- Open Access
Loss of SETDB1 decompacts the inactive X chromosome in part through reactivation of an enhancer in the IL1RAPL1 gene
Epigenetics & Chromatin volume 11, Article number: 45 (2018)
The product of dosage compensation in female mammals is the inactive X chromosome (Xi). Xi facultative heterochromatin is organized into two different types, one of which is defined by histone H3 trimethylated at lysine 9 (H3K9me3). The rationale for this study was to assess SET domain bifurcated 1 (SETDB1) as a candidate for maintaining this repressive modification at the human Xi.
Here, we show that loss of SETDB1 does not result in large-scale H3K9me3 changes at the Xi, but unexpectedly we observed striking decompaction of the Xi territory. Close examination revealed a 0.5 Mb region of the Xi that transitioned from H3K9me3 heterochromatin to euchromatin within the 3′ end of the IL1RAPL1 gene that is part of a common chromosome fragile site that is frequently deleted or rearranged in patients afflicted with intellectual disability and other neurological ailments. Centrally located within this interval is a powerful enhancer adjacent to an ERVL-MaLR element. In the absence of SETDB1, the enhancer is reactivated on the Xi coupled with bidirectional transcription from the ERVL-MaLR element. Xa deletion of the enhancer/ERVL-MaLR resulted in loss of full-length IL1RAPL1 transcript in cis, coupled with trans decompaction of the Xi chromosome territory, whereas Xi deletion increased detection of full-length IL1RAPL1 transcript in trans, but did not impact Xi compaction.
These data support a critical role for SETDB1 in maintaining the ERVL-MaLR element and adjacent enhancer in the 3′ end of the IL1RAPL1 gene in a silent state to facilitate Xi compaction.
The XX/XY chromosome mode of sex determination necessitates the need to compensate levels of X-linked gene expression between the sexes. In mammals, this is achieved through the process of X chromosome inactivation (XCI), whereby one of the two X chromosomes in females is rendered transcriptional silent early in development . Gene silencing at the inactive X chromosome (Xi) is achieved by repackaging the chromosome into facultative heterochromatin, which includes acquisition of repressive histone marks such as histone H3 methylated at lysine 9 and trimethylated at lysine 27 (H3K27me3) [2,3,4,5]. Histone H3 trimethylated at lysine 9 (H3K9me3) and H3K27me3 occupy distinct regions of the Xi [6,7,8], with H3K27me3 bands associating with gene-rich regions of the chromosome and H3K9me3 predominantly occupying gene-poor regions [7, 9]. H3K27me3 is catalyzed by the histone methyltransferase (HMTase) enhancer of Zeste 2 (EZH2) [10,11,12,13], which applies the mark to chromatin of the Xi early during XCI [4, 5]. In contrast, while H3K9me3 has been reported at the Xi [6,7,8], which HMTase is responsible for the maintenance of this modification at the Xi is uncertain [14, 15]. Recent data suggest that SET domain bifurcated 1 (SETDB1), an H3-K9 HMTase with highest activity for trimethylation of lysine 9 [16, 17], is involved in maintaining gene silencing on the mouse Xi , and while it is important for establishing H3K9me3 on the mouse Xi  and is enriched on the vole Xi in trophoblast stem cells , a central role for this protein in maintaining this mark post-XCI is less certain . SETDB1 is important for gene and repeat silencing during development , and a role for this protein in maintaining H3K9me3 at the human Xi has not been explored. Therefore, we sought to further investigate the relationship between SETDB1 and the human Xi.
By generating SETDB1 knockouts (KO) in human cells, we reveal that while SETDB1 is not required to maintain chromosome-wide H3K9me3 at the human Xi, its loss results in decompaction of the Xi chromosome territory. The most obvious chromatin change in the Xi corresponds to a 0.5-Mb interval embedded within the 3′ end of the large interleukin-1 receptor accessory protein-like 1 (IL1RAPL1) gene that transitioned from a H3K9me3-defined region of heterochromatin to euchromatin. Centrally located within this interval we identified a powerful enhancer element adjacent to an ERVL-MaLR that is reactivated from the Xi. Through characterization of these elements and their deletion from either the Xa or Xi, we reveal complex cis and trans effects that influence IL1RAPL1 transcription and chromosome compaction.
SETDB1 loss results in decompaction of the territory of the Xi
In order to knock out SETDB1, we used the fast ligation-based automatable solid-phase high-throughput system (FLASH) to assemble a pair of previously reported active transcription activator-like effector nuclease (TALENs) that target exon-2 (Fig. 1a) of the SETDB1 locus . These were introduced into hTERT-RPE1 (RPE1) cells along with a promoterless neomycin trap targeting construct  to act as a template for homology-mediated repair (Additional file 1). Numerous independent targeted clones were isolated (Additional file 2), and three were selected for further investigation. Two clones (S6 and S40) had exchanged exon-2 with the neomycin cassette at both alleles. The promoter trap construct is designed to terminate transcription immediately after transcribing through the cassette. Therefore, we would expect not to be able to detect SETDB1 RNA beyond exon-1 for these clones, which was indeed the case with the lack of product by reverse transcription PCR (RT-PCR) (Fig. 1b) and quantitative RT-PCR (qRT-PCR) (Fig. 1c). Furthermore, massively parallel sequencing of RNA (RNA-Seq) shows a lack of signal at and beyond exon-2 (Fig. 1d) confirming the lack of SETDB1 transcript in these clones. The third clone (S3) had incorporated the neomycin cassette at one allele, whereas the second allele was disrupted by non-homologous end joining. As such, we would expect transcript lacking exon-2 (and the translation initiation codon) to be generated from this allele. RT-PCR clearly detects transcript without exon-2 (Fig. 1b) that exists at significantly lower levels than parental cells (Fig. 1c). Western blot analysis using an antibody raised against the C-terminus of the protein failed to detect SETDB1 protein in any of the three clones, validating each as SETDB1-KOs (Fig. 1e). Initially we looked to see whether loss of SETDB1 impacted facultative heterochromatin bands along the length of the Xi at metaphase. However, the typical alternating banding pattern of H3K9me3 and H3K27me3 at the RPE1 Xi  was not obviously impacted (Fig. 2a). Next, we examined the organization of the Xi at interphase. RPE1 and SETDB1-KO clones were stained for H3K27me3 and heterochromatin protein 1 beta (HP1β) as a marker of the H3K9me3 territory. While both territories of the bipartite structure could be detected , we found that in SETDB1-KO clones the H3K27me3 territory was very obvious and substantially larger than that of parental RPE1 cells (Fig. 2b) in the absence of any increase in overall nuclear volume (Additional file 3) or change to H3K27me3 banding at the Xi (Fig. 2a). Volume measurements of H3K27me3 at the Xi confirmed that the Xi volume had significantly increased in SETDB1-KO clones (Fig. 2c).
