The relationship between transcription initiation RNAs and CCCTC-binding factor (CTCF) localization
© Taft et al; licensee BioMed Central Ltd. 2011
Received: 1 April 2011
Accepted: 3 August 2011
Published: 3 August 2011
Transcription initiation RNAs (tiRNAs) are nuclear localized 18 nucleotide RNAs derived from sequences immediately downstream of RNA polymerase II (RNAPII) transcription start sites. Previous reports have shown that tiRNAs are intimately correlated with gene expression, RNA polymerase II binding and behaviors, and epigenetic marks associated with transcription initiation, but not elongation.
In the present work, we show that tiRNAs are commonly found at genomic CCCTC-binding factor (CTCF) binding sites in human and mouse, and that CTCF sites that colocalize with RNAPII are highly enriched for tiRNAs. To directly investigate the relationship between tiRNAs and CTCF we examined tiRNAs originating near the intronic CTCF binding site in the human tumor suppressor gene, p21 (cyclin-dependent kinase inhibitor 1A gene, also known as CDKN1A). Inhibition of CTCF-proximal tiRNAs resulted in increased CTCF localization and increased p21 expression, while overexpression of CTCF-proximal tiRNA mimics decreased CTCF localization and p21 expression. We also found that tiRNA-regulated CTCF binding influences the levels of trimethylated H3K27 at the alternate upstream p21 promoter, and affects the levels of alternate p21 (p21 alt ) transcripts. Extending these studies to another randomly selected locus with conserved CTCF binding we found that depletion of tiRNA alters nucleosome density proximal to sites of tiRNA biogenesis.
Taken together, these data suggest that tiRNAs modulate local epigenetic structure, which in turn regulates CTCF localization.
In addition to mRNAs, it is now clear that most eukaryotic genic loci generate a complex network of overlapping short (<200) and long non-protein coding RNA (ncRNA) species [1–3]. This growing catalog of ncRNAs includes a host of small RNA (sRNA) transcripts proximal to transcription start sites (TSSs) , some of which are capped  or associate with polycomb repressive complex (PCR2) components [6, 7]. We have recently described a set of nuclear localized dominantly 18 nucleotide tiny RNAs that are generated from regions immediately downstream of TSSs and conserved across metazoa but absent in fungi and plants [8, 9]. We have previously suggested that these transcription initiation RNAs (tiRNAs) may be connected to epigenetic regulation in light of the fact that (i) they originate from the same position relative to the +1 nucleosome in evolutionarily distant animals, suggesting that expression of tiRNAs is influenced by the position of the nucleosome, or vice versa, (ii) they are intimately connected with peaks of RNA polymerase II (RNAPII) binding and levels of gene expression, and (iii) they are enriched genome-wide at chromatin marks associated with the activation, but not elongation, of transcription [4, 8, 9]. We have also observed that tiRNAs are enriched at sites of CCCTC-binding factor (CTCF) , an enigmatic epigenetic regulator that has been recently dubbed 'the master weaver' of the genome .
CTCF is a highly conserved zinc finger protein associated with a diverse set of phenomena including epigenetic insulation, imprinting and transcriptional regulation [10–13]. Intriguingly, CTCF has been shown to both positively and negatively regulate gene expression in a gene-specific and context-specific manner [10, 14]. A resolution to this apparent incongruity has recently been proposed: CTCF does not directly influence the surrounding genes or transcriptional machinery, but rather acts as a three-dimensional orchestrator of chromatin architecture . CTCF's involvement in a wide range of epigenetic phenomena appears to be the secondary, but undoubtedly regulated, effects of its ability to form specific intrachromosomal and interchromosomal connections .
