer’s instructions. RAW 264.7 were transiently transfected with a 3xCArG luciferase reporter using Superfect reagent (Qiagen) and luciferase activities were measured using the luciferase assay system (Promega). Cells were treated with or without zymosan A (1 mg/mL, Sigma-Aldrich) as stated in each experiment.
Generation of BLRP-MKL1-BirA cell lines
To achieve rapid and high affinity purification of MKL1 for ChIP-sequencing assay, I generated a BLRP (biotin ligase recognition peptide)-TEV-Flag-MKL1 expression vector containing a puromycin resistance gene. BLRP is a high affinity substrate for the E. coli biotin ligase, BirA, which biotinylates a lysine residue within the peptide [49, 50]. A RAW264.7 cell line that stably expresses BirA under neomycin selection has been previously described . The BLRP-MKL1 expression vector was transfected into the BirA expressing RAW264.7 stable cell line and stable clones expressing both BirA and BLRP-tagged MKL1 were identified by puromycin and neomycin double selection.
RNA isolation and Q-PCR
Total RNA (isolated by RNeasy kit, Qiagen) was prepared from untreated or zymosan treated primary macrophages and digested with DNase I according to the manufacturer's instructions. cDNA was synthesized from 1 μg of total RNA using Superscript III (Invitrogen) reverse transcriptase according to the manufacturer's instructions. Quantitative real-time PCR (Q-PCR) analysis was performed using 1 μl of cDNA template, 50 ng of each gene-specific primer, and SYBR greenER master mix (Invitrogen) on a 7300 real-time PCR system (Applied Biosystems). Primer sequences are available upon request.
Gene expression profiling
For the Mkl1/2 double knockdown samples, 0.5 μg of purified RNA per sample was labeled using the LRILAK PLUS, two color low RNA input Linear Amplification kit and hybridized to Whole Mouse Genome Microarray 4 × 44 K 60 mer slides (Agilent) according to the manufacturer’s instructions. Slides were scanned using the Agilent GZ505B Scanner. For Elk4 knockdown samples, 100 ng of purified RNA per sample was reverse transcribed using M-MLV (Takara Chemicals) and amplified by an in vitro transcription based method. The Cyanine 3 (Cy3) or Cyanine 5 (Cy5) labeled cDNA was hybridized to the CapitalBio Mouse Genome Oligo Array (CapitalBio) for 16 h at 42°C. Arrays were scanned with a LuxScan™ 10 K-A confocal scanner (CapitalBio), and the data were extracted with GenePix pro4.0 software (Axon Instruments).
Gene ontology (GO) analysis and motif analysis
GO analysis was performed using the web-based functional-annotation tool, DAVID (http://david.abcc.ncifcrf.gov/home.jsp). Gene ontology terms were considered significant if they had a p-value of less than 0.05. The oPOSSUM human/mouse single site analysis tool (http://www.cisreg.ca/oPOSSUM/) was used to identify motifs of 12-bps in length that were overrepresented in different groups of target sequences . Motifs with a Z-score of more than 5 and a Fisher Score of less than 0.05 were regarded as significantly enriched. Terms presented here are sorted by their respective Fisher scores. Analysis of the overrepresented miRNAs upstream of target genes was performed using Ingenuity Pathway Analysis (Ingenuity Systems, http://www.ingenuity.com).
Chromatin immunoprecipitation (ChIP) assay
ChIP assays against MKL1 were performed using the BLRP-MKL1-BirA cell line with methods similar to those previously described in . Briefly, cells were crosslinked with formaldehyde then chromatin was fragmented into 200–300 bp pieces by sonication and subjected to high affinity purification with Dynabeads® MyOne™ Streptavidin T1 (Life technologies). The beads were subjected to AcTEV Protease (Life Technologies) digestion to release the tagged MKL1 proteins complexed with interacting genomic DNA, leaving non-specific proteins bound to the beads. The MKL1-DNA elution without TEV digestion was used as a background control. Elutions from TEV digestion were reverse-crosslinked by heating, and DNA was recovered and purified.
ChIP assays against SRF and ELK4 were performed in the BLRP-MKL1-BirA cell line with methods similar to those previously described in . Immunoprecipitations were performed by incubating with 2.5 μg of anti-SRF antibody (sc-335, Santa Cruz Biotechnology) or anti-ELK4 antibody (sc-13030, Santa Cruz Biotechnology) overnight at 4°C. Protein-DNA complexes were recovered using 50 μl of blocked ImmunoPure Protein A Agarose (Pierce) and then washed, eluted, digested and purified. Rabbit preimmune serum was used as a control for non-specific binding.