Loss of SETDB1 results in gain of euchromatin within the 3′ end of the IL1RAPL1 gene on the Xi
Given the decompaction of the Xi in the absence of large-scale facultative heterochromatin change, we next sought to determine whether changes to euchromatin markers at the Xi had occurred. Typically in female nuclei, histone H3 dimethylated at lysine 4 (H3K4me2) shows a general nuclear distribution with obvious underrepresentation at nucleoli and the territory of the Xi that appears as a hole in the staining pattern within which is a single intensely staining focus [2, 23]. This signal was subsequently shown to correspond to the macrosatellite DXZ4 that adopts the opposite chromatin configuration than the flanking chromosome arms: heterochromatin on the Xa and euchromatin on the Xi . While RPE1 cells showed a single focus, in all three mutant clones two intense foci were observed (Fig. 3a) in significantly more cells (Fig. 3b). In addition to DXZ4, nucleosomes of the FIRRE and ICCE tandem repeats are uniquely marked by H3K4me2 at the Xi alleles  and, despite residing many megabases apart, these large tandem repeats make frequent Xi-specific contact [25,26,27]. One possible explanation for the observation of two foci at the Xi could be reduced contact between the three repeat elements accounting the decompaction phenotype. However, none of the tandem repeats overlapped with the new H3K4me2 signal by FISH (data not shown). This suggested that a new euchromatin band had been acquired on the Xi in SETDB1 mutants. To confirm that the H3K4me2 signals reside within the territory of the Xi, we compared the location of the dot/dots with a robust Xi territory marker structural maintenance of chromosomes flexible hinge domain containing 1 (SMCHD1) . Both H3K4me2 dots overlapped SMCHD1 signal at the Xi in the SETDB1-KO clones (Fig. 3c). As a large body of heterochromatin, the Xi is also under represented for histone acetylation . Immunofluorescence to acetylated lysine also clearly defines the territory of the Xi and can detect the euchromatic DXZ4 as a single focus . Like H3K4me2, a single focus of acetylated lysine could be detected within the territory of the Xi in parental RPE1 cells, whereas two foci could be detected in SETDB1-KO cells (Fig. 3d). To identify the origins of this new signal, the distribution of H3K4me2 was determined at metaphase. While RPE1 metaphase Xi showed characteristic intense H3K4me2 bands at DXZ4 and the pseudoautosomal region , the Xi in SETDB1-KO clones had an additional intense H3K4me2 band centered at Xp21 (Fig. 3e). Chromatin immunoprecipitation coupled with high-throughput sequencing (ChIP-Seq) was employed in order to fine map the region of chromatin change. Consistent with the metaphase chromosome fluorescence microscopy, a broad interval of approximately 500 kb embedded within the 3′ end of the IL1RAPL1 gene showed gain of H3K4me2 and a corresponding reduction in H3K9me3 for the same region (Fig. 4). Bacterial artificial chromosomes (BACs) from the chromatin change region were used as FISH probes on metaphase chromosomes stained for H3K4me2. Hybridizing signals overlapped with the new H3K4me2 band at the Xi, whereas the same interval on the Xa appears to lack H3K4me2 signal (Additional file 4). Based on these data, we conclude that loss of SETDB1 results in the acquisition of a broad region of euchromatin within the 3′ end of the IL1RAPL1 gene on the Xi.
IL1RAPL1 is involved in regulating neuron development [31,32,33,34,35], and mutations in IL1RAPL1 have been reported to cause X-linked intellectual disability  and autism spectrum disorder , and it is downregulated in brain tumor cell lines and xenografts . Intriguingly, the genomic interval embedded within IL1RAPL1 that shows chromatin change in the absence of SETDB1 falls within a common fragile site (FRAXC) on the X chromosome , indicating that not only is this region susceptible to chromatin transformation but also genomic instability, the two of which may be mechanistically linked.
IL1RAPL1 transcript levels differ between the 5′ and 3′ ends and are altered in the absence of SETDB1
In order to determine the impact that the observed euchromatic transition on the Xi may have on expression of IL1RAPL1, we began by further characterizing IL1RAPL1 expression in RPE1 and SETDB1-KO clones. Initially qRT-PCR was performed on cDNA from parental RPE1 cells using oligonucleotide primer sets designed to amplify the 5′ and 3′ end of IL1RAPL1 (Fig. 5a). Unexpectedly, transcript levels at the 3′ end were dramatically higher than the 5′ end (Fig. 5b), suggesting that a substantial proportion of transcripts from the 3′ end may be transcribed from a promoter distinct from the one located at the very 5′ end of the gene. The qRT-PCR analysis was repeated to compare RPE1 and SETDB1-KO clones. Transcripts originating from the 5′ end were significantly reduced in SETDB1-KO clones, whereas transcripts from the 3′ end were significantly elevated (Fig. 5c). To validate these observations and extend them to single-cell analysis, BAC clones from the 5′ and 3′ regions of IL1RAPL1 were selected for use in RNA FISH experiments (Fig. 5d). RNA FISH was performed with the IL1RAPL1 BACs in combination with an XIST probe to define the territory of the Xi in the nucleus. Four distinct patterns were observed including no IL1RAPL1 signal, IL1RAPL1 signal distinct from the XIST cloud (interpreted as originating from the Xa), IL1RAPL1 signal associated with the XIST cloud (interpreted as originating from the Xi) and two IL1RAPL1 signals (one associated with the XIST cloud and one distinct, interpreted as being expressed from both alleles) (Fig. 5e). Consistent with the qRT-PCR data, transcripts originating from the 5′ end were significantly reduced in SETDB1-KO clones (Fig. 5f) and almost exclusively originate from the Xa (compare Fig. 5f and g). In contrast, expression from the 3′ end was significantly increased from the Xa (Fig. 5f) and Xi (Fig. 5g) with most transcripts originating from the Xi. Of note, in SETDB1-KO clones 3′ probe RNA FISH detected at the Xi most often appeared as multiple signals interspersed with the XIST cloud, which is in contrast to RNA FISH signals at the Xa that typically were single or double hybridizing foci (most likely due to cells in mid-late S-phase or G2, post-Xa DNA replication) (Fig. 5e). Although at very low incidence, we did occasionally detect 5′ and 3′ RNA FISH signals in proximity to the XIST cloud in parental RPE1 cells, suggesting that under normal circumstances, IL1RAPL1 escapes XCI albeit at substantially lower levels than the expression from the Xa (compare RPE1 between Fig. 5f, g).
A powerful enhancer located in the 3′ end of IL1RAPL1 drives bidirectional expression of a novel antisense long noncoding RNA and short sense transcript isoform
These data support a model in which an alternative isoform of IL1RAPL1 originates from the 3′ end of the gene that is dramatically upregulated from the Xa and Xi in the absence of SETDB1. In order to validate this model, we identified four informative single nucleotide polymorphisms (SNPs) within the 3′ transcript [rs140261831, rs113985890, rs190632360 and rs144991617: SNP-A through D, respectively (Additional file 5)]. RPE1 cells are clonal and therefore the chromosomes that were selected as the Xa and Xi are always the Xa and Xi in all cells at all times . Therefore, SNP alleles can be assigned to Xa and Xi, and their presence in RNA indicates their transcriptional origins, although not quantitatively by this approach. Oligonucleotide primers flanking each SNP were designed (Additional file 6) and used to PCR amplify the SNPs in RPE1 DNA and a rodent–human somatic cell hybrid in which the RPE1 Xa is the only human chromosome. Sequencing of the PCR products allowed assignment of SNP alleles to the Xa and Xi. Next, the same intervals were amplified and sequenced from RPE1 and SETDB1-KO clone cDNA. In RPE1 cells, only the Xa allele was detected. This indicates either that Xi 3′ transcript is too low for the SNP allele to be detected by this method or that the observed low-level RNA FISH signals may actually be Xa-derived transcript in the vicinity of the Xi. In contrast, the Xi allele was readily detected in cDNA from SETDB1-KO clones, with minor to moderate contribution of the Xa allele (Additional file 5).
Next, we set out to identify regulatory elements within the 3′ interval. In addition to H3K4me2 and H3K9me3 ChIP-Seq, we also included histone H3 acetylated at lysine 27 (H3K27Ac) (Fig. 4), a histone modification associated with enhancer activity [41,42,43]. Numerous novel H3K27Ac peaks were observed spread throughout the 3′ end of IL1RAPL1 in the SETDB1-KO clones, with the most prominent peak in vicinity to the strongest H3K4me2 peak (Fig. 4). Therefore, we focused our search for regulatory elements on this region. SETDB1-KO clone is associated with H3K4me2 peaks aligned with RPE1 H3K9me3 peaks that were substantially reduced in the mutant clones (Fig. 6a). The major gain of H3K27Ac centered upon a DNaseI hypersensitive site (DHS); regions typically associated with regulatory elements throughout the genome . Within the DNA underlying the H3K27Ac peak was a highly conserved 600 bp sequence. We tested this and a larger sequence underlying the major H3K27Ac peak for enhancer activity in vitro. We observed that the core conserved sequence possessed enhancer activity comparable to the well-characterized and potent SV40 viral enhancer, whereas activity associated with the longer DNA fragment was significantly higher (Fig. 6b), supporting this sequence as a powerful enhancer element.
