Regulatory dissection of the CBX5 and hnRNPA1 bi-directional promoter in human breast cancer cells reveals novel transcript variants differentially associated with HP1α down-regulation in metastatic cells
BMC Cancer volume 16, Article number: 32 (2016)
The three members of the human heterochromatin protein 1 (HP1) family of proteins, HP1α, HP1β, and HPγ, are involved in chromatin packing and epigenetic gene regulation. HP1α is encoded from the CBX5 gene and is a suppressor of metastasis. CBX5 is down-regulated at the transcriptional and protein level in metastatic compared to non-metastatic breast cancer. CBX5 shares a bi-directional promoter structure with the hnRNPA1 gene. But whereas CBX5 expression is down-regulated in metastatic cells, hnRNAP1 expression is constant. Here, we address the regulation of CBX5 in human breast cancer.
Transient transfection and transposon mediated integration of dual-reporter mini-genes containing the bi-directional hnRNPA1 and CBX5 promoter was performed to investigate transcriptional regulation in breast cancer cell lines. Bioinformatics and functional analysis were performed to characterize transcriptional events specifically regulating CBX5 expression. TSA treatment and Chromatin Immunoprecipitation (ChIP) were performed to investigate the chromatin structure along CBX5 in breast cancer cells. Finally, expression of hnRNPA1 and CBX5 mRNA isoforms were measured by quantitative reverse transcriptase PCR (qRT-PCR) in breast cancer tissue samples.
We demonstrate that an hnRNPA1 and CBX5 bi-directional core promoter fragment does not comprise intrinsic capacity for specific CBX5 down-regulation in metastatic cells. Characterization of transcriptional events in the 20 kb CBX5 intron 1 revealed existence of several novel CBX5 transcripts. Two of these encode consensus HP1α protein but used autonomous promoters in intron 1 by which HP1α expression could be de-coupled from the bi-directional promoter. In addition, another CBX5 transcriptional isoform, STET, was discovered. This transcript includes CBX5 exon 1 and part of intron 1 sequences but lacks inclusion of HP1α encoding exons. Inverse correlation between STET and HP1α coding CBX5 mRNA expression was observed in breast cancer cell lines and tissue samples from breast cancer patients.
We find that HP1α is down-regulated in a mechanism involving CBX5 promoter downstream sequences and that regulation through alternative polyadenylation and splicing generates a transcript, STET, with potential importance in carcinogenesis.
The heterochromatin protein 1 (HP1) family was first identified in Drosophila melanogaster as essential components of pericentric heterochromatin and shown to be implicated in chromatin compaction and epigenetic repression of gene expression . In mammalian cells, the HP1 family is composed of three distinct genes: CBX5, CBX1, and CBX3 encoding the highly conserved proteins: HP1α, HP1β, and HP1γ [2–5]. The HP1 proteins consist of an N-terminal chromo domain (CD) and a structurally similar C-terminal chromo shadow domain (CSD) separated by a flexible hinge domain [6, 7]. The HP1 proteins have distinct chromatin distributions with HP1α present mainly in heterochromatin, HP1β in both hetero- and euchromatin, and HP1γ primarily located in euchromatin [5, 8, 9]. Tethering HP1 proteins to chromatin through the CD, CSD or heterologous DNA-binding domains results in transcriptional repression in cis [8, 10]. The CD mediates HP1 binding to chromatin through specific interactions with di- and tri-methylated lysine 9 on the H3 histone tail (H3K9me2/3). Furthermore, the affinity for CD binding increases proportionally with the degree of methylation [8, 11, 12]. The CD also interacts with the tail of linker histone H1.4 methylated on lysine 26 which participates in further chromatin compaction . The CSD functions as a HP1 protein-protein dimerization domain forming homo- and hetero-dimers [8, 14, 15]. The CSD dimeric structure is also an interaction platform for additional proteins through the core amino acid sequence PXVXL (X = any amino acid) [14, 15]. Many different types of proteins containing PXVXL motifs have been shown to interact with HP1 proteins through the CSD [4, 5, 16–20]. However, there are proteins that associate with the CSD of HP1 through alternative sequence motifs [10, 21, 22]. Notably, the CSD also interacts with the first helix of the histone fold of H3 to a PXVXL-like motif and this H3 region is involved in chromatin remodeling [23–26]. The hinge region of HP1 contributes to chromatin association through interactions with histone H1 and RNA. Through this interaction, RNA components are thought to be important in the maintenance and localization of HP1 proteins along specific sites at the genome, e.g. for HP1α pericentric heterochromatin localization [8, 27–30]. When HP1 is bound to di- or tri-methylated H3K9 through the CD, subsequent recruitment of SUV39h1 causes adjacent H3K9 residues to become methylated. This creates new binding sites for additional HP1 proteins, which, in turn, will further recruit SUV39h1 proteins. This mechanism explains how HP1 modulates the spread of heterochromatin into neighboring euchromatin, a phenomenon known as position effect variegation (PEV) [31–33]. PEV is suppressed with decreased HP1 expression and enhanced with increased HP1 expression [32, 33].
In breast cancer, the expression level of CBX5 and encoded HP1α correlates with both clinical outcome in terms of patient survival and clinical data in terms of tumor size and stage of this disease . Tumor cells from primary breast carcinomas exhibit higher expression levels of HP1α encoding mRNA and protein compared to normal breast tissue . Moreover, HP1α encoding mRNA and protein have also been shown to be down-regulated in highly invasive breast cancer cell lines (e.g. HS578T and MDA-MB-231) compared to poorly invasive breast cancer cell lines (e.g. T47D and MCF7) while HP1β and HP1γ were relative equally expressed [20, 35–37]. Immunohistochemical analysis of in vivo breast cancer samples showed that HP1α expression was reduced in metastatic cells relative to the primary tumor corroborating the cell line findings . Following RNAi-mediated knockdown of HP1α, poorly invasive MCF7 cells have increased invasive potential. Conversely, highly invasive MDA-MB-231 cells loose invasive potential following ectopic HP1α expression [36, 38]. Based on these data, HP1α is defined as a metastasis suppressor, which in contrast to tumor suppressors is defined as factors being able to suppress metastasis without affecting the growth of the tumor [20, 36, 38, 39].
Analysis of the transcriptional regulation of CBX5 in breast cancer cells have been performed with a resulting mapping of cis-elements and trans-factors [40, 41]. CBX5 is orientated in a “head-to-head” bi-directional arrangement with hnRNPA1. The hnRNPA1 encoded protein belongs to the A/B subfamily of heterogeneous nuclear ribonucleoproteins involved in the packaging of pre-mRNA into hnRNP particles, transport of poly adenylated mRNA from the nucleus to the cytoplasm, and may modulate splice site selection . CBX5 and hnRNPA1 shares a 0.6 kb promoter sequence including binding sites for E2F and MYC-family transcription factors. Introduction of mutation in a USF/C-MYC recognition site upstream for the CBX5 transcriptional start site diminished differential expression in invasive versus poorly invasive breast cancer cells . Also, CBX5 promoter binding of the transcription factor YY1 is involved in regulating the differential expression levels in breast cancer cells . The decrease in CBX5 expression level in metastatic breast cancer cells correlates with decreased presence of H3K36me3, RNA polymerase II (Pol-II), and basal transcription factors at the promoter .
In this study, we find the differential expression of CBX5 in metastatic versus non-metastatic breast cancer cells requires a decoupling from the bi-directional promoter architecture of CBX5 and hnRNPA1, and investigate sequences downstream of the CBX5 promoter as possible mediators hereof.
MCF-7 (non-invasive breast cancer cells), MDA-MB-231 (highly invasive breast cancer cells), HEMC (Primary human mammary epithelial cells) and HeLa (cervical cancer cells) were grown in Dulbecco’s Modified Eagle’s Medium DMEM (Lonza) supplemented with 10 % fetal bovine serum, 1 % penicillin and 1 % glutamine. The cells were kept in a CO2-incubator with 5 % CO2 at 37 °C. The MCF7 and MDA-MB-231 cell lines were purchased from American Type Culture Collection, USA and HEMC from Life Technologies. For TSA treatment of cells 3x105 MCF7 and MDA-MB-231 cells were seeded in 6 - well plates the day before treatment. At the day of treatment, the media was replaced with growth media containing 1 μM TSA (Sigma) from a stock of 1 mM dissolved in a DMSO solution of 1:3.3. As a control, separate cells where given growth media containing the same amount of DMSO. The cells were harvested after 24 hours. mRNA stability in the MDA-MB-231 and MCF7 cells lines was examined by treating cells with Actinomycin D (Sigma), which inhibits de novo Pol-II transcription. 24 hours prior to treatment, 5x105 cells were seeded in 25 cm2 flasks to reach a confluence of 80 % at the time of treatment. Cells were added fresh DMEM growth media with Actinomycin D diluted in DMSO (1:3) to a final concentration of 10 μg/ml. Cells from one 25 cm2 flask were harvested after 0, 2, 4, 8, 12 and 24 hours, by washing twice with PBS and scraping in 1 ml Tri Reagent™ (Sigma) and subjected to RNA purification.