High-throughput ChIP sequencing (ChIP-seq) and data analysis
Purified ChIP DNA was adapter ligated and PCR amplified according to the manufacturer’s instructions (Illumina). High-throughput sequencing was performed on an Illumina Genome Analyzer and short reads (first 23 to 25 bp) were mapped to the mouse reference genome. Tag counts for each experiment were normalized to 107 specifically mapped tags. Sequences with tag counts of more than 20 were regarded as binding peaks. To determine SRF peaks, SRF ChIP-seq data was compared to a background data set where SRF ChIP-seq was performed in SRF knockout primary macrophages. Only those peaks with tag counts at least 4-fold more than the tag counts in SRF knockout cells were considered specific. Peaks were visualized by preparing custom tracks using the UCSC Genome Brower (http://www.genome.ucsc.edu/) based on the protocol previously described . Peaks were assigned to specific genes by proximity to the nearest transcription start site. To search for associated ncRNAs, sequences +/-20 kb away from target peaks were extracted and mapped to annotated ncRNAs based on UCSC mm9 and NCBI build37.
I thank Christopher K. Glass, Amy L. Sullivan, Christopher Benner and Jine Li for their help with experiment design and data analysis. I am grateful to Jing Cheng for his helpful discussion and suggestions. I thank Wendy Huang and Ling Yu for their assistance with manuscript revisions. I thank the UCSD Biogem Core facility and CapitalBio Corporation for microarray and sequencing services. I thank Obrizus Communications for the English copy-editing.
This work was supported by a grant from the National Natural Science Foundation of China [Grant number 81200464].
- Shore P, Sharrocks AD: The MADS-box family of transcription factors. Eur J Biochem. 1995, 229 (1): 1-13. 10.1111/j.1432-1033.1995.tb20430.x.PubMedView ArticleGoogle Scholar
- Arsenian S, Weinhold B, Oelgeschlager M, Ruther U, Nordheim A: Serum response factor is essential for mesoderm formation during mouse embryogenesis. EMBO J. 1998, 17 (21): 6289-6299. 10.1093/emboj/17.21.6289.PubMed CentralPubMedView ArticleGoogle Scholar
- Li S, Czubryt MP, McAnally J, Bassel-Duby R, Richardson JA, Wiebel FF, Nordheim A, Olson EN: Requirement for serum response factor for skeletal muscle growth and maturation revealed by tissue-specific gene deletion in mice. Proc Natl Acad Sci U S A. 2005, 102 (4): 1082-1087. 10.1073/pnas.0409103102.PubMed CentralPubMedView ArticleGoogle Scholar
- Miano JM, Ramanan N, Georger MA, de Mesy Bentley KL, Emerson RL, Balza RO, Xiao Q, Weiler H, Ginty DD, Misra RP: Restricted inactivation of serum response factor to the cardiovascular system. Proc Natl Acad Sci U S A. 2004, 101 (49): 17132-17137. 10.1073/pnas.0406041101.PubMed CentralPubMedView ArticleGoogle Scholar
- Alberti S, Krause SM, Kretz O, Philippar U, Lemberger T, Casanova E, Wiebel FF, Schwarz H, Frotscher M, Schutz G, Nordheim A: Neuronal migration in the murine rostral migratory stream requires serum response factor. Proc Natl Acad Sci U S A. 2005, 102 (17): 6148-6153. 10.1073/pnas.0501191102.PubMed CentralPubMedView ArticleGoogle Scholar
- Mylona A, Nicolas R, Maurice D, Sargent M, Tuil D, Daegelen D, Treisman R, Costello P: The essential function for serum response factor in T-cell development reflects its specific coupling to extracellular signal-regulated kinase signaling. Mol Cell Biol. 2011, 31 (2): 267-276. 10.1128/MCB.01058-10.PubMed CentralPubMedView ArticleGoogle Scholar
- Fleige A, Alberti S, Grobe L, Frischmann U, Geffers R, Muller W, Nordheim A, Schippers A: Serum response factor contributes selectively to lymphocyte development. J Biol Chem. 2007, 282 (33): 24320-24328. 10.1074/jbc.M703119200.PubMedView ArticleGoogle Scholar