The enhancer is located downstream of expressed SNPs A and B and upstream of expressed SNPs C and D. Therefore, we sought to determine where this transcript originates through RNA-Seq. To ensure we did not bias toward poly-adenylated mRNA, we resorted to rRNA-depleted strand-specific total RNA-Seq. Through this approach, we identified a sense and antisense transcript originating in the vicinity of the newly identified enhancer element, extending approximately 295 kb in the sense direction and 118 kb antisense, both of which are more prominent in the SETDB1-KO clones (Fig. 6c). Close examination of the most 5′ reads of each transcript revealed that they emanate approximately 80 bp apart and originate within an ERVL-MaLR retrotransposon long terminal repeat (LTR) (Fig. 6d), consistent with promoter activity associated with these elements  and their silencing through the activity of SETDB1 [46,47,48]. The RNA-Seq profiles indicate that both transcripts appear to be spliced, which is confirmed through the generation of Sashimi plots, that allow quantitative visualization of spliced isoforms of transcripts . The forward transcript predominantly incorporates the last 6 exons (exons 6–11) of the full-length IL1RAPL1 gene, along with a novel first exon (Fig. 6e, top panel). In contrast, all exons associated with the antisense transcript are novel and exon usage is more variable (Fig. 6e, bottom panel). To validate the existence of the novel first exon of the sense transcript and the antisense transcripts, RT-PCR was performed between these exons and downstream exons, generating products of the expected size (Data not shown). The ERVL-MaLR element from within which both first exons originate is located approximately 2 kb proximal to the defined enhancer element (Fig. 6a). To confirm bidirectional promoter activity of the ERVL-MaLR element, it was cloned in both orientations upstream of a promoterless luciferase reporter gene. Activity was slightly higher in the forward orientation when compared to the reverse (Fig. 6f), consistent with the forward transcript being detected at higher levels than the reverse transcript in RPE1 cells (Fig. 6c, e).
Loss of the ERVL-MaLR promoter and associated enhancer from the Xa decompacts the Xi
These data indicate that loss of SETDB1 results in the derepression of the Xi enhancer and bidirectional promoter embedded within the 3′ end of IL1RAPL1, coupled with loss of H3K9me3 and gain of H3K4me2 throughout the extent of the two novel transcripts. Given the dramatic changes that are occurring at this interval, could the reactivation of this powerful enhancer be at least in part responsible for the Xi decompaction phenotype observed in the SETDB1-KO clones? To test this, we used a pair of active guide RNAs (gRNAs) flanking the enhancer and bidirectional promoter with the RNA-guided Cas9 nuclease in an attempt to delete the interval . Numerous clones were isolated in which the desired interval was removed, and assignment of the deletion to the Xa or Xi was achieved by FISH (Additional file 7). PCR coupled with sequencing was performed across each flanking gRNA site on the intact allele to ensure that extensive damage had not occurred in the absence of deletion and in those where this was observed, they were excluded from further analysis (Data not shown).
To further characterize these mutants, we initially assessed expression levels of IL1RAPL1 from the 5′ and 3′ ends by qRT-PCR. Interestingly, loss of the enhancer element from the Xa resulted in compete loss of 5′ transcript that initiates transcription from a promoter located greater than 1 Mb upstream. This indicates that transcription from the 5′ promoter is dependent upon the enhancer element. Interestingly, loss of the enhancer element from the Xi resulted in an increase in expression from the 5′ end that surprisingly corresponds to upregulation from the Xa in trans (see below). With the exception of one Xa enhancer mutant, expression from the 3′ end decreased, regardless of whether the enhancer was deleted from the Xa or Xi (Fig. 7a). In order to determine the predominant origins of the 3′ transcripts, cDNA isolated from the mutants was genotyped for two of the SNPs. As expected, only the Xa SNP could be detected in 3′ transcripts from Xi deletion mutants. However, surprisingly the 3′ transcripts detected in Xa enhancer mutants only showed the Xi allele, suggesting that, like the SETDB1-KO clones, the Xi enhancer and bidirectional promoter were active in these clones (Additional file 7). If the Xi enhancer was indeed activated in these clones, we might expect to see some degree of decompaction of the Xi, mimicking the SETDB1-KO phenotype. Staining of enhancer mutant cells for H3K27me3 showed that the Xi territory was not obviously different in the Xi enhancer mutants but was noticeably larger in clones lacking the enhancer from the Xa (Fig. 7b). Subsequent volume measurements of the Xi in these clones confirmed that loss of the enhancer from the Xa, but not Xi, resulted in a significant decompaction of the Xi territory (Fig. 7c). Collectively, these data reveal complex cis and trans effects upon deletion of the enhancer interval.
SETDB1 loss in human cells does not result in chromosome-wide changes to H3K9me3 bands along the Xi, although a role in establishing these territories during XCI similar to what has been described in mouse cannot be ruled out . However, testing XCI onset questions in human cells in vitro faces many technical challenges . Which HMTase is responsible for maintenance of H3K9me3 at the human Xi remains an open question, although functional redundancy between this group of enzymes remains a possibility. Nevertheless, we find that SETDB1 loss does result in a striking Xi decompaction phenotype based on H3K27me3 volume measurements. The overall distribution of H3K27me3 at the Xi did not change, ruling out spread of this modification beyond its normal sites of occupancy, and therefore decompaction may reflect changes to the interchromatin compartment organization at the Xi . To our knowledge, the only other report of Xi decompaction involves knockdown of the heterochromatin proteins SMCHD1 and LRIF1 . Whether SETDB1 is acting in the same pathway as these proteins has yet to be determined.
Alongside the decompaction phenotype, we observed that loss of SETDB1 triggered a large-scale chromatin state transition on the Xi within an approximately 500 kb interval located in the 3′ end of the IL1RAPL1 gene. H3K9me3 was lost coupled with gain of H3K4me2 and broad acquisition of H3K27Ac throughout the interval. The highest peaks of H3K27Ac and H3K4me2 reside near the center of the chromatin change interval, and the DNA underlying these peaks correspond to a powerful enhancer adjacent to an ERVL-MaLR element that promotes bidirectional transcription. While transcription in the reverse direction produces a novel long noncoding RNA (lncRNA), the forward transcript has the potential to generate a protein isoform of IL1RAPL1 that lacks part of the N-terminus. Both transcripts are abundantly transcribed from the Xi in SETDB1-KO clones and appear interspersed with the XIST cloud. Given the central role of SETDB1 in silencing endogenous retroviral elements [46,47,48], we interpret these data to indicate that under normal circumstances, SETDB1 is recruited to the ERVL-MaLR element at the Xi and facilitates heterochromatin formation and maintenance, but in its absence H3K9me3 is lost permitting reactivation of the LTR and adjacent enhancer driving escape from XCI. In contrast, the Xa allele is unlikely to be repressed by SETDB1 as the enhancer is essential to permit transcription of IL1RAPL1 from the promoter located at the 5′ end of the gene.
Interestingly, mutations in or loss of SETDB1 have been reported in cancer [54, 55]. Based on our data, we would predict that full-length IL1RAPL1 would be downregulated, which is indeed the case in brain tumors . Notably, no other regions of the Xi showed such chromatin instability, while only speculating, it has not escaped our notice that this same interval is embedded within FRAXC, a common fragile site on the X , indicating that it is also a region of genomic instability. Mutation or loss of IL1RAPL1 results in intellectual disability  and the unstable chromatin transition interval is almost always lost or rearranged in patients [36, 56,57,58,59,60,61], suggesting that the two may be mechanistically linked. The DNA sequence of FRAXC does not hold clues as to why this region is fragile, but perhaps its chromatin state might. Furthermore, IL1RAPL1 genomic instability has been implicated in numerous other neurological and neuropsychiatric disorders including startle epilepsy , autism spectrum disorder [37, 63] and schizophrenia . The link between SETDB1 and neurological disorders extends beyond what is described here for IL1RAPL1, as neuronal ablation of SETDB1/Setdb1 results in heterochromatin loss and disrupted expression at the protocadherin cluster .