Breast cancer tissue
Breast tissue specimens were obtained from primary breast cancer surgical procedures as described . The Regional Ethics Committee Northern Jutland, Denmark approved the study (N-20070047), and signed informed consent was obtained from each patient.
RNA and cDNA
RNA purification was performed using Tri Reagent™ (Sigma). The suspension was transferred to RNAse-free eppendorf tubes and incubated for 5 minutes. 200 μl chloroform (Merck) was added per ml Tri Reagent and incubated for 10 minutes. After centrifugation at 12,000xg for 15 minutes at 4 °C, the upper RNA-containing phase was transferred to RNAse-free eppendorf tubes. 500 μl isopropanol (Merck) and 2 μl glycogen (Sigma) was added followed by centrifugation at 12,000xg for 30 minutes at 4 °C. The pellet was washed in 75 % RNAse-free ethanol and dissolved in 50 μl DEPC H2O and stored at −20 °C. RNA concentration was measured using a Thermo Scientific Nanodrop™ spectrophotometer. RNA integrity was confirmed by running samples on 1 % agarose gels with added ethidium bromide (AppliChem). For cell lines cDNA was synthesized from 0.5 μg RNA using the BIO-RAD iScript™ cDNA Synthesis kit containing a mix of oligo(dT) and random hexamer primers was used. After synthesis the cDNA product was diluted with redistilled water to a total volume of 100 μl and stored at −20 °C. For breast cancer samples, cDNA was synthesized from RNA previously isolated from primary normal breast tissue, breast carcinomas and lymph node metastases [43, 44]. cDNA was synthesized in a 20 μl reaction mix including 50 μmol/L Oligo(dT), reverse transcriptase (50 units/μL), RNase inhibitors (20 units/μL), 0.4 mmol/L of each dNTP, 1xPCR buffer, and 25 mmol/L MgCL2 (all from Applied Biosystems Inc., CA, USA). Reverse transcription was performed on the Perkin-Elmer GeneAmp PCR System 9600 Thermal Cycler (PerkinElmer Inc., MA, USA) with the profile: 42 °C for 30 minutes, 99 °C for 5 minutes and 4 °C until samples had cooled. cDNA was stored at −20 °C until further use.
For rapid amplification of cDNA 3′-ends (3′RACE) the first synthesis reaction utilized an oligo(dT)V primer with anchor sequence (GCGGAATTCGGATCCCTCGAGTTTTTTTTTTTTTTTTTTTV*, *V denotes G, C or A). cDNA was synthesized using 2 μg total RNA, 1 μl oligo(dT)V primer (50 pmol), 1 μl dNTP mix 10 mM (Qiagen), and nuclease-free water to a final volume of 13 μl. After incubation at 65 °C for 5 minutes, 4 μl First Strand Buffer (Invitrogen) and 2 μl DTT (Invitrogen) was added. Following incubation at 42 °C for 2 minutes, samples were added 1 μl (15U) Superscript II Reverse Transcriptase (Invitrogen) to a total volume of 20 μl and further incubated at 42 °C for 50 minutes. The PCR reaction was conducted with 5 μl of synthesized cDNA template, 10 pmol of target cDNA forward primer (CBX5 exon1 forward, GCAGACGTTAGCGTGAGTG) and 10 pmol of reverse oligo(dT)-r primer (GCGGAATTCGGATCCCTCGAGTT). A nested PCR was performed using reverse oligo(dT)-r primer and a target cDNA forward primer located downstream of the forward primer (STET nested forward, TGTAAGCCACTCGAAGCCACA). PCR products of interest were extracted after gel electrophoresis and sequenced.
Quantitative reverse transcriptase polymerase chain reaction (RT-qPCR)
For cell lines, RT-qPCR was performed in a total reaction volume of 10 μl including 1 μl cDNA, 5 μl Roche LightCycler® 480 SYBR Green I Master enzyme (Roche), 10 pmol of both forward and reverse primer and double distilled water up to 10 μl. A LightCycler® 480 (Roche) was used with a PCR profile of 10 sec denaturation at 95 °C, 20 sec annealing at 95 °C and 1 min elongation at 72 °C for 50 cycles. A list of primers used in the study is given in Additional file 1: Table S1. All primers were checked for amplification efficiency to be above 90 %. Amplification efficiencies were calculated using data collected from a relative standard curve, constructed by performing serial dilutions of cDNA or purified PCR product. The relative mRNA expression was calculated using the X0-method, and normalized to the reference gene GAPDH . For breast cancer samples, HMBS was used to control for variations in RNA concentration and integrity and was found to be the best suited reference gene when compared to ACTB, GAPDH, YWHAZ and B2M according to the Normfinder method . Quantitative real-time PCR was performed using Roche LightCycler® 480 with the settings stated above. The reaction mix consisted of 5 μL SYBR Green I Master Mix Buffer (Roche), 2.5 pmol forward and reverse primers (Eurofins MWG Synthesis GmbH), 1 μL cDNA and H20 to a final volume of 10 μL. The concentration was calculated using the standard curve method. Amplicon measurements outside of the range of the standard curve, or producing an incorrect melting peak were discarded.
Morpholino and siRNA
Morpholinos were designed by Gene Tools, LLC and transfected by the following procedure. 24 hours before transfection 5x104 MDA-MB-231 cells were seeded in 12 well plates. A transfection media of 1 ml was prepared containing 6 μl Endo-Porter (6 μM), 10 μl Morpholinos (10 μM) and 984 μl DMEM growth media, added to the cells, and incubated in a CO2 incubator at 37 °C for 48 hours. The morpholinos had the following sequences: STET E2A1 ATCAGGAGAAAAAGATGATTGCCCA, STET E2A2 GGACTCCTTCCTATTAGTACAATGA, and Standard Control CCTCTTACCTCAGTTACAATTTATA. STET-targeting Morpholinos were pooled in equal amounts during preparation of transfection media. For siRNA Transfections, 100,000 MCF7 cells and 50,000 MDA-MB-231 cells were used per reaction. 20 μM siRNA stocks kept at −80 °C were diluted to 2 μM with 1x Dharmacon buffer (Thermo Scientific). 25 μl siRNA was added to 25 μl DMEM (serum and penicillin/streptomycin free) and incubated for 5 minutes. Transfection-mix was made by mixing 1 μl Dharmafect 1 (Thermo Scientific) with 49 μl DMEM (serum and penicillin free) per reaction and incubated for 5 minutes at room temperature. 50 μL siRNA was added to 50 μl transfection-mix and incubated for 20 minutes at room temperature before added to the cells following incubation in CO2 incubator for 72 hours. Transfections were made in duplicates for each siRNA. siRNA sequences were the following: RRP6, CCAGUUAUACAGACCUAU; and RRP40, CACGCACAGUACUAGGUC. As a negative control, Non-Targeting siRNA (Thermo Scientific, Cat. No. D-001810-10-05) was used.
Dual reporter mini-gene constructions, transfections and genomic transpositions
Dual reporter mini-genes were constructed from the basis of the pVP4 vector, which includes a CMV promoter driven expression cassette with the β − globin exon1-intron-exon2 fused to the EGFP encoding gene . In addition, pVP4 includes an expression cassette for an autonomous neomycin resistance gene. By site directed mutagenesis, an AscI site was inserted central in the β − globin intron. By AseI and AscI digestion the entire CMV promoter as well as the β − globin exon1 and 5′end of the intron was removed. A 1.1 kb PCR fragment representing the bi-directional hnRNPA1 and CBX5 promoter with the exon1 sequences and approximately 200 bp intron 1 sequences was inserted. The promoter fragment was inserted in two different orientations using either primers Ase1-hnRNPA1, GATCATTAATGCAAGGAACGAAACCCAGCAGCATC, and Asc1-CBX5, GATCGGCGCGCCGTCCATTCATTTCACACAATAAC or Asc1-hnRNPA1, GATCGGCGCGCCGCAAGGAACGAAACCCAGCAGCATC, and Ase1-HP1α, GATCATTAATGTCCATTCATTTCACACAATAAC and thereby generating pCBX5-EGFP and phnRNPA1-EGFP. The vectors were cut by AseI and a PCR fragment inserted encompassing a 2 kb fragment with the 3′-end of the β − globin intron, β − globin exon 2, and the katushka reporter gene. This PCR fragment was generated with primers including NdeI sites, which are compatible with AseI. Thereby pBDf was generated that has the katushka transcriptional unit under control of the hnRNPA1 promoter and the EGFP transcriptional unit under control of the CBX5 promoter. pBDr has the katushka transcriptional unit under control of the CBX5 promoter and the EGFP transcriptional unit under control of the hnRNPA1 promoter. To generate a sleeping beauty transposon mini-gene, sbBDf, the required repetitive inverted elements were inserted to flank the katushka and EGFP transcriptional units in pBDf. A 2 kb fragment representing a continued extension of the CBX5 intron 1 present in sbBDf was generated by PCR with primers CBX5-Intron1-Asc1-f, ACTGGGCGCGCCCGTTATTGTGTGAAATGAATG and CBX5-Intron1-Asc1-r, ACTGGGCGCGCCACTCCCTAAACATTTCAAC and cloned in the AscI site to generate sbBDfPE. A 2 kb PCR fragment representing the STET exon including 3′-flanking intron sequences and pA signal downstream sequences was generated using the primers STET-Asc1-f,
TGACGGCGCGCCAGGTTTGGTATCAGGGTACA and STET-Asc1-r, TGACGGCGCGCCATAGCAGCCACAGGAAACTA and cloned in the AscI sites of pBDf and sbBDf to generate pBDfS and sbBDfS, respectively. 24 hours before transfection 2x105 cells were seeded in a 6 well plate. Next day, 2 μg of plasmid DNA, 6 μl X-treme gene 9 (Roche) and serum free DMEM media was mixed in a volume of 200 μl and incubated for 30 minutes at room temperature. The transfection mix was then added drop-wise to the growth media of the plated cells and incubated in CO2-incubator at 37 °C for 48 hours. For mini-gene genomic integration by transposition, 2x105 cells were seeded in a 6 well plate the day before transfection. Next day, 2 μg of transposon mini-gene constructs, 200 ng of SB Puro and 200 ng of SB100 (10:1:1) were mixed with 7.2 μl X-treme gene 9 and serum free DMEM media in a volume of 200 μl and mixed thoroughly and incubated for 30 minutes at room temperature. The transfection mix was then added drop-wise to the growth media of the plated cells and incubated in CO2-incubator at 37 °C for 48 hours. The transfection media was replaced by selection media (DMEM supplemented with 1 μg/ml puromycin (Sigma)) to select for cells stably expressing the puromycin resistance gene. Every 2–3 days cells were washed twice with 1 ml PBS and supplied with fresh selection media.