- Chai J, Tarnawski AS: Serum response factor: discovery, biochemistry, biological roles and implications for tissue injury healing. J Physiol Pharmacol. 2002, 53 (2): 147-157.PubMedGoogle Scholar
- Miano JM: Serum response factor: toggling between disparate programs of gene expression. J Mol Cell Cardiol. 2003, 35 (6): 577-593. 10.1016/S0022-2828(03)00110-X.PubMedView ArticleGoogle Scholar
- Treisman R: Identification of a protein-binding site that mediates transcriptional response of the c-fos gene to serum factors. Cell. 1986, 46 (4): 567-574. 10.1016/0092-8674(86)90882-2.PubMedView ArticleGoogle Scholar
- Miano JM, Long X, Fujiwara K: Serum response factor: master regulator of the actin cytoskeleton and contractile apparatus. Am J Physiol Cell Physiol. 2007, 292 (1): C70-C81.PubMedView ArticleGoogle Scholar
- Norman C, Runswick M, Pollock R, Treisman R: Isolation and properties of cDNA clones encoding SRF, a transcription factor that binds to the c-fos serum response element. Cell. 1988, 55 (6): 989-1003. 10.1016/0092-8674(88)90244-9.PubMedView ArticleGoogle Scholar
- Sun Q, Chen G, Streb JW, Long X, Yang Y, Stoeckert CJ, Miano JM: Defining the mammalian CArGome. Genome Res. 2006, 16 (2): 197-207.PubMed CentralPubMedView ArticleGoogle Scholar
- Gineitis D, Treisman R: Differential usage of signal transduction pathways defines two types of serum response factor target gene. J Biol Chem. 2001, 276 (27): 24531-24539. 10.1074/jbc.M102678200.PubMedView ArticleGoogle Scholar
- Hill CS, Marais R, John S, Wynne J, Dalton S, Treisman R: Functional analysis of a growth factor-responsive transcription factor complex. Cell. 1993, 73 (2): 395-406. 10.1016/0092-8674(93)90238-L.PubMedView ArticleGoogle Scholar
- Wang D, Chang PS, Wang Z, Sutherland L, Richardson JA, Small E, Krieg PA, Olson EN: Activation of cardiac gene expression by myocardin, a transcriptional cofactor for serum response factor. Cell. 2001, 105 (7): 851-862. 10.1016/S0092-8674(01)00404-4.PubMedView ArticleGoogle Scholar
- Sotiropoulos A, Gineitis D, Copeland J, Treisman R: Signal-regulated activation of serum response factor is mediated by changes in actin dynamics. Cell. 1999, 98 (2): 159-169. 10.1016/S0092-8674(00)81011-9.PubMedView ArticleGoogle Scholar
- Miralles F, Posern G, Zaromytidou AI, Treisman R: Actin dynamics control SRF activity by regulation of its coactivator MAL. Cell. 2003, 113 (3): 329-342. 10.1016/S0092-8674(03)00278-2.PubMedView ArticleGoogle Scholar
- Zaromytidou AI, Miralles F, Treisman R: MAL and ternary complex factor use different mechanisms to contact a common surface on the serum response factor DNA-binding domain. Mol Cell Biol. 2006, 26 (11): 4134-4148. 10.1128/MCB.01902-05.PubMed CentralPubMedView ArticleGoogle Scholar
- Wang Z, Wang DZ, Hockemeyer D, McAnally J, Nordheim A, Olson EN: Myocardin and ternary complex factors compete for SRF to control smooth muscle gene expression. Nat. 2004, 428 (6979): 185-189. 10.1038/nature02382.View ArticleGoogle Scholar
- Murai K, Treisman R: Interaction of serum response factor (SRF) with the Elk-1 B box inhibits RhoA-actin signaling to SRF and potentiates transcriptional activation by Elk-1. Mol Cell Biol. 2002, 22 (20): 7083-7092. 10.1128/MCB.22.20.7083-7092.2002.PubMed CentralPubMedView ArticleGoogle Scholar
- Lee SM, Vasishtha M, Prywes R: Activation and repression of cellular immediate early genes by serum response factor cofactors. J Biol Chem. 2010, 285 (29): 22036-22049. 10.1074/jbc.M110.108878.PubMed CentralPubMedView ArticleGoogle Scholar