The reactivation of the powerful enhancer coupled with adjacent bidirectional expression on the Xi upon SETDB1 loss raised the possibility that this could be mechanistically linked to the Xi decompaction phenotype. Deletion of the enhancer from the Xi in the absence of SETDB1 mutation did not result in Xi decompaction, but deletion of the enhancer from the Xa did, which was coupled with detection of 3′ bidirectional transcripts from the Xi only. How this trans-chromosomal effect is mediated is unclear but was not a phenomenon restricted to the Xa deletion impacting the Xi, because cells with the enhancer deleted from the Xi showed increased expression on the Xa from the 5′ end of the gene. A summary of our findings is outlined in Fig. 8. In parental cells (top panel), IL1RAPL1 expression is almost exclusively originating from the Xa, both from the 5′ promoter and the bidirectional ERVL-MaLR promoter. The adjacent enhancer element promotes expression of the 5′ transcript in cis. Upon loss of SETDB1 (second panel), local heterochromatin around the enhancer and adjacent bidirectional promoter are lost at the Xi resulting in activation of the enhancer and 3′ transcription. Heterochromatin loss does not extend sufficiently far to permit activation of the Xi 5′ promoter. The enhancer and ERVL-MaLR reactivation is coupled with dramatic decompaction of the Xi territory by unknown mechanisms. Deletion of the bidirectional promoter and enhancer from the Xa (third panel) results in loss of cis-mediated activation of the 5′ promoter coupled with inappropriate activation of the Xi bidirectional promoter as well as substantial decompaction of the Xi territory. In contrast, loss of the enhancer and bidirectional promoter from the Xi (bottom panel) does not impact Xi compaction, but does result in a significant increase in expression from the 5′ promoter on the Xa coupled with reduced 3′ transcription. How these trans-allele effects are mediated is unclear. An attractive candidate are the transcripts generated from the 3′ end, especially the antisense lncRNA, as trans-induction effects of enhancer-associated lncRNA have been reported [66, 67]. One possibility may be posttranscriptional regulation of the 5′ transcript, as the levels of antisense lncRNA appear to be indirectly correlated with 5′ derived transcript levels. To decipher exactly what the underlying mechanisms are is deserving of further investigation as is exploring this novel enhancer element in the context of neuronal function. While we recognize that the decompaction of the Xi in the Xa enhancer deletion mutants is not as extensive as observed in the SETDB1-KO clones, it is a major contributor to the decompaction phenotype. What other factors are involved as well as how and why the Xi decompacts remain to be determined.
Collectively we reveal a novel critical function for SETDB1 in ensuring the proper compaction of the human Xi chromosome territory through the silencing and seeding of heterochromatin at an ERVL-MaLR LTR and adjacent enhancer in the 3′ end of the IL1RAPL1 locus on the Xi allele. Through targeted deletion of the ERVL-MaLR element and enhancer, we reveal unexpected cis and trans effects impacting chromosome compaction and transcription of IL1RAPL1 isoforms. In light of these new data, further investigation of these findings in the context of genomic instability, neurological disorders and expression changes in brain tumors is warranted.
hTERT-RPE1 (RPE1), a female telomerase-immortalized human retinal pigment epithelial cell line, was obtained from Clontech (C4000-1). This product is no longer available through Clontech but can be obtained directly through the American Type Culture Collection (ATCC). Human female embryonic kidney cell line 293 (CRL-1573) was obtained from ATCC. Cells were maintained according to the supplier recommendations. Transfection of plasmid DNA into 293 cells was performed using Lipofectamine 3000 (Cat. No. L3000008) according to the supplier instructions (ThermoFisher Scientific). TALEN expression plasmids and targeting constructs were introduced into RPE1 cells using a 4D-Nucleofector (Lonza) using SF Cell Line 4D-Nucleofector reagent (Cat. No. V4XC-2024), as were gRNA/Cas9 expression constructs.
TALEN and gRNA/Cas9 targeting
TALEN pairs previously reported to actively cut the human SETDB1 locus were assembled using the FLASH procedure essentially as described . Activity of the TALENs was validated using the Surveyor assay (Transgenomic) . The homology-mediated repair promoterless neomycin trap construct was generated by four-way cloning of a left and right homology arm fragment with the pSEPT vector into pAAV [22, 69]. The left homology arm was generated by PCR of a 1217 bp genomic fragment proximal to SETDB1 exon-2 incorporating a NotI site at the most distal edge and a XbaI site at the proximal edge. The right homology arm was generated by PCR of a 785 bp genomic fragment distal to SETDB1 exon-2 incorporating a EcoRI site at the most proximal edge and a NotI site at the distal edge. Restriction enzyme sites were introduced into the PCR products by including the recognition sequences at the 5′ end of the oligonucleotide design. Homology arm PCR fragments were TA cloned into pCR2.1 (ThermoFisher Scientific), and clones lacking mutations were selected. Homology arm inserts were excised with XbaI-NotI or EcoRI-NotI, respectively, and gel purified along with gel purification of the XbaI-EcoRI pSEPT neomycin fragment. These fragments were mixed with NotI-cut phosphatase-treated pAAV and ligated for 1 h at room temperature before transformation into competent DH10B before plating on ampicillin-containing LB agar plates. Transfection-grade plasmid DNA was isolated from a positive clone and linearized with SmaI before introduction alongside TALEN constructs into 1 million RPE1 cells by Nucleofection. Twenty-four hours later, the cells were manually seeded to four 96-well plates and allowed to attach overnight before supplementing the media with neomycin (580 ng/μl). Three to four weeks later, colonies were expanded and genomic DNA isolated. The DNA was used in two initial rounds of PCR (Additional files 1 and 2). The first PCR used a forward primer located proximal to the left homology arm and a reverse primer located in pSEPT. The second PCR used a forward primer located in pSEPT and a reverse primer located distal to the right homology arm. Successfully targeted clones were positive to both of these PCRs and were subjected to a third PCR. The third PCR amplified a 269 bp fragment spanning the TALEN cut sites. Samples negative for this PCR (but positive for an unrelated PCR of similar size) are interpreted as successfully targeted at both alleles. Those clones positive for this PCR were repeated and the product sequenced to determine whether any mutations from non-homologous end joining had been introduced at the cut site.
Sequences flanking the putative IL1RAPL1 enhancer core were used to identify suitable gRNAs using the Optimized CRISPR Design (http://crispr.mit.edu) and cloned into pSpCas9(BB)-2A-GFP (pX458) as described . Paired combinations of gRNA constructs capable of excising the intervening sequence were identified by co-transfection experiments into 293 cells followed by isolation of genomic DNA using the NucleoSpin Tissue kit from Macherey–Nagel (Cat. No. 740952). Genomic DNA was used to perform PCR across the interval to determine which combination of gRNAs was most efficient at generating the desired deletion. Transfection-grade plasmid DNA was isolated for the desired pair of gRNA expression constructs (Qiagen, Cat. No. 12945) and was introduced into RPE1 cells by Nucleofection. Seventy-two hours later, single GFP positive cells were directly sorted into single wells of four 96-well plates using a BD FACSAria SORP flow cytometer. Colonies were expanded 3–4 weeks later and assessed for the presence or absence of the desired deletion by PCR. Assignment of the deletion to the Xa or Xi was performed by hybridizing a probe contained within the deleted region onto dropped metaphase chromosomes (Additional file 7). The Xa can be cytologically distinguished from the Xi due to an X:10 translocation at Xq28 on the Xa making this chromosome substantially longer than the Xi. The karyotypically normal X is the Xi in all RPE1 cells .