CTCF has been shown to regulate the expression of several tumor suppressor genes, including p21 (informal gene name for the cyclin-dependent kinase inhibitor 1A gene, CDKN1A) [11, 15] and p16 (INK4a), the latter by insulating the promoter from silent-state histone modifications such as H3K27 trimethylation (H3K27me3) . CTCF has also recently been shown to be involved in the epigenetic regulation of frataxin (FXN), a gene mutated and silenced in Friedreich ataxia, which causes progressive damage to the nervous system . Loss of CTCF binding in the 5' untranslated region (UTR) of FXN leads to a deficiency of the FXN transcript, an increase in FXN antisense transcript 1, and heterochromatin formation involving the +1 nucleosome . Given that tiRNAs and RNAPII are intimately connected, and that there is increasing evidence that CTCF and RNAPII are coupled together (see below) [18–22], we speculated that tiRNAs at CTCF-binding sites might be involved in the alteration of local chromatin states, and therefore transcript expression, via indirect regulation CTCF.
Results and discussion
We have previously shown that tiRNAs isolated from THP-1 cells (a human monocytic leukemia cell line) are systematically enriched at white blood cell CTCF binding sites . To examine if this relationship is preserved across cell and tissue types, and multiple species, we interrogated small RNA enrichments at CTCF binding sites in MCF-7 breast cancer cells and mouse embryonic stem cells (mESCs) (for a full list of data sources please see (Additional file 1, Table S1).
MCF-7 CCCTC-binding factor (CTCF), RNA polymerase II (RNAPII) and CTCF-RNAPII site intersections with small RNAs (sRNAs)
Total number of MCF-7 sites
Number that overlap with sRNAs (%)
Total number of sRNAs overlapped (percentage total sRNAs)
CTCF + RNAPII
Mouse embryonic stem (mES) CCCTC-binding factor (CTCF), RNA polymerase II (RNAPII) and CTCF-RNAPII site intersections with small RNAs (sRNAs)
Total number of mES sites
Number that overlap with sRNAs (%)
Total number of sRNAs overlapped (percentage total sRNAs)
CTCF + RNAPII
To examine if the association between tiRNAs, CTCF and RNAPII extends beyond MCF-7 and mESCs we identified CTCF sites conserved across an additional eight human cell lines (GM12878, HepG2, HMEC, HSMM, HUVEC, K562, NHEK, and NHLF cells) [23, 24] and RNAPII sites conserved across three (K562, GM12878, and HUVEC), and intersected them with nuclear and cytoplasmic small RNAs (sRNAs) from THP-1 and 5-8f cells (a nasopharyngeal carcinoma cell line ) and MCF-7 total sRNAs. Despite the fact that these datasets are derived from disparate origins, nuclear sRNAs from THP-1 and 5-8f are 33-fold and 16-fold enriched, respectively, and total sRNAs from MCF cells are 31-fold enriched at conserved CTCF-RNAPII sites (Additional file 2, Figure S1a). Additionally, like the MCF-7 and mESC datasets discussed above, the small RNAs that overlap CTCF-RNAPII sites are dominantly 18 nucleotides, indicating they are tiRNAs (Additional file 2, Figure S1b-d). Overall, greater than 10% of the conserved CTCF sites, and 60% of conserved CTCF-RNAPII sites, overlap with sequences that generate tiRNAs (Additional file 3, Table S2). To further ensure that the tiRNA enrichment at CTCF-RNAPII sites was robust we parsed the conserved human CTCF sites into two groups by origin, 'cancer' and 'normal', and removed all CTCF sites that overlapped with TSSs, repeat masker annotations and small RNAs. Using the most robust RNAPII datasets in each group (MCF-7 and HUVEC for 'cancer' and 'normal', respectively), we found that this dramatically reduced set still shows robust enrichment for tiRNAs at CTCF-RNAPII sites (Additional file 4, Figure S2).
The p21 locus encodes two tiRNA clusters, one at the TSS (tss-tiRNAs) and the other at the CTCF-RNAPII site (CTCF proximal (cp)-tiRNAs) that are antisense to one another. The tss-tiRNAs are sense to the gene (as observed generally), while the cp-tiRNAs are antisense. Both overlap distinct peaks of RNAPII binding, suggesting that their biogenesis is tied to RNAPII molecules heading in opposite directions, possibly linked to nucleosome position , and this reinforces our previous finding that tiRNAs are found at sites of active RNAPII transcription initiation outside of canonical transcription start sites (Figure 2).