- Cen B, Selvaraj A, Burgess RC, Hitzler JK, Ma Z, Morris SW, Prywes R: Megakaryoblastic leukemia 1, a potent transcriptional coactivator for serum response factor (SRF), is required for serum induction of SRF target genes. Mol Cell Biol. 2003, 23 (18): 6597-6608. 10.1128/MCB.23.18.6597-6608.2003.PubMed CentralPubMedView ArticleGoogle Scholar
- Akira S, Takeda K: Toll-like receptor signalling. Nat Rev Immunol. 2004, 4 (7): 499-511. 10.1038/nri1391.PubMedView ArticleGoogle Scholar
- Gantner BN, Simmons RM, Canavera SJ, Akira S, Underhill DM: Collaborative induction of inflammatory responses by dectin-1 and toll-like receptor 2. J Exp Med. 2003, 197 (9): 1107-1117. 10.1084/jem.20021787.PubMed CentralPubMedView ArticleGoogle Scholar
- Sullivan AL, Benner C, Heinz S, Huang W, Xie L, Miano JM, Glass CK: Serum response factor utilizes distinct promoter- and enhancer-based mechanisms to regulate cytoskeletal gene expression in macrophages. Mol Cell Biol. 2011, 31 (4): 861-875. 10.1128/MCB.00836-10.PubMed CentralPubMedView ArticleGoogle Scholar
- Xie L, Sullivan AL, Collier JG, Glass CK: Serum response factor indirectly regulates type I interferon-signaling in macrophages. J Interferon Cytokine Res. 2013, 33 (10): 588-596. 10.1089/jir.2012.0065.PubMed CentralPubMedView ArticleGoogle Scholar
- Suzuki K, Takeshita F, Nakata N, Ishii N, Makino M: Localization of CORO1A in the macrophages containing Mycobacterium leprae. Acta Histochem Cytoch. 2006, 39 (4): 107-112. 10.1267/ahc.06010.View ArticleGoogle Scholar
- Jongstra-Bilen J, Jongstra J: Leukocyte-specific protein 1 (LSP1): a regulator of leukocyte emigration in inflammation. Immunol Res. 2006, 35 (1–2): 65-74.PubMedView ArticleGoogle Scholar
- Morley SC: The actin-bundling protein L-plastin: a critical regulator of immune cell function. Int J Cell Biol. 2012, 2012: 935173-PubMed CentralPubMedView ArticleGoogle Scholar
- Park C, Hennig GW, Sanders KM, Cho JH, Hatton WJ, Redelman D, Park JK, Ward SM, Miano JM, Yan W, Ro S: Serum response factor-dependent MicroRNAs regulate gastrointestinal smooth muscle cell phenotypes. Gastroenterol. 2011, 141 (1): 164-175. 10.1053/j.gastro.2011.03.058.View ArticleGoogle Scholar
- Xin M, Small EM, Sutherland LB, Qi X, McAnally J, Plato CF, Richardson JA, Bassel-Duby R, Olson EN: MicroRNAs miR-143 and miR-145 modulate cytoskeletal dynamics and responsiveness of smooth muscle cells to injury. Gene Dev. 2009, 23 (18): 2166-2178. 10.1101/gad.1842409.PubMed CentralPubMedView ArticleGoogle Scholar
- Niu Z, Li A, Zhang SX, Schwartz RJ: Serum response factor micromanaging cardiogenesis. Curr Opin Cell Biol. 2007, 19 (6): 618-627. 10.1016/j.ceb.2007.09.013.PubMed CentralPubMedView ArticleGoogle Scholar
- Belaguli NS, Schildmeyer LA, Schwartz RJ: Organization and myogenic restricted expression of the murine serum response factor gene: a role for autoregulation. J Biol Chem. 1997, 272 (29): 18222-18231. 10.1074/jbc.272.29.18222.PubMedView ArticleGoogle Scholar
- Spencer JA, Misra RP: Expression of the SRF gene occurs through a Ras/Sp/SRF-mediated-mechanism in response to serum growth signals. Oncogene. 1999, 18 (51): 7319-7327. 10.1038/sj.onc.1203121.PubMedView ArticleGoogle Scholar
- Kasza A, O’Donnell A, Gascoigne K, Zeef LA, Hayes A, Sharrocks AD: The ETS domain transcription factor Elk-1 regulates the expression of its partner protein, SRF. J Biol Chem. 2005, 280 (2): 1149-1155. 10.1074/jbc.M411161200.PubMedView ArticleGoogle Scholar
- Verger A, Duterque-Coquillaud M: When Ets transcription factors meet their partners. Bioessays. 2002, 24 (4): 362-370. 10.1002/bies.10068.PubMedView ArticleGoogle Scholar
- Gupta M, Kogut P, Davis FJ, Belaguli NS, Schwartz RJ, Gupta MP: Physical interaction between the MADS box of serum response factor and the TEA/ATTS DNA-binding domain of transcription enhancer factor-1. J Biol Chem. 2001, 276 (13): 10413-10422. 10.1074/jbc.M008625200.PubMedView ArticleGoogle Scholar