Immunofluorescence on interphase cells and metaphase chromosomes
Indirect immunofluorescence on interphase cells was performed essentially as described previously  and on metaphase chromosomes . Direct labeling of primary antibodies was achieved using the Zenon Antibody Labeling Kit from ThermoFisher Scientific according to the supplied instructions (Cat. No. Z2305).
DNA and RNA FISH on interphase cells and metaphase chromosomes
Dropped metaphase chromosome spreads and subsequent DNA FISH were performed essentially as described . Direct-labeled fluorescent probes were prepared using the Nick Translation DNA Labeling System from Enzo Lifesciences (Cat. No. ENZ-42910) with fluorescent deoxynucleotides Spectrum Orange and Spectrum Green (Abbott Molecular, Cat. Nos. 02N32-050 and 02N33-050). RNA FISH was performed as described previously . The identity of BAC clones used for FISH is given in Additional file 8.
Rabbit polyclonal antibodies to histone H3 trimethylated at lysine 27 were obtained from EMD Millipore (Cat. No. 07-449), as were rabbit polyclonal antibodies to histone H3 trimethylated at lysine 9 (Cat. No. 07-523), histone H3 dimethylated at lysine 4 (07-0030), anti-acetyl-lysine (06-933) and mouse monoclonal antibodies to HP1β (Cat. No. MAB3448). Alexa-Fluor-conjugated secondary antibodies were obtained from ThermoFisher Scientific. Rabbit polyclonal antibodies to SMCHD1 were obtained from Bethyl Laboratories Inc. (Cat. No. A302-872A). Rabbit antibodies to β-actin were obtained from Cell Signaling Technology (Cat. No. 4970). Rabbit polyclonal antibodies to SETDB1 were obtained from Cell Applications Inc. (Cat. No. CY1112).
Protein extracts, polyacrylamide gel electrophoresis, Western blotting and detection were carried out as described previously .
Quantitative RT-PCR analysis and standard PCR
All qRT-PCR was performed on a CFX96 (Bio-Rad) using an EvaGreen 2X qPCR mastermix (ABM, Cat. No. Mastermix-S) as described previously . Standard endpoint PCR analysis used HotStar Taq Plus (Qiagen) according to the supplier recommendation (Cat. No. 203603). All oligonucleotides were obtained from Eurofins Genomics and are given in Additional file 6.
ChIP-Seq to H3K4me2, H3K27Ac and H3K9me3 was performed through the full-service procedure provided by Zymo Research according to their established protocols. This included the ChIP assay, library preparation, Next-Gen 50 bp single-end sequencing, bioinformatics and all quality control steps. Three independent frozen pellets of 5 million formaldehyde cross-linked cells for each sample were provided to Zymo Research for the ChIP procedure. In brief, cells were cross-linked with formaldehyde at 1% final concentration for 7 min at room temperature. ChIP assays were conducted using the Zymo-Spin ChIP kit (Zymo Research Corp., Cat. No. D5210) following the manufacturer’s instructions. Sonication was performed at high power setting for 40 cycles (30 s on, 30 s off) using a Bioruptor Plus (Diagenode Inc., Denville, NJ), yielding a modal fragment size of < 600 bp. Antibodies used in ChIP assays included: anti-H3K4me2 (Abcam ab7766), anti-H3K9me3 (Abcam ab8898), anti-H3K27ac (Abcam ab4729) and normal rabbit IgG (Millipore 12-370 or Diagenode C15410206). Approximately 10 µg of chromatin from RPE1 or SETDB1 cells was used in each ChIP assay with 4 µg of antibodies. IgG negative control was included with each assay. DNA libraries were prepared by Zymo Research Epigenetics Services and were sequenced on a HiSeq sequencer. ChIP-Seq reads were aligned to human reference genome GRCh37/hg19 by Bowtie  with at most two mismatches. Reads that appeared more than twice at the same position on the same strand were discarded to remove PCR duplication. WIG files were generated from the coverage for visualization purposes. MACS2  was used to identify target peaks at a q-value cutoff 0.01 using narrow peak for H3K4me2 and H3K27ac and broad peak setting for H3K9me3 using normalized mapped sequencing reads. In addition, target peaks overlapping by more than 50% were considered “common” to both samples; otherwise, both of these two peaks would be considered “unique.”
RNA-Seq was performed through the services provided by Novogene. Triplicate total RNA extracts for each clone were prepared using the Nucleospin RNA Plus kit from Macherey–Nagel (Cat. No. 740984). For each sample, 6 μg of total RNA was provided to Novogene who then performed quality control, removed rRNA and prepared strand-specific libraries before generating at least 60 million 150 bp paired-end reads per sample. Adapter sequences were removed using Cutadapt ; Fastq stranded data files were mapped to the plus or minus strand of human genome build hg38 using HISAT2 . SAM files were converted to BAM files using SAMtools  and BAM files were converted to bedGraph files using BEDTools  before conversion to bigWig format for viewing on the UCSC Genome Browser (https://genome.ucsc.edu/index.html). Sashimi plots were generated using the function provided by the Integrative Genomics Viewer (IGV_2.3.97).
All Sanger sequencing was performed using the services provided by Eurofins Genomics, and sequences were edited and visualized using Sequencher 5.4.6 (Gene Codes Corporation).
Luciferase promoter and enhancer assays
A DNA fragment of 810 bp encompassing the core conserved putative enhancer region of IL1RAPL1 and a larger fragment of 2613 bp were amplified with primers that incorporate a 5′ SalI and 3′ BamHI site before cloning into pMiniT2.0 (NEB, Cat. No. E1202S). Clones were verified to be free of PCR-induced mutations before subcloning into the SalI-BamHI sites of pGL4.23 (Promega, Cat. No. E8411) downstream of the luciferase expression cassette. As an enhancer control, the SV40 enhancer fragment of pGL3.control (Promega, Cat. No. E1741) was excised with XbaI and BamHI and subcloned into XbaI-BamHI cut pGl4.23. A DNA fragment of 529 bp encompassing the ERVL putative promoter element was amplified and cloned into pMiniT2.0. Clones were verified to be free of mutations by sequencing, and the insert was excised using XhoI and subcloned into XhoI cut and de-phosphorylated pGL4.10 (Promega, Cat. No. E6651). Clones were isolated that contained the ERVL element in either orientation. Dual luciferase assays were carried out as described previously . Empty vectors served as negative controls, whereas the SV40 enhancer construct served as a positive control for the enhancer assay and a previously characterized promoter construct for the DANT2 lncRNA  served as a promoter positive control.
Bacterial artificial chromosomes
All BAC clones were obtained from ThermoFisher Scientific. Clones were cultured according to the supplier recommendations and DNA isolated using the NucleoBond Xtra BAC isolation kit from Macherey–Nagel (Cat. No. 740436). BAC clone information is given in Additional file 8.
Image acquisition and volume measurements
Images were collected on a Delta Vision pDV. Images were de-convolved with softWoRx 6.5.2 (GE Healthcare) and compiled into images using Adobe Photoshop CC 2018 (Adobe Systems). For nuclear volume, de-convolved D3D files were used with Model-2D polygon finder, selecting a rectangle box around the DAPI image with a minimum perimeter setting of 300. 3D object builder was used to generate 3D objects followed by the Measurements function to generate a table of 3D measurements. H3K27me3 Xi volumes were measured as above setting the minimum perimeter to 30. The Xi to DAPI ratio was calculated in Microsoft Excel before importing into JMP pro 12 for statistical analysis of volume measurement. Typically, 40 nuclei are assessed for each sample.