As reverse transcription in the qPCR samples was not specifically primed (Figure 3a, b), these transcripts might represent sense and/or antisense transcripts associated with these regions  or any of the plethora of splice variants. To determine the extent of the effect that the cp-tiRNA sponge has on relative sense and antisense p21 transcript levels, strand-specific reverse transcription PCR (RT-PCR) was performed. Upon treatment with the cp-tiRNA sponge, p21 mRNA, sense p21 alt , and antisense p21 alt transcript levels increased, whereas transcripts antisense to p21 mRNA were unaffected (Figure 3c, d). These data indicate that CTCF-proximal tiRNAs may be involved in the negative regulation of p21.
We next performed the reciprocal experiment testing the effect that overexpression of CTCF-proximal tiRNA mimics has on p21 expression. Consistent with our speculation that tiRNAs are connected to transcriptional regulation, we found that overexpression of a set of four cp-tiRNA mimics resulted in a marked reduction of the p21 mRNA (Figure 3e). To confirm that the effect of the cp-tiRNA sponges and mimics was not restricted to MCF-7 cells we repeated these experiments in THP-1 cells and found that the principal results were recapitatulated (Additional file 6, Figure S4), indicating that cp-tiRNAs have a regulatory effect on p21 transcription in multiple human cell systems.
Consistent with this, treatment with the cp-tiRNA sponge resulted in a significant increase in CTCF binding (Figure 5a), and overexpression of the cp-tiRNA mimics exhibited a significant decrease of CTCF binding (Figure 5b). This indicates that the effect of cp-tiRNAs on p21 transcription is directly related to its ability to modulate CTCF binding, which may be involved in three-dimensional (re)ordering of the p21 locus. Indeed, western blot analysis showed that p21 protein levels were increased in samples treated with the cp-tiRNA sponge, and decreased in samples treated with the cp-tiRNA mimic constructs (Figure 5d, e). Taken together, these data suggest that one function of p21 cp-tiRNAs may be to inhibit CTCF binding to the p21 gene, possibly as a means to repress transcription and downstream translation.
The mechanism by which tiRNAs inhibit CTCF localization is unclear, although there are several obvious possibilities: (i) cp-tiRNAs spanning the CTCF binding site may coat local chromatin by binding nascent transcripts  or chromatin associated RNAs [40–42], which could sterically hinder CTCF from accessing its binding site; (ii) cp-tiRNAs may directly interact with CTCF and inhibit CTCF binding, although attempts to immunoprecipitate CTCF with biotin-linked cp-tiRNAs were unsuccessful (data not shown); (iii) cp-tiRNAs may bind to regulatory elements including cis-acting ncRNAs (for example, bx332409 at p21) or polycomb group components and direct their action to specific sites; or (iv) cp-tiRNAs may serve as sequence-specific markers for chromatin modification complexes.
The data presented here indicate that cp-tiRNAs can have a powerful effect on CTCF binding and local transcription. Indeed, tiRNA-mediated modulation of CTCF binding at p21 not only reduces p21 mRNA and protein levels, but also appears to affect chromatin state and expression of p21 alt transcripts. This suggests that at some loci the role of tiRNAs, whose biogenesis is connected to RNAPII activity and progression, may be to modulate (presumably indirectly) local chromatin states, which in turn regulates the binding of other factors including CTCF. Indeed, the relationship between tiRNAs and epigenetic structures may indicate a self-reinforcing feedback loop wherein the RNAPII-nucleosome interaction generates tiRNAs, which in turn serve to mark (directly or indirectly) nucleosome positions and/or epigenetic state. Although the mechanism of tiRNA action is still elusive, this work is the first to report a role for tiRNAs in gene regulation, and shows that at least a subset of tiRNAs are functional modulators of CTCF, which may lead to the development of novel RNA-based therapeutics that target epigenetic regulation of gene structure and transcription.