Chromatin immunoprecipitation (ChIP)
ChIP analyses were done essential as previously described [37, 48]. In summary, ChIP was performed with 10 ml cultures fixed with 1 % formaldehyde for 10 min followed by addition of glycine to 0.25 mM final concentration. Cross-linked cells were washed twice with cold PBS, scraped and lysed for 10 min at 4 °C in 1 % SDS, 50 mM Tris–HCl (pH 8.0) and 10 mM EDTA containing protease inhibitors. Lysates were sheared by sonication using a bioruptor (Diagenode, Liege, Belgium) to obtain chromatin fragments <0.5 kb and centrifuged for 15 min in a microfuge at 4 °C. 20 μg of soluble chromatin of each sample was incubated with antibody to the following epitopes: H3 (ab1791, Abcam, MA, USA) and H3K9ac (ab4441, Abcam) at 4 °C for 18 h and immunoprecipitated with a protein A and protein G magnetic bead mix (1:1) at 4 °C for 60 min. A mock precipitation including pre-immune polyclonal serum was included for each ChIP experiment. After sequential washing by the following buffers: three times with ChIP washing buffer I (20 mM Tris–HCl, 150 mM NaCl, 2 mM EDTA, 1 % Triton X-100. 0.1 % SDS), two times with ChIP washing buffer II (20 mM Tris–HCl, 350 mM NaCl. 2 mM EDTA, 1 % Triton X-100. 0.1 % SDS), two times with ChIP washing buffer III (20 mM Tris–HCl, 500 mM NaCl. 2 mM EDTA, 1 % Triton X-100), the chromatin was eluted from the beads with Elution buffer (100 mM NaHCO3. 1 % SDS) by rotating 15 min at room temperature. Cross-links were reversed by incubation at 65 °C for 5 to 20 h and treated with proteinase K and RNase A. DNA was purified by phenol-chloroform extraction and ethanol precipitation and eluted in 100 μl TE buffer. For quantitative detection of retained DNA, RT-qPCR were performed in triplicate and normalized to values obtained for amplicons corresponding to GAPDH.
Western blot and immunofluorescence
Proteins were detected in western blotting using mouse anti-HP1α clone15.19 s2 (Millipore 05–689) in 1:1,000 dilution and rabbit anti-β − Actin (Sigma A2013) in 1:10,000 dilution. Secondary antibodies were goat anti-mouse-HRP (Dako P0447) and goat anti-rabbit-HRP (Dako P0448) in 1:10,000 dilutions. Western blot procedures using 75 μg protein extract in each lane were as previously described except using Supersignal West Dure Extended Duration Substrate (Thermo Scientific 34076) and ImageQuant LAS4000 (GE Healthcare Life Sciences) for visualization . For immunofluorescence experiments cells were grown in 12 well plates on coverslips (VWR) pre-coated with Poly-L-Lysine (Sigma) to a confluence of ~60 %. Cells were cross-linked in 1 ml PBS containing formaldehyde (final concentration of 1 %) for 10 minutes at room temperature. Crosslinking was quenched by adding 114 μl 1.25 M glycine mixing by gentle pipetting in the well and incubated further for 5 minutes at room temperature. Cells were washed twice with 1 ml cold PBS and added 1 ml PBS containing 0.5 % Triton X-100 and protease inhibitors, and incubated for 15 minutes on ice. Cells were again washed twice with 1 ml cold PBS and blocked by adding 1 ml cold PBS containing 1 % BSA (Sigma) and incubated for 1 hour on ice. Primary mouse anti-HP1α antibody (1H5, Millipore) was diluted in PBS containing 1 % BSA of which 40 μl was placed on the bottom of a 10 cm2 petri-dish. The coverslips were placed on top of the 40 μl antibody with the cell side downwards. The petri-dish was sealed and incubated on ice for 1 hour. Coverslips were transferred to a new 12 well plate containing 1 ml cold PBS with the cell side upwards and washed 3x5 minutes on ice in 1 ml cold PBS. Secondary antibodies (Invitrogen) were diluted 1:2000 in cold PBS containing 1 % BSA, of which 1 ml was added to the coverslips after removing the PBS. The plate was wrapped in tinfoil and incubated for 30–60 minutes on ice. Coverslips were washed 5x5 minutes in 1 ml cold PBS and wrapped in tinfoil. Nuclei were dyed by adding 1 ml DAPI (Sigma) and incubating for 2–5 minutes at room temperature, and washed twice in 1 ml PBS. Coverslips were then dipped a few times in double distilled water and left to air dry in a tray wrapped in tinfoil. Coverslips were mounted on slides by adding a drop of Prolong Gold anti-fade reagent (Invitrogen) on the slide and transferring the coverslips on top with the cell side downwards.
Statistical analyses were performed using the experimental results calculated by the X0-method from triple RT-qPCR measurements for each sample  or the direct relative concentrations generated from the standard curves in the patient sample experiments. P-values were calculated using Students paired two-tailed t-test. Each experiment was repeated minimum three times.
HP1α down-regulation in MDA-MB-231 cells and the CBX5 and hnRNPA1 bi-directional transcriptional unit structure
The expression of CBX5 transcripts with coding potential for HP1α is decreased in invasive and migratory MDA-MB-231 breast cancer cells compared to the poorly invasive and migratory MCF-7 breast cancer cells [20, 36, 38, 40]. The decrease in HP1α expression is functionally linked to the enhanced invasion and migration capacity of MDA-MB-231 cells [36, 38, 40]. CBX5 has a bi-directional promoter arrangement with hnRNAP1 (Fig. 1a). In contrast to CBX5, hnRNPA1 is relative equally expressed in MDA-MB-231 and MCF7 cells (Fig. 1, Additional file 2: Table S2 and ). Thus, expression regulation of cellular amounts of HP1α must mechanistically be possible without associated alterations in the housekeeping gene hnRNPA1. We note that previous analyses of HP1α coding mRNA regulation have been focused on the CBX5 promoter sequences. However, due to the close proximity, it must be taken into account that an element affecting the transcriptional activity of CBX5 could also affect the activity of hnRNPA1. Despite the bi-directional promoter structure, no overall significant correlation in expression pattern is observed between CBX5 and hnRNPA1 in the NCI-60 cancer cell line panel (correlation coefficient 0.129) (Fig. 1b and Additional file 3: Figure S1). To investigate the relation between CBX5 and hnRNPA1 expression, RT-qPCR analysis in HMEC, MCF7 and MDA-MB-231 cells was performed. This showed 2.9-fold up-regulation of CBX5 relative to hnRNPA1 in MCF7 cells versus non-cancer breast epithelial cells (HMEC) and 0.62-fold down-regulation in MDA-MB-231 cells relative to HMEC (Fig. 1c). The expression analyses supported existence of independent regulation of CBX5 and hnRNPA1 transcription in breast cancer cells with a concordant up-regulation of the two genes from normal cells to cancer cells and subsequently specific down-regulation of CBX5 in metastatic cells (Fig. 1c). In a previous study, we showed that the CBX5 promoter is less occupied by basal transcription factors such as TBP, TFIIB, TFIIH as well as Pol-II in MDA-MB-231 cells when compared to MCF7 cells . The decrease in Pol-II presence was over the entire CBX5 gene. In contrast, histone H3 and the promoter signature marks, tri-methylated lysine 4 (H3K4me3) and acetylated lysine 9 (H3K9ac) on the histone tail of H3, were equally present throughout the promoter . Thus, we hypothesized two models facilitating differential regulation of CBX5 and hnRNPA1 from the basis of a bi-directional promoter. Either cis-binding of trans-regulators mediates specific regulation in the CBX5 transcriptional orientation or presence of regulatory elements outside the bi-directional promoter region that control transcription specifically in the CBX5 orientation. To test this, we constructed dual reporter mini-genes wherein the CBX5 and hnRNPA1 bi-directional promoter including both first exons and flanking intron sequences drives bi-directional expression of either green (EGFP) or red (Katushka) fluorescent proteins (Fig. 1d). After transient transfection into MCF7 and MDA-MB-231 cells, we observed no preferential down-regulation of CBX5 in MDA-MB-231 cells compared to MCF7 cells (Fig. 1d). Flipping the promoter region relative to the marker genes provided similar results (Fig. 1d). Thus, we conclude that the bi-directional promoter region per se is not sufficient to mediate preferential CBX5 down-regulation compared to hnRNPA1 in MDA-MB-231 cells versus MCF7 cells.