Unpaired t tests were performed using the QuickCalcs function in GraphPad software. JMP Pro 12 was used for the statistical analysis of Xi volume measurements and luciferase assay data. Means of all pairs were compared using the Tukey’s honest significance test.
bacterial artificial chromosomes
chromatin immunoprecipitation coupled with high-throughput sequencing
DNase I hypersensitive site
enhancer of Zeste 2
fluorescent in situ hybridization
fast ligation-based automatable solid-phase high-throughput system
common fragile site on the X chromosome site-C
histone H3 dimethylated lysine 2
histone H3 trimethylated at lysine 9
histone H3 acetylated at lysine 27
histone H3 trimethylated at lysine 27
heterochromatin protein 1 beta
interleukin 1 receptor accessory protein-like 1
long noncoding RNA
long terminal repeat
quantitative reverse transcription PCR
reverse transcription PCR
retinal pigment epithelial cells
SET domain bifurcated 1
single nucleotide polymorphism
structural maintenance of chromosomes flexible hinge domain containing 1
transcription activator-like effector nuclease
active X chromosomes
X chromosome inactivation
inactive X chromosome
X inactive specific transcript
Lyon MF. Gene action in the X-chromosome of the mouse (Mus musculus L.). Nature. 1961;190:372–3.
Boggs BA, Cheung P, Heard E, Spector DL, Chinault AC, Allis CD. Differentially methylated forms of histone H3 show unique association patterns with inactive human X chromosomes. Nat Genet. 2002;30:73–6.
Peters AH, Mermoud JE, O’Carroll D, Pagani M, Schweizer D, Brockdorff N, Jenuwein T. Histone H3 lysine 9 methylation is an epigenetic imprint of facultative heterochromatin. Nat Genet. 2002;30:77–80.
Plath K, Fang J, Mlynarczyk-Evans SK, Cao R, Worringer KA, Wang H, de la Cruz CC, Otte AP, Panning B, Zhang Y. Role of histone H3 lysine 27 methylation in X inactivation. Science. 2003;300:131–5.
Silva J, Mak W, Zvetkova I, Appanah R, Nesterova TB, Webster Z, Peters AH, Jenuwein T, Otte AP, Brockdorff N. Establishment of histone h3 methylation on the inactive X chromosome requires transient recruitment of eed-enx1 polycomb group complexes. Dev Cell. 2003;4:481–95.
Chadwick BP, Willard HF. Multiple spatially distinct types of facultative heterochromatin on the human inactive X chromosome. Proc Natl Acad Sci USA. 2004;101:17450–5.
Keniry A, Gearing LJ, Jansz N, Liu J, Holik AZ, Hickey PF, Kinkel SA, Moore DL, Breslin K, Chen K, et al. Setdb1-mediated H3K9 methylation is enriched on the inactive X and plays a role in its epigenetic silencing. Epigenet Chromatin. 2016;9:16.
Shevchenko AI, Pavlova SV, Dementyeva EV, Zakian SM. Mosaic heterochromatin of the inactive X chromosome in vole Microtus rossiaemeridionalis. Mamm Genome. 2009;20:644–53.
Chadwick BP. Variation in Xi chromatin organization and correlation of the H3K27me3 chromatin territories to transcribed sequences by microarray analysis. Chromosoma. 2007;116:147–57.
Cao R, Wang L, Wang H, Xia L, Erdjument-Bromage H, Tempst P, Jones RS, Zhang Y. Role of histone H3 lysine 27 methylation in Polycomb-group silencing. Science. 2002;298:1039–43.
Czermin B, Melfi R, McCabe D, Seitz V, Imhof A, Pirrotta V. Drosophila enhancer of Zeste/ESC complexes have a histone H3 methyltransferase activity that marks chromosomal Polycomb sites. Cell. 2002;111:185–96.
Kuzmichev A, Nishioka K, Erdjument-Bromage H, Tempst P, Reinberg D. Histone methyltransferase activity associated with a human multiprotein complex containing the Enhancer of Zeste protein. Genes Dev. 2002;16:2893–905.
Muller J, Hart CM, Francis NJ, Vargas ML, Sengupta A, Wild B, Miller EL, O’Connor MB, Kingston RE, Simon JA. Histone methyltransferase activity of a Drosophila Polycomb group repressor complex. Cell. 2002;111:197–208.
Ohhata T, Tachibana M, Tada M, Tada T, Sasaki H, Shinkai Y, Sado T. X-inactivation is stably maintained in mouse embryos deficient for histone methyl transferase G9a. Genesis. 2004;40:151–6.
Peters AH, O’Carroll D, Scherthan H, Mechtler K, Sauer S, Schofer C, Weipoltshammer K, Pagani M, Lachner M, Kohlmaier A, et al. Loss of the Suv39h histone methyltransferases impairs mammalian heterochromatin and genome stability. Cell. 2001;107:323–37.
Schultz DC, Ayyanathan K, Negorev D, Maul GG, Rauscher FJ 3rd. SETDB1: a novel KAP-1-associated histone H3, lysine 9-specific methyltransferase that contributes to HP1-mediated silencing of euchromatic genes by KRAB zinc-finger proteins. Genes Dev. 2002;16:919–32.
Yang L, Xia L, Wu DY, Wang H, Chansky HA, Schubach WH, Hickstein DD, Zhang Y. Molecular cloning of ESET, a novel histone H3-specific methyltransferase that interacts with ERG transcription factor. Oncogene. 2002;21:148–52.
Minkovsky A, Sahakyan A, Rankin-Gee E, Bonora G, Patel S, Plath K. The Mbd1-Atf7ip-Setdb1 pathway contributes to the maintenance of X chromosome inactivation. Epigenet Chromatin. 2014;7:12.
Shevchenko AI, Grigor’eva EV, Medvedev SP, Zakharova IS, Dementyeva EV, Elisaphenko EA, Malakhova AA, Pavlova SV, Zakian SM. Impact of Xist RNA on chromatin modifications and transcriptional silencing maintenance at different stages of imprinted X chromosome inactivation in vole Microtus levis. Chromosoma. 2018;127:129–39.
Minajigi A, Froberg JE, Wei C, Sunwoo H, Kesner B, Colognori D, Lessing D, Payer B, Boukhali M, Haas W, Lee JT. A comprehensive Xist interactome reveals cohesin repulsion and an RNA-directed chromosome conformation. Science. 2015. https://doi.org/10.1126/science.aab2276.
Reyon D, Tsai SQ, Khayter C, Foden JA, Sander JD, Joung JK. FLASH assembly of TALENs for high-throughput genome editing. Nat Biotechnol. 2012;30:460–5.
Topaloglu O, Hurley PJ, Yildirim O, Civin CI, Bunz F. Improved methods for the generation of human gene knockout and knockin cell lines. Nucleic Acids Res. 2005;33:e158.
Chadwick BP, Willard HF. Cell cycle-dependent localization of macroH2A in chromatin of the inactive X chromosome. J Cell Biol. 2002;157:1113–23.
Chadwick BP. DXZ4 chromatin adopts an opposing conformation to that of the surrounding chromosome and acquires a novel inactive X-specific role involving CTCF and antisense transcripts. Genome Res. 2008;18:1259–69.
Horakova AH, Moseley SC, McLaughlin CR, Tremblay DC, Chadwick BP. The macrosatellite DXZ4 mediates CTCF-dependent long-range intrachromosomal interactions on the human inactive X chromosome. Hum Mol Genet. 2012;21(20):4367–77.
Rao SS, Huntley MH, Durand NC, Stamenova EK, Bochkov ID, Robinson JT, Sanborn AL, Machol I, Omer AD, Lander ES, Aiden EL. A 3D map of the human genome at kilobase resolution reveals principles of chromatin looping. Cell. 2014;159:1665–80.
Tang Z, Luo OJ, Li X, Zheng M, Zhu JJ, Szalaj P, Trzaskoma P, Magalska A, Wlodarczyk J, Ruszczycki B, et al. CTCF-mediated human 3D genome architecture reveals chromatin topology for transcription. Cell. 2015;163:1611–27.