Bioinformatic analyses were performed on a local high-performance computer at the UQ Institute for Molecular Bioscience that houses a mirror of the UCSC Genome Brower . We used a suite of in-house AWK, C, Perl, and Python scripts and UCSC backend tools. All small RNA, CTCF binding and RNAPII binding data were obtained from publicly available sources and are listed in detail in Additional file 1, Table S1. For all ChIP-seq datasets the available peak calls were used, except in the case of the mES RNAPII data where peaks were defined as regions with signal greater than 3 SDs from the mean. All intersections were performed using a modified version of the UCSC backend tools bedIntersect or overlapSelect. A minimum of 1 bp of overlap was required, but generally >50% of any given feature intersected with another. The relative enrichment of small RNAs at CTCF sites with or without RNAPII coverage was computing using an in-house (Perl) bootstrapping program over 1,000 iterations as previously described . Bootstrapping was constrained such that the randomized placements of small RNAs excluded TSSs, known small RNA annotations, repeat masker annotations and genome assembly gaps. For the analysis of the MCF-7, mES, and human CTCF data grouped into 'cancer' and 'normal' the data was parsed so that data points that intersected with known small RNA annotations, the 500 bp adjacent to TSSs, repeat masker annotations or Ensembl annotations less than 300 nucleotides were removed. The conserved CTCF site data set were generated by taking all the peaks identified by Broad/ENCODE as significant across all eight sources (see Additional file 1, Table S1) and intersecting them against one another using the UCSC backend tool overlapSelect. Overlapping CTCF features (called peaks) were collapsed into one concordant set of coordinates using the UCSC tool featureBits. Small RNA size distributions were computed as previously described .
Cell culture and transfection
Experiments were conducted in MCF-7 and THP-1 cells cultured at 37°C and 5% CO2 in Dulbecco's modified Eagle's medium or RPMI 1640 (THP-1 cells only) supplemented with 10% fetal bovine serum and penicillin-streptomycin (Life Technologies, Carlsbad, California, USA). Plasmid transfections of MCF-7 cells were performed using Lipofectamine 2000 (Life Technologies, Carlsbad, California, USA) per the manufacturer's guidelines at a concentration of 1 μg/1 × 106 cells. Plasmid transfections of THP-1 cells were carried out using the Neon electroporation system (Life Technologies, Carlsbad, CA, USA), per manufacturer's guidelines.
Sponge and mimic plasmid construction
Sponge plasmids: reverse complement sequences to the promoter-proximal and CTCF-proximal tiRNA sites in p21 were amplified from MCF-7 genomic DNA by polymerase chain reaction (PCR) using primers with Bgl II restriction sites on either end (Additional file 3, Table S2). Amplified DNA was digested by Bgl II and ligated into the similarly cut pCDNA3 U6M2 plasmid. The parent vector, pCDNA3 U6M2, was used as a control in sponge experiments. The resulting sponge sequences were: p21 promoter-proximal tiRNA sponge (pp-tiRNA) 5'CCGCCGGCCCGGGGTCCCCTGTTGTCTGCCGCCGCTCTCTCACCTCCTCTGAGTGCCTCGGT GCCTCGGCGAATCCGCGCCCAGCTCCGGCTCCACAAGGAACTGACTTCGGCAGCTGCTCACA CCTCAGCTGG3' and p21 CTCF-proximal tiRNA sponge (cp-tiRNA) 5'GGGCTCAGGGCTTCCCGACCTAGCCCAGATTCCCTCTCCGAAAGCTACAGGGCTGAGCGGA GCAGGGGGGCGAGTCGCCCCCTGGGGCGCCGCCGCCTGGCGCGGACCACAGCGCGTCCTCT CCGTCCCAAACCCCTGGGGGACACTTGCGCCCTCTTCGTGAGGAAAAGCATCTTGGAGCTGG GTTAGGAACTTGGGGCGCCCAGGCAGCTTCCCCTCTCCTTGCCTCCCTCCACGTCGCGTTTCT GGGAGGACTTGCGAGCGGTTTTGTTTTCGTTGCTCCCGTCTATTTTTATTTTCCAGGGATCTGA CT3'.