The transient transfection approach most likely eliminates detection of putative chromatin mediated effects and can be affected by high promoter sequence copy-number mediated titration of trans-factors. To reduce such confounders, we constructed a sleeping beauty based transposon mini-gene with the CBX5 and hnRNPA1 bi-directional promoter (Fig. 1e). The mini-gene was used to generate stable genome insertion with sleeping beauty transposase in MCF7 and MDA-MB-231 cells. Pools of cells with genome insertions were examined for transcriptional orientation specific mRNA expression. The result again showed that the bi-directional promoter does not have intrinsic capacity to preferential mediate CBX5 relative to hnRNPA1 transcriptional down-regulation in MDA-MB-231 cells versus MCF7 cells (Fig. 1e). The mini-gene lacked complete inclusion of the two CpG islands overlapping the bi-directional promoter and we therefore generated a mini-gene with a 2 kb intron 1 extension (Fig. 1a and e). Similar to the CBX5 and bi-directional promoter structure, CBX3 and hnRNPA2B1 have a 0.4 kb bi-directional promoter region, suggesting an evolutionary relationship between the HP1 encoding genes (Additional file 3: Figure S1C). The CBX3 and hnRNPA2B1 bi-directional transcriptional unit has been carefully analyzed due to the insulator capacity towards heterochromatin mediated gene silencing in transgenic constructs by the bi-directional promoter overlapping A2UCOE CpG island . We note that the CpG containing fragment from the CBX5 promoter resembles the A2UCOE from CBX3 and hnRNPA2B1, and we abbreviate the corresponding sequence A1UCOE. The inclusion of A1UCOE had a similar positive effect on hnRNPA1 and CBX5 transcriptional orientations (Fig. 1e). Based on the presented expression analyses, we conclude that the observed specific down-regulation of the CBX5 transcriptional orientation in MDA-MB-231 breast cancer cells, and thereby HP1α protein, most likely is not strictly promoter dependent, but involves promoter downstream sequences.
Deciphering novel transcripts originating from the large intron 1 of CBX5
Inspection of CBX5 revealed existence of a large intron 1 sequence of approximately 20 kb (Fig. 1a). Intron 1 sequences are approximately 23 kb and 1 kb for CBX1 and CBX3 (Additional file 3: Figure S1). In an attempt to address the importance of the intron 1 sequence for CBX5 regulation, we checked for the presence of transcriptional signatures using ENCODE data in the UCSC browser. We note that human CBX1 and CBX3 genes have alternative exon 1 sequences, and thereby alternative promoters (Additional file 3: Figure S1). From ENCODE derived data, two CBX5 signatures were evident. One representing possible additional promoter sequences in the 3′-region of intron 1 and another indicating the presence of a splice form between CBX5 exon 1 and an intron 1 embedded alternatively used exon (Fig. 2a). The latter will be described in further details below, and we will here focus on the putative alternative promoters in intron 1. Due to the existing nomenclature in UCSC of various transcriptional isoforms from CBX5, we will in the following term the HP1α protein-coding mRNA isoform originating from the CBX5 and hnRNPA1 bi-directional promoter for HP1α-Variant 3 (V3). The two novel potential mRNA isoforms are termed HP1α-Variant 1 (V1) and HP1α–Variant 2 (V2) with the latter having the most 5′-intron 1 location of the alternative exon 1 (Fig. 2a). The ENCODE data showed peaks of promoter mark signatures, H3K27ac and H3K4me3, as well as the presence of Pol-II over the alternative exon 1 sequences for HP1α-V1 and HP1α-V2 (Fig. 2a). This is in support of the presence of functional promoter sequences. We note that HP1α-V1, HP1α-V2, and HP1α-V3 mRNA isoforms all have coding potential for full-length HP1α protein given that the first consensus translational initiation codon resides in exon 2 for all three transcripts (Fig. 2a). The novel HP1α encoding transcriptional isoforms, V1 and V2, could participate in generating relatively higher HP1α expression in non-metastatic MCF7 breast cancer cells without requirement of specific CBX5 to hnRNPA1 transcriptional enhancement from the bi-directional promoter. To address this, we performed RT-qPCR analysis specifically detecting each transcriptional isoform in HMEC, MCF7 and MDA-MB-231 cells. We observed similar expression profiles for HP1α-V1 and HP1α-V2. HP1α-V3 had a distinct expression profile, which was similar to HP1α encoding mRNA detected by primers located in exons 4 and 5 and thereby the three isoforms altogether (HP1α-pan) (Fig. 2b). PCR experiments showed that the HP1α-V3 expression ratio relative to HP1α-V1 and HP1α-V2 was approximately 20-fold higher in HMEC, 3,500-fold higher in MCF7 and 30-fold higher in MDA-MB-231 cells (Fig. 2c). Thus, expression data did not support that HP1α-V1 and HP1α-V2 transcripts contribute significantly to the overall HP1α encoding transcript levels in neither MCF7 nor MDA-MB-231 cells. ENCODE data showed the highest peak of Pol-II over the alternative promoter sequences in HeLa cells (Fig. 2a). By RT-qPCR, we also found that HeLa cells express HP1α-V1 and HP1α-V2 at a level comparable to HP1α-V3 (Fig. 2b and c). Thus, the HP1α encoding V1 and V2 transcripts might in some cellular contexts quantitatively contribute to the total HP1α encoding transcript levels. In conclusion, the analysis of the novel HP1α-V1 and HP1α-V2 transcript isoforms were not supportive for a role directly involved in HP1α transcript and protein down-regulation in MDA-MB-231 compared to MCF7 cells.
We have previously shown that the H3 content over CBX5 is equal in MCF7 and MDA-MB-231 cells, whereas the chromatin mark coupled with transcriptional elongation, H3K36me3, was decreased over the CBX5 gene body in MDA-MB-231 cells compared to MCF7 cells . Chromatin compaction in CBX5 intron 1 could contribute to the low expression of HP1α-V1 and HP1α-V2. To address chromatin-mediated regulation, we treated MCF7 and MDA-MB-231 cells with the histone de-acetylase inhibitor trichostatin-A (TSA). Previous results have shown equal amounts of H3K9ac at the CBX5 promoter in MCF7 and MDA-MB-231 cells . To our surprise, we observed that in MDA-MB-231 cells TSA treatment resulted in 5-fold decreased CBX5 expression for all three HP1α encoding transcript isoforms (Fig. 3a). In MCF7, no significant TSA effect was observed (Fig. 3a). hnRNPA1 expression was 2-fold decreased following TSA treatment and this was also observed in MCF7 cells (Fig. 3a). We also observed HP1α protein down-regulation by western blotting and immunofluorescence analysis (Fig. 3b and Additional file 4: Figure S2B and S2C). ChIP analysis showed that the H3K9ac/H3 ratio in MDA-MB-231 cells decreased or was equal at the CBX5 and hnRNPA1 bi-directional promoter and increased at CBX5 downstream sequences following TSA treatment (Fig. 3c). Notably, the ChIP results for the alternative promoter regions for HP1α-V1 and HP1α-V2 showed a 3-fold increased level of H3K9ac, which did not correlate with increased mRNA expression (Fig. 3c).