Blewitt ME, Gendrel AV, Pang Z, Sparrow DB, Whitelaw N, Craig JM, Apedaile A, Hilton DJ, Dunwoodie SL, Brockdorff N, et al. SmcHD1, containing a structural-maintenance-of-chromosomes hinge domain, has a critical role in X inactivation. Nat Genet. 2008;40:663–9.
Jeppesen P, Turner BM. The inactive X chromosome in female mammals is distinguished by a lack of histone H4 acetylation, a cytogenetic marker for gene expression. Cell. 1993;74:281–9.
Chadwick BP, Willard HF. Chromatin of the Barr body: histone and non-histone proteins associated with or excluded from the inactive X chromosome. Hum Mol Genet. 2003;12:2167–78.
Montani C, Ramos-Brossier M, Ponzoni L, Gritti L, Cwetsch AW, Braida D, Saillour Y, Terragni B, Mantegazza M, Sala M, et al. The X-linked intellectual disability protein IL1RAPL1 regulates dendrite complexity. J Neurosci. 2017;37:6606–27.
Pavlowsky A, Gianfelice A, Pallotto M, Zanchi A, Vara H, Khelfaoui M, Valnegri P, Rezai X, Bassani S, Brambilla D, et al. A postsynaptic signaling pathway that may account for the cognitive defect due to IL1RAPL1 mutation. Curr Biol. 2010;20:103–15.
Ramos-Brossier M, Montani C, Lebrun N, Gritti L, Martin C, Seminatore-Nole C, Toussaint A, Moreno S, Poirier K, Dorseuil O, et al. Novel IL1RAPL1 mutations associated with intellectual disability impair synaptogenesis. Hum Mol Genet. 2015;24:1106–18.
Valnegri P, Montrasio C, Brambilla D, Ko J, Passafaro M, Sala C. The X-linked intellectual disability protein IL1RAPL1 regulates excitatory synapse formation by binding PTPdelta and RhoGAP2. Hum Mol Genet. 2011;20:4797–809.
Wendt KS, Yoshida K, Itoh T, Bando M, Koch B, Schirghuber E, Tsutsumi S, Nagae G, Ishihara K, Mishiro T, et al. Cohesin mediates transcriptional insulation by CCCTC-binding factor. Nature. 2008;451:796–801.
Carrie A, Jun L, Bienvenu T, Vinet MC, McDonell N, Couvert P, Zemni R, Cardona A, Van Buggenhout G, Frints S, et al. A new member of the IL-1 receptor family highly expressed in hippocampus and involved in X-linked mental retardation. Nat Genet. 1999;23:25–31.
Piton A, Gauthier J, Hamdan FF, Lafreniere RG, Yang Y, Henrion E, Laurent S, Noreau A, Thibodeau P, Karemera L, et al. Systematic resequencing of X-chromosome synaptic genes in autism spectrum disorder and schizophrenia. Mol Psychiatry. 2011;16:867–80.
McAvoy S, Ganapathiraju S, Perez DS, James CD, Smith DI. DMD and IL1RAPL1: two large adjacent genes localized within a common fragile site (FRAXC) have reduced expression in cultured brain tumors. Cytogenet Genome Res. 2007;119:196–203.
Durkin SG, Glover TW. Chromosome fragile sites. Annu Rev Genet. 2007;41:169–92.
Darrow EM, Huntley MH, Dudchenko O, Stamenova EK, Durand NC, Sun Z, Huang SC, Sanborn AL, Machol I, Shamim M, et al. Deletion of DXZ4 on the human inactive X chromosome alters higher-order genome architecture. Proc Natl Acad Sci USA. 2016;113:E4504–12.
Bonn S, Zinzen RP, Girardot C, Gustafson EH, Perez-Gonzalez A, Delhomme N, Ghavi-Helm Y, Wilczynski B, Riddell A, Furlong EE. Tissue-specific analysis of chromatin state identifies temporal signatures of enhancer activity during embryonic development. Nat Genet. 2012;44:148–56.
Heintzman ND, Stuart RK, Hon G, Fu Y, Ching CW, Hawkins RD, Barrera LO, Van Calcar S, Qu C, Ching KA, et al. Distinct and predictive chromatin signatures of transcriptional promoters and enhancers in the human genome. Nat Genet. 2007;39:311–8.
Koch CM, Andrews RM, Flicek P, Dillon SC, Karaoz U, Clelland GK, Wilcox S, Beare DM, Fowler JC, Couttet P, et al. The landscape of histone modifications across 1% of the human genome in five human cell lines. Genome Res. 2007;17:691–707.
Sheffield NC, Thurman RE, Song L, Safi A, Stamatoyannopoulos JA, Lenhard B, Crawford GE, Furey TS. Patterns of regulatory activity across diverse human cell types predict tissue identity, transcription factor binding, and long-range interactions. Genome Res. 2013;23:777–88.
Cohen CJ, Lock WM, Mager DL. Endogenous retroviral LTRs as promoters for human genes: a critical assessment. Gene. 2009;448:105–14.
Karimi MM, Goyal P, Maksakova IA, Bilenky M, Leung D, Tang JX, Shinkai Y, Mager DL, Jones S, Hirst M, Lorincz MC. DNA methylation and SETDB1/H3K9me3 regulate predominantly distinct sets of genes, retroelements, and chimeric transcripts in mESCs. Cell Stem Cell. 2011;8:676–87.
Maksakova IA, Goyal P, Bullwinkel J, Brown JP, Bilenky M, Mager DL, Singh PB, Lorincz MC. H3K9me3-binding proteins are dispensable for SETDB1/H3K9me3-dependent retroviral silencing. Epigenet Chromatin. 2011;4:12.
Matsui T, Leung D, Miyashita H, Maksakova IA, Miyachi H, Kimura H, Tachibana M, Lorincz MC, Shinkai Y. Proviral silencing in embryonic stem cells requires the histone methyltransferase ESET. Nature. 2010;464:927–31.
Katz Y, Wang ET, Silterra J, Schwartz S, Wong B, Thorvaldsdottir H, Robinson JT, Mesirov JP, Airoldi EM, Burge CB. Quantitative visualization of alternative exon expression from RNA-seq data. Bioinformatics. 2015;31:2400–2.
Ran FA, Hsu PD, Wright J, Agarwala V, Scott DA, Zhang F. Genome engineering using the CRISPR-Cas9 system. Nat Protoc. 2013;8:2281–308.
Sahakyan A, Plath K, Rougeulle C. Regulation of X-chromosome dosage compensation in human: mechanisms and model systems. Philos Trans R Soc Lond B Biol Sci. 2017. https://doi.org/10.1098/rstb.2016.0363.
Smeets D, Markaki Y, Schmid VJ, Kraus F, Tattermusch A, Cerase A, Sterr M, Fiedler S, Demmerle J, Popken J, et al. Three-dimensional super-resolution microscopy of the inactive X chromosome territory reveals a collapse of its active nuclear compartment harboring distinct Xist RNA foci. Epigenet Chromatin. 2014;7:8.
Nozawa RS, Nagao K, Igami KT, Shibata S, Shirai N, Nozaki N, Sado T, Kimura H, Obuse C. Human inactive X chromosome is compacted through a PRC2-independent SMCHD1-HBiX1 pathway. Nat Struct Mol Biol. 2013;20:566–73.
Bueno R, Stawiski EW, Goldstein LD, Durinck S, De Rienzo A, Modrusan Z, Gnad F, Nguyen TT, Jaiswal BS, Chirieac LR, et al. Comprehensive genomic analysis of malignant pleural mesothelioma identifies recurrent mutations, gene fusions and splicing alterations. Nat Genet. 2016;48:407–16.