Sponge constructs for C2Orf41 and STARD13 were constructed by annealing the respective oligonucleotides together (Additional file 3, Table S2), top strand oligo (200 μM): 5 μl bottom strand oligo (200 μM): 5 μl, 10 × Oligo Annealing Buffer (BLOCK-iT kit*, Life Technologies, Carlsbad, California, USA): 2 μl, DNase/RNase-free water: 8 μl. The reaction was heated to 95°C for 4 min, cooled to room temperature and treated to polynucleotide kinase (PNK) (1 μl PNK (10,000 U/ml), 1 μl T4 ligase buffer, 4 μl dsOligo, 4 μl water, at 37°C for 30 min). The oligonucleotides were purified using minelute PCR purification kit and ligated to pCDNA3 U6M2 as described above.
A negative control and four sequences of CTCF-proximal tiRNAs were synthesized (Integrated DNA Technologies) and cloned into the BLOCK-iT U6 RNAi Entry Vector (Life Technologies, Carlsbad, CA, USA) per manufacturer's guidelines. The mimics, four predominant cp-tiRNA sequences (Additional file 9, Table S3) were independently cloned into the U6 driven BLOCK-iT system (Life Technologies, Carlsbad, CA, USA). The resultant plasmids were transfected into MCF-7 cells as described previously .
Quantitative strand-specific PCR (qPCR)
RNA was extracted (RNeasy Qiacube, Qiagen), DNase treated (TURBO DNase, Ambion), reverse transcribed (Reverse Transcriptase Core Kit, Eurogentec) using the non-specific or indicated primers (for strand-specific RT-PCR), and analyzed by qPCR using indicated primers (Kapa Sybr Fast Universal qPCR Kit, Kapa Biosystems, Woburn, MA, USA) (Additional file 9, Table S3). In strand-specific RT-PCR, reverse transcription is primed with a gene specific forward or reverse primer alone, thereby generating cDNA of specifically the antisense or sense strand of the targeted region respectively. Controls for this assay are reverse transcription or template RNA in the absence of any primer. Quantitative PCR (qPCR) is then performed using forward and reverse primers, yielding amplicons that represent sense or antisense transcripts overlapping that region with the control no primer RT sample values subtracted as background from the directional RT primed samples.
ChIP assays were performed as previously described . DNA was immunoprecipitated using anti-RNAPII phosphor-S2 (AbCam no. ab5095, AbCam Cambridge, MA USA), anti-H3K27me3 (Cell Signaling no. 9756S, Danvers, MA, USA), or anti-CTCF (Santa Cruz Biotechnology no. sc-15914, Santa Cruz, CA, USA) antibody bound complexes were then pulled down using magnetic Dynabeads Protein A (Life Technologies, Carlsbad, CA, USA). DNA was then recovered by phenol/chloroform extraction and analyzed by qPCR using indicated primers (Additional file 9, Table S3) (Kapa Sybr Fast Universal qPCR Kit, Kapa Biosystems, Woburn, MA, USA).
Cells were lysed in modified RIPA buffer (25 mM Tris HCl, pH 7.5, 15 mM NaCl, 1% Nonidet P-40, 1% NaD, and 0.1% SDS) and separated on a NuPAGE 4% to 12% BisTris gel (Life Technologies, Carlsbad, CA, USA). Proteins were transferred to a nitrocellulose membrane which was blocked with 5% milk for 1 h and then incubated overnight at 4°C with anti-p21 (Cell Signaling no. 2946) and anti-glyceraldehyde 3-phosphate dehydrogenase (GAPDH) (Millipore no. MAB374, Billerica, MA, USA) antibodies. The membrane was then washed (10 mM Tris HCl, pH 7.5, 50 mM NaCl, 0.075% Tween 20) and incubated with an anti-mouse horseradish peroxidase-conjugated secondary antibody for 1 h at room temperature (Upstate no. 12-349, Billerica, MA, USA). The membrane was then washed, treated with chemiluminescent detection reagent (HyGLO, Denville Metuchen, NJ, USA), and exposed to film. Blot density of a binary image of Figure 5d was calculated using ImageJ. Results were standardized to GAPDH and expressed as fractions of control values.
This project was supported by NIH R01 grants HL083473-02 and AI084406-01A1 (KVM) a University of Queensland Postdoctoral Research Fellowship (RJT) and ARC Discovery Project Grant DP DP0988851 and ARC Federation Fellowship FF0561986 (JSM).
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