Identifying a novel transcript isoform, STET, originating from alternative splicing and polyadenylation in intron 1 of CBX5
To further delineate the transcriptional structure of CBX5 intron 1 we next focused on an embedded alternative exon indicated by transcriptional signatures using ENCODE data in the UCSC browser. In silico a CBX5 transcript was identified consisting of exon 1 fused to this alternative spliced and polyadenylated exon embedded in intron 1 (Figs. 2a and 4a). We abbreviated this transcript for CBX5 skipped terminal exon transcript (STET). To verify the expression of STET, and eventual other CBX5 intron 1 derived transcripts, we screened for RNA expression using RT-PCR amplicons representing different intron 1 positions (Fig. 4a). Relative to amplicon A4 representing the intron 1 to STET1 exon boundary we observed an increase in RNA levels particularly in MDA-MB-231 cells corresponding to amplicon A5 representing the STET 3′-UTR (Fig. 4b). Amplicons located further downstream in intron 1 showed pronounced decrease in RNA levels in accordance with a major transcriptional stop mediated by the STET pA signal (Fig. 4b). We notice the presence of an array of 7 consensus pA signals 2 kb downstream from the STET pA signal in the CBX5 intron 1 sequence. Downstream of this multiple pA signal array, RNA transcript levels approached background (Fig. 4b). However, we could not identify transcripts terminated by the seven downstream pA signals by 3′-RACE. We note that downstream AU-rich regions can be important contributors in co-transcriptional cleavage (CoTC). During CoTC cleavage of the nascent transcript occurs 1–2 kb downstream of the polyadenylation signaling event, thereby releasing the polymerase followed by a subsequent cleavage at the pA signal . In conclusion, the expression data supported the existence of significant amounts of cellular RNA representing intron 1, including the STET exon (Fig. 4b). Further RT-PCR analyses and sequencing of amplicons verified the existence of STET mRNA in both MCF7 and MDA-MB-231 cells and that two different STET mRNAs were present (Fig. 4a-d). STET1 included an additional extension of 32 bases in the 5′-end compared to STET2 (Fig. 4a and c). 3′-RACE analyses showed that the STET isoforms were polyadenylated from an AUUAAA pA signal resulting in exon lengths of 383 and 351 bp for STET1 and STET2, respectively (Fig. 4c). Of additional sequence elements required for a functional pA signal, we note the presence of an upstream UGUA-element and downstream U-rich elements, which mediates binding of CstF-64  surrounding the STET AUUAAA motif (Fig. 4c). BLAST searches identified significant STET evolutionary conservation in various primates, including existence of the two alternative splice forms of STET in e.g. marmoset, but absence of STET in rodents. PCR experiments showed that STET2 mRNA was more abundant than STET1 mRNA in MCF7 and MDA-MB-231 cells (Fig. 4d). However, whereas STET1 was 0.43-fold down-regulated in MDA-MB-231 compared to MCF7 cells, STET2 was 1.65-fold up-regulated (Fig. 4d). Using a primer set detecting both STET mRNA isoforms, STET-pan, we observed that HP1α-V3 down-regulation in MDA-MB-231 versus MCF7 cells was not linked to decreased STET expression supporting independent regulation of the transcript levels (Fig. 4e). In contrast, TSA treatment resulted in similar response profiles for STET and HP1α-V3 (Figs. 4f and 3a).
Increased STET mRNA expression is not directly functionally associated with down-regulation of HP1α encoding mRNA
Each coupled alternative splicing and pA event resulting in one STET mRNA could decrease the generation of one consensus HP1α encoding transcript isoform V3 through STET exon pA mediated transcriptional termination. In a straightforward hypothesis, the increased generation of STET mRNA could mediate HP1α encoding mRNA down-regulation in metastatic breast cancer cells. In this case, the generation of STET transcripts would be at the same order of magnitude as HP1α encoding transcripts and STET mRNA down-regulation would follow HP1α-V3 mRNA up-regulation and vice versa. Expression analysis, however, showed a HP1α-V3 relative to STET expression in the order of 90-fold in MCF cells and 10-fold in MDA-MB-231 cells (Fig. 4e). HP1α-V3 mRNA is stable and low STET mRNA stability could lead to underestimation of the STET mRNA synthesis rate [37, 41]. This was not the case as RNA stability analysis showed an approximately similar stability of STET mRNA and HP1α-V3 mRNA (Additional file 5: Figure S3A). Moreover, rapid degradation of nascent STET mRNA by the RNA exosome could decrease the steady-state levels. siRNA mediated depletion of essential exosome components RRP6 and RRP40 influenced HP1α-V3 mRNA and STET mRNA levels, but not in an order of magnitude to support this mechanism to be involved generating preferential low levels of STET mRNA (Additional file 5: Figure S3B and C).
We next examined if down-regulation of STET mRNA directly associated with HP1α-V3 mRNA up-regulation. For this, we examined the consequences of down-regulating STET synthesis with morpholinos corresponding to the splice sites for the STET exon. Morpholino transfection of MDA-MB-231 cells with an equal mix of morpholinos targeting either of the splice sites resulted in 5-fold decrease in the amounts of spliced STET transcripts (Fig. 5a). This was not accompanied by a similar alteration in the amounts of un-spliced STET mRNA (amplicon A4) or RNA corresponding to the downstream utilized STET pA signal (amplicon A6) (Fig. 5a). A 0.63-fold decrease in expression was observed using an amplicon detecting both spliced and un-spliced STET (amplicon A5) (Fig. 5b). This was in accordance with a linkage between blocking of STET mRNA splicing and blocking of STET pA signal usage altogether resulting in a decrease in total STET generation. No corresponding increase in HP1α-V3 mRNA expression was observed un-favouring that STET mRNA generation is directly linked with HP1α-V3 mRNA generation in a significant amount (Fig. 5b). This cannot rule out the possibility for a stoichiometric effect such that each STET mRNA generated is accompanied with a decreased generation of one HP1α-V3 mRNA, but since the total amount of STET mRNA relative to HP1α-V3 mRNA is low this will be left undetectable. Finally, we examined how insertion of the STET exon in a dual reporter mini-gene under transcriptional control of the hnRNPA1 and CBX5 bi-directional promoter influenced expression. For this, we used the same expression vectors as described in Fig. 1 with the addition of a 1.17 kb STET exon and flanking sequences insert (Fig. 5c). Transient transfections in MCF7 and MDA-MB-231 cells resulted in no significant decrease in the CBX5 transcriptional orientation by inclusion of the STET exon (Fig. 5c). In cell lines with mini-gene integrations by transposition, we also did not detect significant STET exon mediated effects on the CBX5 transcriptional orientation (Fig. 5d). In conclusion, data did not support a model wherein STET exon sequences are mechanistically involved in abolishing the inclusion of downstream consensus HP1α encoding exons in quantitative amounts to mediate significant down-regulation of HP1α-V3 mRNA expression. Instead, the results favour that transcriptional down-regulation of the CBX5 gene in MDA-MB-231 cells increases the relative abundance of coupled STET exon alternative splicing and polyadenylation with a resulting increase in STET mRNA expression.
hnRNAP1, HP1α-V3 and STET mRNA expression during breast cancer progression
We next analysed the relationship between hnRNPA1, HP1α-V3 and STET mRNA expression in breast cancer samples to see whether this corresponds to observations from breast cancer cell lines. cDNA was prepared from paired tissue samples from 193 patients with breast cancer [43, 44]. 81 of the patients had metastases in the lymph nodes. From each patient a sample of normal breast tissue and primary breast carcinoma were obtained. From 78 of the patients a sample from the lymph node metastases was obtained. Expression levels for HP1α-V3, STET, and hnRNPA1 mRNA were measured by RT-qPCR in the normal breast, primary carcinoma samples and lymph node metastases. To acquire a normal distribution, the normalized expression values were log-transformed and all datasets passed the D’Agastino-Pearson normality test. Compared to normal breast tissue samples, HP1α-V3 mRNA expression was higher in both primary carcinoma samples from patients with lymph node metastasis (1.75-fold, P < 0.0001) and without lymph metastasis (2.02-fold, P < 0.0001) (Fig. 6b). HP1α-V3 expression was also higher in lymph node metastases compared to normal breast tissue (1.44-fold, P < 0.001) (Fig. 6b). HP1α-V3 expression in the primary carcinoma samples from patients without lymph node metastases was significantly higher than expression in lymph node metastases samples (1.40-fold, P < 0.01) (Fig. 6b). Albeit not statistically significant, there was also a tendency towards down-regulation of HP1α-V3 expression in primary carcinoma from patients with metastases compared to lymph nodes metastases (Fig. 6b). For hnRNPA1 mRNA we observed an increased expression between normal breast tissue and primary carcinoma samples from patients without metastasis (1.33-fold, P < 0.01) (Fig. 6a). hnRNPA1 also appeared upregulated in primary carcinoma samples from patients with metastasis, but not significantly (Fig. 6a). No difference in hnRNPA1 mRNA expression was observed between primary carcinoma and lymph node metastases samples (Fig. 6a). These results support the HMEC, MCF7 and MDA-MB-231 cell line results. For the expression ratio between HP1α-V3 and hnRNPA1, we observed an increase between normal breast tissue and primary carcinoma samples both from patients without metastasis (1.46-fold, P < 0.0001) and patients with metastasis (1.79-fold, P < 0.0001) (Fig. 6c). Also an increase from normal breast tissue to lymph node metastases was significant (1.2-fold, P < 0.05) (Fig. 6c). Thereby, the results from the in vivo material were in agreement with the results from cancer cell lines. No significant difference in STET mRNA expression was found between normal tissue and primary carcinoma from patients with or without lymph node metastasis (Fig. 6d). However, expression of STET was in normal breast lower than in lymph node metastases (0.75-fold, P < 0.05) (Fig. 6d). STET expression was also lower in carcinomas from patients without metastasis (0.73-fold, P < 0.05) and with metastasis (0.70-fold, P < 0.05) relative to lymph node metastases (Fig. 6d). The HP1α-V3 to STET ratio was significantly higher in primary carcinomas both from patients without metastasis (1.97-fold, P < 0.0001) and with metastasis (1.81-fold, P < 0.0001) relative to normal breast (Fig. 6e). The HP1α-V3 to STET ratio was also significantly higher in primary carcinomas both from patients without metastasis (1.76-fold, P < 0.0001) and with metastasis (1.61-fold, P < 0.01), compared to lymph node metastases (Fig. 6e). To account for variation in baseline HP1α-V3 mRNA expression levels between patients, we performed an alternative data analysis where we normalized the expression of HP1α-V3 and STET mRNA to the corresponding normal breast tissue sample (Additional file 6: Figure S4). For the HP1α-V3 to STET mRNA expression ratio, significant differences were observed for both primary carcinoma samples both from patients with metastasis (1.81-fold, P < 0.01) and without metastasis (1.68-fold, P < 0.01) compared to lymph node metastases (Additional file 6: Figure S4). Thus, irrespective of our data analysis method, we identified inverse correlation between HP1α-V3 and STET mRNA expression levels for primary breast carcinoma versus lymph node metastases. These findings are in alignment with the data presented for HMEC, MCF7 and MDA-MB-231 cell lines.