Kang HC, Kim HK, Lee S, Mendez P, Kim JW, Woodard G, Yoon JH, Jen KY, Fang LT, Jones K, et al. Whole exome and targeted deep sequencing identify genome-wide allelic loss and frequent SETDB1 mutations in malignant pleural mesotheliomas. Oncotarget. 2016;7:8321–31.
Behnecke A, Hinderhofer K, Bartsch O, Numann A, Ipach ML, Damatova N, Haaf T, Dufke A, Riess O, Moog U. Intragenic deletions of IL1RAPL1: report of two cases and review of the literature. Am J Med Genet A. 2011;155A:372–9.
Franek KJ, Butler J, Johnson J, Simensen R, Friez MJ, Bartel F, Moss T, DuPont B, Berry K, Bauman M, et al. Deletion of the immunoglobulin domain of IL1RAPL1 results in nonsyndromic X-linked intellectual disability associated with behavioral problems and mild dysmorphism. Am J Med Genet A. 2011;155A:1109–14.
Laino L, Bottillo I, Piedimonte C, Bernardini L, Torres B, Grammatico B, Bargiacchi S, Mulargia C, Calvani M, Cardona F, et al. Clinical and molecular characterization of a boy with intellectual disability, facial dysmorphism, minor digital anomalies and a complex IL1RAPL1 intragenic rearrangement. Eur J Paediatr Neurol. 2016;20:971–6.
Moyses-Oliveira M, Guilherme RS, Meloni VA, Di Battista A, de Mello CB, Bragagnolo S, Moretti-Ferreira D, Kosyakova N, Liehr T, Carvalheira GM, Melaragno MI. X-linked intellectual disability related genes disrupted by balanced X-autosome translocations. Am J Med Genet B Neuropsychiatr Genet. 2015;168:669–77.
Nawara M, Klapecki J, Borg K, Jurek M, Moreno S, Tryfon J, Bal J, Chelly J, Mazurczak T. Novel mutation of IL1RAPL1 gene in a nonspecific X-linked mental retardation (MRX) family. Am J Med Genet A. 2008;146A:3167–72.
Youngs EL, Henkhaus R, Hellings JA, Butler MG. IL1RAPL1 gene deletion as a cause of X-linked intellectual disability and dysmorphic features. Eur J Med Genet. 2012;55:32–6.
Dinopoulos A, Stefanou MI, Attilakos A, Tsirouda M, Papaevangelou V. A case of startle epilepsy associated with IL1RAPL1 gene deletion. Pediatr Neurol. 2014;51:271–4.
Bhat SS, Ladd S, Grass F, Spence JE, Brasington CK, Simensen RJ, Schwartz CE, Dupont BR, Stevenson RE, Srivastava AK. Disruption of the IL1RAPL1 gene associated with a pericentromeric inversion of the X chromosome in a patient with mental retardation and autism. Clin Genet. 2008;73:94–6.
Melhem N, Middleton F, McFadden K, Klei L, Faraone SV, Vinogradov S, Tiobech J, Yano V, Kuartei S, Roeder K, et al. Copy number variants for schizophrenia and related psychotic disorders in Oceanic Palau: risk and transmission in extended pedigrees. Biol Psychiatry. 2011;70:1115–21.
Jiang Y, Loh YE, Rajarajan P, Hirayama T, Liao W, Kassim BS, Javidfar B, Hartley BJ, Kleofas L, Park RB, et al. The methyltransferase SETDB1 regulates a large neuron-specific topological chromatin domain. Nat Genet. 2017;49:1239–50.
Alvarez-Dominguez JR, Knoll M, Gromatzky AA, Lodish HF. the super-enhancer-derived alncRNA-EC7/bloodlinc potentiates red blood cell development in trans. Cell Rep. 2017;19:2503–14.
Ashe HL, Monks J, Wijgerde M, Fraser P, Proudfoot NJ. Intergenic transcription and transinduction of the human beta-globin locus. Genes Dev. 1997;11:2494–509.
Guschin DY, Waite AJ, Katibah GE, Miller JC, Holmes MC, Rebar EJ. A rapid and general assay for monitoring endogenous gene modification. Methods Mol Biol. 2010;649:247–56.
Rago C, Vogelstein B, Bunz F. Genetic knockouts and knockins in human somatic cells. Nat Protoc. 2007;2:2734–46.
McLaughlin CR, Chadwick BP. Characterization of DXZ4 conservation in primates implies important functional roles for CTCF binding, array expression and tandem repeat organization on the X chromosome. Genome Biol. 2011;12:R37.
Horakova AH, Calabrese JM, McLaughlin CR, Tremblay DC, Magnuson T, Chadwick BP. The mouse DXZ4 homolog retains Ctcf binding and proximity to Pls3 despite substantial organizational differences compared to the primate macrosatellite. Genome Biol. 2012;13:R70.
Culver-Cochran AE, Chadwick BP. Loss of WSTF results in spontaneous fluctuations of heterochromatin formation and resolution, combined with substantial changes to gene expression. BMC Genom. 2013;14:740.
Langmead B, Trapnell C, Pop M, Salzberg SL. Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol. 2009;10:R25.
Zhang Y, Liu T, Meyer CA, Eeckhoute J, Johnson DS, Bernstein BE, Nusbaum C, Myers RM, Brown M, Li W, Liu XS. Model-based analysis of ChIP-Seq (MACS). Genome Biol. 2008;9:R137.
Martin M. Cutadapt removes adapter sequences from high-throughput sequencing reads. EMBnet J. 2011;17:10–2.
Kim D, Langmead B, Salzberg SL. HISAT: a fast spliced aligner with low memory requirements. Nat Methods. 2015;12:357–60.
Li H, Handsaker B, Wysoker A, Fennell T, Ruan J, Homer N, Marth G, Abecasis G, Durbin R. Genome project data processing S: the sequence alignment/map format and SAMtools. Bioinformatics. 2009;25:2078–9.
Quinlan AR, Hall IM. BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics. 2010;26:841–2.
Figueroa DM, Darrow EM, Chadwick BP. Two novel DXZ4-associated long noncoding RNAs show developmental changes in expression coincident with heterochromatin formation at the human (Homo sapiens) macrosatellite repeat. Chromosome Res. 2015;23:733–52.
Cermak T, Doyle EL, Christian M, Wang L, Zhang Y, Schmidt C, Baller JA, Somia NV, Bogdanove AJ, Voytas DF. Efficient design and assembly of custom TALEN and other TAL effector-based constructs for DNA targeting. Nucleic Acids Res. 2011;39:e82.
BPC conceived this project; BPC and ZS performed the experiments, analyzed the data, and wrote the manuscript. Both authors read and approved the final manuscript.
We thank R. Didier (Florida State University, College of Medicine) for assistance with flow cytometry; F. Bunz (Johns Hopkins University School of Medicine) for the pSEPT and pAAV vectors; and F. Zhang (Broad Institute of MIT) for the gift of pSpCas9(BB)-2A-GFP (Addgene plasmid # 48138).
The authors ZS and BPC declare that they do not have any competing interests.
Availability of data and materials
The datasets generated during the current study are available through GenBank and GEO. Accession number for the shorter IL1RAPL1 transcript can be obtained through GenBank (Accession Number MH212163) as can the two most common antisense spliced transcripts (Accession Numbers MH212164 and MH212165). All RNA-Seq and ChIP-Seq data are available through GEO (Accession Number GSE113399).
Consent for publication
Ethics approval and consent to participate
This work was supported by National Institute of General Medical Science Grant R01GM117003 (to B.P.C.). The funding agency had no role in the design of the study or collection, analysis, or interpretation of data or writing of the manuscript.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Sun, Z., Chadwick, B.P. Loss of SETDB1 decompacts the inactive X chromosome in part through reactivation of an enhancer in the IL1RAPL1 gene. Epigenetics & Chromatin 11, 45 (2018) doi:10.1186/s13072-018-0218-9
- X chromosome inactivation
- Inactive X chromosome