- Yamada K, Osawa H, Granner DK: Identification of proteins that interact with NF-YA. FEBS Lett. 1999, 460 (1): 41-45. 10.1016/S0014-5793(99)01311-3.PubMedView ArticleGoogle Scholar
- Kuang AA, Novak KD, Kang SM, Bruhn K, Lenardo MJ: Interaction between NF-kappa B- and serum response factor-binding elements activates an interleukin-2 receptor alpha-chain enhancer specifically in T lymphocytes. Mol Cell Biol. 1993, 13 (4): 2536-2545.PubMed CentralPubMedView ArticleGoogle Scholar
- Franzoso G, Carlson L, Brown K, Daucher MB, Bressler P, Siebenlist U: Activation of the serum response factor by p65/NF-kappaB. EMBO J. 1996, 15 (13): 3403-3412.PubMed CentralPubMedGoogle Scholar
- He A, Kong SW, Ma Q, Pu WT: Co-occupancy by multiple cardiac transcription factors identifies transcriptional enhancers active in heart. Proc Natl Acad Sci U S A. 2011, 108 (14): 5632-5637. 10.1073/pnas.1016959108.PubMed CentralPubMedView ArticleGoogle Scholar
- Mysickova A, Vingron M: Detection of interacting transcription factors in human tissues using predicted DNA binding affinity. BMC Genomics. 2012, 13 (Suppl 1): S2-10.1186/1471-2164-13-S1-S2.PubMed CentralPubMedView ArticleGoogle Scholar
- Boros J, Donaldson IJ, O’Donnell A, Odrowaz ZA, Zeef L, Lupien M, Meyer CA, Liu XS, Brown M, Sharrocks AD: Elucidation of the ELK1 target gene network reveals a role in the coordinate regulation of core components of the gene regulation machinery. Genome Res. 2009, 19 (11): 1963-1973. 10.1101/gr.093047.109.PubMed CentralPubMedView ArticleGoogle Scholar
- Valouev A, Johnson DS, Sundquist A, Medina C, Anton E, Batzoglou S, Myers RM, Sidow A: Genome-wide analysis of transcription factor binding sites based on ChIP-Seq data. Nat Meth. 2008, 5 (9): 829-834. 10.1038/nmeth.1246.View ArticleGoogle Scholar
- Nissen LJ, Gelly JC, Hipskind RA: Induction-independent recruitment of CREB-binding protein to the c-fos serum response element through interactions between the bromodomain and Elk-1. J Biol Chem. 2001, 276 (7): 5213-5221. 10.1074/jbc.M007824200.PubMedView ArticleGoogle Scholar
- Kasza A, Wyrzykowska P, Horwacik I, Tymoszuk P, Mizgalska D, Palmer K, Rokita H, Sharrocks AD, Jura J: Transcription factors Elk-1 and SRF are engaged in IL1-dependent regulation of ZC3H12A expression. BMC Mol Biol. 2010, 11: 14-10.1186/1471-2199-11-14.PubMed CentralPubMedView ArticleGoogle Scholar
- Ghisletti S, Huang W, Ogawa S, Pascual G, Lin ME, Willson TM, Rosenfeld MG, Glass CK: Parallel SUMOylation-dependent pathways mediate gene- and signal-specific transrepression by LXRs and PPARgamma. Mol Cell. 2007, 25 (1): 57-70. 10.1016/j.molcel.2006.11.022.PubMed CentralPubMedView ArticleGoogle Scholar
- Heinz S, Benner C, Spann N, Bertolino E, Lin YC, Laslo P, Cheng JX, Murre C, Singh H, Glass CK: Simple combinations of lineage-determining transcription factors prime cis-regulatory elements required for macrophage and B cell identities. Mol Cell. 2010, 38 (4): 576-589. 10.1016/j.molcel.2010.05.004.PubMed CentralPubMedView ArticleGoogle Scholar
- Fan W, Morinaga H, Kim JJ, Bae E, Spann NJ, Heinz S, Glass CK, Olefsky JM: FoxO1 regulates Tlr4 inflammatory pathway signalling in macrophages. EMBO J. 2010, 29 (24): 4223-4236. 10.1038/emboj.2010.268.PubMed CentralPubMedView ArticleGoogle Scholar
- Ho Sui SJ, Mortimer JR, Arenillas DJ, Brumm J, Walsh CJ, Kennedy BP, Wasserman WW: oPOSSUM: identification of over-represented transcription factor binding sites in co-expressed genes. Nucleic Acids Res. 2005, 33 (10): 3154-3164. 10.1093/nar/gki624.PubMed CentralPubMedView ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly credited. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.