HP1α is over-expressed in several types of cancers and the over-expression is associated with increased cell proliferation most likely through silencing of cell proliferation inhibitors . Moreover, HP1α has a proliferation dependent expression level, which is reduced under transient cell cycle exit . Finally, a decrease in HP1α expression is functionally associated with an increased invasive potential of breast cancer cells most likely due to decreased silencing of pro-invasive genes. The Janus-faced regulation of HP1α expression during carcinogenesis can be a reflection of the inverse correlation that has been suggested between cancer cell proliferation and invasion [34, 52]. Cancer cell metastasis requires an acquisition of invasive potential and adaptation to a new environment, which can be incompatible with a high proliferation rate. A temporal slowdown of cell proliferation, accompanied by down-regulation of HP1α expression, can permit the expression of pro-invasive genes, thereby resulting in metastasis . However, the outgrowth of metastases requires cell proliferation and this process can be paramount for the final patient outcome, since high HP1α expression correlates with earlier diagnosis of metastasis . Because of the inverse correlation between HP1α expression and the invasive potential of cancer cells, knowledge on the differential regulation of HP1α expression is an important prospect in fundamental cancer research . In this study, we have shown that the decrease in HP1α expression in metastatic breast cancer cells involves promoter downstream sequences of the HP1α encoding CBX5 gene. hnRNPA1 and CBX5 shares a bi-directional promoter structure. Such “head-to-head” gene arrangements are found at a high frequency throughout the human genome with ~11 % of all genes defined as bi-directional promoter genes by being divergently transcribed, and with transcriptional start sites (TSS) less than 1 kb away from each other [53–55]. Bi-directional arrangements are often evolutionary conserved, indicating functional importance of this specific gene structural modulation [56–58]. In this line, expression of bi-directional promoter genes are more correlated than those of randomly selected and neighboring genes. This is exemplified by gene pairs needed in stoichiometric amounts e.g. histone genes, functioning in the same biological pathway e.g. DNA repair, and co-expressed at specific time points during cycle or in response to induction signals e.g. heat shock [54, 59]. Bi-directional promoter sequences share several features separating them from the general non-bi-directional promoters . Bi-directional promoters are more often located within a CpG island (77 %) compared to non-bi-directional promoters (38 %) and bi-directional promoters have a GC-content (66 %), which is higher than non-bi-directional promoters (53 %) [56–58]. Furthermore, the relative presence of canonical TATA box elements is significantly less for bi-directional promoters (8 %) compared to other promoters (28 %) [54, 60]. Bi-directional promoters display an enriched occurrence of specific transcription factor binding sites, including GABPA, MYC, E2F, NRF and YY1 . These cis-elements are often functionally shared for both transcriptional directions [54, 61]. The hnRNPA1 and CBX5 bi-directional promoter lacks TATA box elements, contains a CpG island, and includes binding motifs for signature bi-directional promoter transcription factors e.g. YY1, E2F and MYC, and thus is a consensus representative of bi-directional promoters [37, 40, 41, 62, 63]. We identified no significant correlated expression pattern between hnRNPA1 and CBX5 in the NCI-60 cancer cell panel. This is illustrated by the CBX5 down-regulation in metastatic breast cancer cells compared to poorly invasive breast cancer cell lines whereas hnRNPA1 is relatively evenly expressed in both types of cell lines [36, 37, 40, 41]. However, we note that from normal breast epithelial cells to MCF7 cells both hnRNPA1 and CBX5 are up-regulated. The scenario is different for the CBX3 and hnRNPA2B1 bi-directional promoter that results in a highly correlated expression of these two genes in the NCI-60 cancer cell panel including MCF7 and MDA-MB-231 cells. Thus, for hnRNPA1 and CBX5 evolution must have adapted regulatory mechanisms un-coupling the expression of the two genes under certain cellular environments e.g. during breast cancer metastasis. Going from an in vitro breast cancer cell model using HMEC, MCF7 and MDA-MB-231 cells to clinical breast cancer samples, we could largely replicate findings concerning the up-regulation of both hnRNPA1 and CBX5 in carcinoma versus normal breast epithelial cells, de-coupling of hnRNAP1 and CBX5 expression in metastatic breast cancer cells, and the relative up-regulation of the STET transcript in metastatic breast cancer cells. This validates that in this case our cell line based model is valuable for investigating in vivo breast cancer progression.
Previous studies have focused on human CBX5 regulation in terms of cis-elements and transcription factor binding to the consensus promoter region upstream and in exon 1. This resulted in the identification of a USF/C-MYC recognition site upstream for the CBX5 transcriptional start site to be involved mediating differential expression in invasive versus poorly invasive breast cancer cells . Based on observations in both transient and genome integrated reporter systems, our presented analyses point to importance of also promoter downstream transcriptional regulatory events. We observed that the isolated hnRNPA1 and CBX5 bi-directional promoter shows no significant preference for CBX5 relative to hnRNPA1 down-regulation in MDA-MB-231 cells. One hint of a transcriptional regulatory mechanism for CBX5 beyond promoter mediated initiation comes from a recent study of transcriptional pausing . The majority of human genes are at the promoter proximal region loaded with paused Pol-II poised for release by the positive elongation factor pTEFb into productive elongation. Gdown1 was shown to be a sub-stoichiometric subunit of Pol-II complex. Gdown1 inhibits termination of Pol II by TTF2 thereby preventing release of short transcripts and Pol-II dissociation, blocking elongation stimulation by TFIIF and influencing pausing factors NEFL and DSIF. The hnRNPA1 and CBX5 promoters are both associated with Gdown1 and poised Pol-II . Notably, two such Pol-II and Gdown1 peaks are present at CBX5 50 and 450 bp downstream of the bi-directional promoter . Since binding of Gdown1 to the promoter is linked with efficient transcriptional elongation and promoting stability of the paused Pol-II complex, deficiency in Gdown1 functional association to the bi-directional promoter in MDA-MB-231 cells could be a theoretical possibility. Thus, a skewed expression pattern in favor of hnRNPA1 expression relative to CBX5 expression will be obtainable, given the Gdown1 effect is directed specifically towards CBX5 in a yet not proven mechanism. This scenario is in line with our previous observation of less abundance of the transcriptional elongation chromatin mark H3K36me3 in MDA-MB-231 cells [37, 65]. Importantly, we observed that throughout the CBX5 gene, with the exception of the STET transcript to be discussed below, lesser amounts of transcripts were present in MDA-MB-231 cells compared to MCF7 cells. We have described that in MDA-MB-231 cells less Pol-II was present at the promoter compared to MCF7 cells . We note that Gdown1 is equally expressed in MCF7 and MDA-MB-231 cells (Additional file 2: Table S2).
Another possibility in breast cancer cells to mechanistically disconnect generation of HP1α from the functionally shared promoter architecture for CBX5 and hnRNPA1 is the use of downstream alternative promoters producing HP1α coding transcripts. We identified two such alternative promoters in the CBX5 intron 1 resulting in two additional HP1α encoding transcripts, HP1α-V1 and HP1α-V2. Both transcripts contain the entire full-length HP1α coding region, but with an alternative first exon not included in the canonical HP1α encoding transcript, HP1α-V3. However, in the cancer cell lines the quantitative significant production of HP1α was concluded to be restricted to transcripts produced from the bi-directional promoter. In HMEC, MCF7 and MDA-MB-231 cells we observed an inverse expression pattern of HP1α-V3 compared to HP1α-V1 and HP1α-V2. This could be a consequence of transcriptional interference where high transcriptional rate dictated from the bi-directional promoter repressed activity of the downstream alternative promoters. It should not be ruled out that the alternative CBX5 promoters e.g. in certain cell or tissue types or during cell cycle or developmental stages, could contribute significantly to HP1α expression. In line with this, we note that we in HeLa cells observed a significant contribution of theses alternative transcripts to the total content of HP1α encoding mRNA. Recently, an alternative downstream promoter for generating HP1α encoding mRNA was described in mice and the significance can be based upon a high degree of sequence conservation in mammalians of the genomic region corresponding to the alternative promoters . Surprisingly, we observed after TSA treatment of MDA-MB-231 cells a coordinated and strong down-regulation of HP1α-V3, HP1α-V1, HP1α-V2, and STET transcripts as well as down-regulation of HP1α protein expression. hnRNPA1 was also down-regulated but to a lesser extent. In MCF7 cells hnRNPA1 was repressed by TSA in magnitude similar to MDA-MB-231 cells whereas CBX5 transcripts displayed only a minor and non-coordinated response. MDA-MB-231 ChIP experiments showed no TSA induced increase in levels of acetylated histone H3 at the bi-directional promoter region. Repression of the CBX5-hnRNPA1 locus could be mediated through recruitment of a TSA induced trans-repressor. However, we note that the TSA induced decrease of the CBX5 transcripts in MDA-MB-231 cells was more pronounced than could expected for only an effect on transcription given the relative high mRNA stability (Additional file 5: Figure S3 and ). This could indicate TSA induced de-stabilization of CBX5 transcripts, similar to e.g. claudin-1 mRNA .
Bioinformatics analysis, as well as analysis of the mouse CBX5 gene, revealed presence of several evolutionary conserved regions and transcribed regions in CBX5 intron 1 . Our further investigation of one such region led to the identification of two novel transcripts from CBX5 termed STET1 and STET2. These are transcribed from the same promoter as HP1α-V3 mRNA and thereby contain exon 1 which is now spliced to an intron 1 embedded alternative exon located ~5 kb downstream of the TSS. The alternative STET exon includes a functional pA signal. STET mRNA generation thereby constitute an alternative cleavage and polyadenylation (APA) event and the STET exon E2A classifies as a composite terminal exon. Studies analyzing APA events have mainly been focused on the 3′-UTR, but RNA-sequence analysis have revealed that 20 % of human genes have at least one intronic APA event and that the APA events can be developmental and cell cycle regulated to regulate expression [68–70]. We note that E2F transcription factors were described to enhance alternative intronic polyadenylation in a cell proliferative dependent manner and the presence of a E2F cis-element in the bi-directional promoter could provide a link to STET mRNA generation . Mechanistic selection of STET alternative splicing and polyadenylation is expected in stoichiometric amounts to decrease the generation of HP1α-V3 transcripts with HP1α encoding potential. Given that STET is relatively more expressed in MDA-MB-231 cells compared to MCF7 cells this opens an appealing model for the specific CBX5 relative to hnRNPA1 down-regulation in MDA-MB-231 cells. This will however require that STET mRNA generation in quantitative amounts is comparable with HP1α encoding mRNA. Since our analyses systematically identified STET mRNA in minor amounts compared to HP1α encoding mRNA, we have no supportive evidence for such a regulatory model. Furthermore, insertion of the STET composite terminal exon in a mini-gene background had neither in transient nor genome integrated analysis a negative influence for the inclusion of a STET exon downstream located exon. Finally, despite that we find the bi-directional promoter equally transcriptional prone in MCF7 and MDA-MB-231 cells, we also observed less exon 1 included transcripts and less Pol-II, TBP, TFIIB, and TFIIH loading on the canonical CBX5 promoter in MDA-MB-231 cells indicating less transcription . It is important to notice that histone H3 as well as H3K9ac and H3K4me3 occupancy over the CBX5 promoter was similar in the two cell lines pointing that the chromatin structure per se is not inhibitory in MDA-MB-231 cells . Thereby, the current results could fit a model wherein reduced CBX5 transcriptional quality in metastatic breast cancer cells mediated by downstream elements e.g. through impaired transcriptional re-initiation and elongation, results in relative increased inclusion of the STET composite exon.
History has dictated genes to be perceived as linear entities confined by promoters and terminators that determine where transcription starts and ends. Studies concerning the regulation of HP1α have hence mainly been restricted to the canonical CBX5 promoter region. However, our presented results for the differentially expressed CBX5 mRNA and the constitutively expressed hnRNPA1 mRNA have indicated novel mechanisms associated with regulation of HP1α expression through sequences located downstream the bi-directional promoter. The present study highlights the need for additional focus on the transcriptional regulatory mechanistic backgrounds for deregulated HP1α expression under development and metastatic progression of breast cancer.
In this study, we demonstrate that an hnRNPA1 and CBX5 bi-directional core promoter fragment shows no significant preference for CBX5 relative to hnRNPA1 down-regulation in metastatic MDA-MB-231 cells. Thus, we conclude that the bi-directional promoter region per se is not sufficient to mediate preferential CBX5 down-regulation compared to hnRNPA1 in MDA-MB-231 cells versus MCF7 cells, but involve sequences located downstream the canonical CBX5 promoter. Characterization of transcriptional events in the CBX5 20 kb long intron 1 revealed existence of several novel CBX5 transcripts. Two of these encoded consensus HP1α protein but used autonomous promoters located within intron 1 by which HP1α expression could be de-coupled from the bi-directional promoter. However, in breast cancer cell lines a quantitative significant production of HP1α was concluded to be restricted to transcripts with origin from the bi-directional promoter. In addition, a novel CBX5 transcriptional isoform, STET, was discovered. This transcript includes CBX5 exon 1 and part of intron 1 sequences through alternative splicing and polyadenylation, but lacks inclusion of HP1α encoding exons. Inverse correlation between STET and HP1α coding mRNA expression, transcribed from the canonical CBX5 bi-directional promoter was observed in both breast cancer cell lines and samples from breast cancer patients. Mechanistic selection of STET alternative splicing and polyadenylation is expected in stoichiometric amounts to decrease the generation of CBX5 transcripts with HP1α encoding potential. This could thereby comprise a novel mechanism of HP1α encoding mRNA regulation. However, we systematically identified STET mRNA in minor amounts compared to HP1α encoding mRNA. Moreover, insertion of the STET composite terminal exon in a mini-gene background had neither in transient nor genome integrated analysis a negative influence for the inclusion of a STET exon downstream located exon. Thus, we have no supportive evidence for such a regulatory model. Therefore, the results more likely reflects a model wherein reduced CBX5 transcriptional quality mediated by promoter downstream mechanisms e.g. through impaired transcriptional re-initiation and elongation, results in relative increased inclusion of the STET composite exon.
Availability of supporting data
All the supporting data are included as additional files.
Alternative cleavage and polyadenylation
Chromo box protein homolog
Enhanced green fluorescent protein
Histone H3 lysine position 9
Histone H3 lysine position 9 acetylation
Histone H3 lysine position 9 di- and tri-methylation
Heterochromatin protein 1
Katushka fluorescent protein
Open reading frame
- pA signal:
Position effect variegation
RNA polymerase II
Reverse transcriptase quantitative PCR
Skipped terminal exon transcript
James TC, Elgin SC. Identification of a nonhistone chromosomal protein associated with heterochromatin in Drosophila melanogaster and its gene. Mol Cell Biol. 1986;6(11):3862–72.
Singh PB, Miller JR, Pearce J, Kothary R, Burton RD, Paro R, et al. A sequence motif found in a Drosophila heterochromatin protein is conserved in animals and plants. Nucleic Acids Res. 1991;19(4):789–94.
Saunders WS, Chue C, Goebl M, Craig C, Clark RF, Powers JA, et al. Molecular cloning of a human homologue of Drosophila heterochromatin protein HP1 using anti-centromere autoantibodies with anti-chromo specificity. J Cell Sci. 1993;104(Pt 2):573–82.
Le Douarin B, Nielsen AL, Garnier JM, Ichinose H, Jeanmougin F, Losson R, et al. A possible involvement of TIF1 alpha and TIF1 beta in the epigenetic control of transcription by nuclear receptors. EMBO J. 1996;15(23):6701–15.
Nielsen AL, Ortiz JA, You J, Oulad-Abdelghani M, Khechumian R, Gansmuller A, et al. Interaction with members of the heterochromatin protein 1 (HP1) family and histone deacetylation are differentially involved in transcriptional silencing by members of the TIF1 family. EMBO J. 1999;18(22):6385–95.
Paro R, Hogness DS. The Polycomb protein shares a homologous domain with a heterochromatin-associated protein of Drosophila. Proc Natl Acad Sci U S A. 1991;88(1):263–7.
Aasland R, Stewart AF. The chromo shadow domain, a second chromo domain in heterochromatin-binding protein 1, HP1. Nucleic Acids Res. 1995;23(16):3168–73.
Nielsen AL, Oulad-Abdelghani M, Ortiz JA, Remboutsika E, Chambon P, Losson R. Heterochromatin formation in mammalian cells: interaction between histones and HP1 proteins. Mol Cell. 2001;7(4):729–39.
Minc E, Allory Y, Worman HJ, Courvalin JC, Buendia B. Localization and phosphorylation of HP1 proteins during the cell cycle in mammalian cells. Chromosoma. 1999;108(4):220–34.
Nielsen AL, Sanchez C, Ichinose H, Cervino M, Lerouge T, Chambon P, et al. Selective interaction between the chromatin-remodeling factor BRG1 and the heterochromatin-associated protein HP1alpha. EMBO J. 2002;21(21):5797–806.
Lachner M, O’Carroll D, Rea S, Mechtler K, Jenuwein T. Methylation of histone H3 lysine 9 creates a binding site for HP1 proteins. Nature. 2001;410(6824):116–20.
Nielsen SJ, Schneider R, Bauer UM, Bannister AJ, Morrison A, O’Carroll D, et al. Rb targets histone H3 methylation and HP1 to promoters. Nature. 2001;412(6846):561–5.
Daujat S, Zeissler U, Waldmann T, Happel N, Schneider R. HP1 binds specifically to Lys26-methylated histone H1.4, whereas simultaneous Ser27 phosphorylation blocks HP1 binding. J Biol Chem. 2005;280(45):38090–5.
Brasher SV, Smith BO, Fogh RH, Nietlispach D, Thiru A, Nielsen PR, et al. The structure of mouse HP1 suggests a unique mode of single peptide recognition by the shadow chromo domain dimer. EMBO J. 2000;19(7):1587–97.
Cowieson NP, Partridge JF, Allshire RC, McLaughlin PJ. Dimerisation of a chromo shadow domain and distinctions from the chromodomain as revealed by structural analysis. Curr Biol. 2000;10(9):517–25.
Le Douarin B, You J, Nielsen AL, Chambon P, Losson R. TIF1alpha: a possible link between KRAB zinc finger proteins and nuclear receptors. J Steroid Biochem Mol Biol. 1998;65(1–6):43–50.
Ye Q, Callebaut I, Pezhman A, Courvalin JC, Worman HJ. Domain-specific interactions of human HP1-type chromodomain proteins and inner nuclear membrane protein LBR. J Biol Chem. 1997;272(23):14983–9.
Seeler JS, Marchio A, Sitterlin D, Transy C, Dejean A. Interaction of SP100 with HP1 proteins: a link between the promyelocytic leukemia-associated nuclear bodies and the chromatin compartment. Proc Natl Acad Sci U S A. 1998;95(13):7316–21.
Murzina N, Verreault A, Laue E, Stillman B. Heterochromatin dynamics in mouse cells: interaction between chromatin assembly factor 1 and HP1 proteins. Mol Cell. 1999;4(4):529–40.
Vad-Nielsen J, Nielsen AL. Beyond the histone tale: HP1alpha deregulation in breast cancer epigenetics. Cancer Biol Ther. 2015;16(2):189–200.
Nozawa RS, Nagao K, Masuda HT, Iwasaki O, Hirota T, Nozaki N, et al. Human POGZ modulates dissociation of HP1alpha from mitotic chromosome arms through Aurora B activation. Nat Cell Biol. 2010;12(7):719–27.
Yamamoto K, Sonoda M. Self-interaction of heterochromatin protein 1 is required for direct binding to histone methyltransferase, SUV39H1. Biochem Biophys Res Commun. 2003;301(2):287–92.
Lavigne M, Eskeland R, Azebi S, Saint-Andre V, Jang SM, Batsche E, et al. Interaction of HP1 and Brg1/Brm with the globular domain of histone H3 is required for HP1-mediated repression. PLoS Genet. 2009;5(12):e1000769.
Richart AN, Brunner CI, Stott K, Murzina NV, Thomas JO. Characterization of chromoshadow domain-mediated binding of heterochromatin protein 1alpha (HP1alpha) to histone H3. J Biol Chem. 2012;287(22):18730–7.
Dawson MA, Bannister AJ, Gottgens B, Foster SD, Bartke T, Green AR, et al. JAK2 phosphorylates histone H3Y41 and excludes HP1alpha from chromatin. Nature. 2009;461(7265):819–22.
Jang SM, Azebi S, Soubigou G, Muchardt C. DYRK1A phoshorylates histone H3 to differentially regulate the binding of HP1 isoforms and antagonize HP1-mediated transcriptional repression. EMBO Rep. 2014;15(6):686–94.
Maison C, Bailly D, Peters AH, Quivy JP, Roche D, Taddei A, et al. Higher-order structure in pericentric heterochromatin involves a distinct pattern of histone modification and an RNA component. Nat Genet. 2002;30(3):329–34.
Muchardt C, Guilleme M, Seeler JS, Trouche D, Dejean A, Yaniv M. Coordinated methyl and RNA binding is required for heterochromatin localization of mammalian HP1alpha. EMBO Rep. 2002;3(10):975–81.
Allo M, Buggiano V, Fededa JP, Petrillo E, Schor I, de la Mata M, et al. Control of alternative splicing through siRNA-mediated transcriptional gene silencing. Nat Struct Mol Biol. 2009;16(7):717–24.
Ameyar-Zazoua M, Rachez C, Souidi M, Robin P, Fritsch L, Young R, et al. Argonaute proteins couple chromatin silencing to alternative splicing. Nat Struct Mol Biol. 2012;19(10):998–1004.
Wallrath LL. Unfolding the mysteries of heterochromatin. Curr Opin Genet Dev. 1998;8(2):147–53.
Eissenberg JC, James TC, Foster-Hartnett DM, Hartnett T, Ngan V, Elgin SC. Mutation in a heterochromatin-specific chromosomal protein is associated with suppression of position-effect variegation in Drosophila melanogaster. Proc Natl Acad Sci U S A. 1990;87(24):9923–7.
Eissenberg JC, Morris GD, Reuter G, Hartnett T. The heterochromatin-associated protein HP-1 is an essential protein in Drosophila with dosage-dependent effects on position-effect variegation. Genetics. 1992;131(2):345–52.
De Koning L, Savignoni A, Boumendil C, Rehman H, Asselain B, Sastre-Garau X, et al. Heterochromatin protein 1alpha: a hallmark of cell proliferation relevant to clinical oncology. EMBO Mol Med. 2009;1(3):178–91.
Kirschmann DA, Seftor EA, Nieva DR, Mariano EA, Hendrix MJ. Differentially expressed genes associated with the metastatic phenotype in breast cancer. Breast Cancer Res Treat. 1999;55(2):127–36.
Kirschmann DA, Lininger RA, Gardner LM, Seftor EA, Odero VA, Ainsztein AM, et al. Down-regulation of HP1Hsalpha expression is associated with the metastatic phenotype in breast cancer. Cancer Res. 2000;60(13):3359–63.
Thomsen R, Christensen DB, Rosborg S, Linnet TE, Blechingberg J, Nielsen AL. Analysis of HP1alpha regulation in human breast cancer cells. Mol Carcinog. 2011;50(8):601–13.
Norwood LE, Moss TJ, Margaryan NV, Cook SL, Wright L, Seftor EA, et al. A requirement for dimerization of HP1Hsalpha in suppression of breast cancer invasion. J Biol Chem. 2006;281(27):18668–76.
Debies MT, Welch DR. Genetic basis of human breast cancer metastasis. J Mammary Gland Biol Neoplasia. 2001;6(4):441–51.
Norwood LE, Grade SK, Cryderman DE, Hines KA, Furiasse N, Toro R, et al. Conserved properties of HP1(Hsalpha). Gene. 2004;336(1):37–46.
Lieberthal JG, Kaminsky M, Parkhurst CN, Tanese N. The role of YY1 in reduced HP1alpha gene expression in invasive human breast cancer cells. Breast Cancer Res. 2009;11(3):R42.
Bekenstein U, Soreq H. Heterogeneous nuclear ribonucleoprotein A1 in health and neurodegenerative disease: from structural insights to post-transcriptional regulatory roles. Mol Cell Neurosci. 2013;56:436–46.
Brügmann A, Jensen V, Garne JP, Nexo E, Sorensen BS. Expression of the Epidermal Growth Factor Receptors and Ligands in Paired Samples of Normal Breast Tissue, Primary Breast Carcinomas and Lymph Node Metastases. Adv Breast Cancer Res. 2014;3:22–37. http://dx.doi.org/10.4236/abcr.2014.32005.
Palimaru I, Brugmann A, Wium-Andersen MK, Nexo E, Sorensen BS. Expression of PIK3CA, PTEN mRNA and PIK3CA mutations in primary breast cancer: association with lymph node metastases. SpringerPlus. 2013;2:464.
Thomsen R, Solvsten CA, Linnet TE, Blechingberg J, Nielsen AL. Analysis of qPCR data by converting exponentially related Ct values into linearly related X0 values. J Bioinform Comput Biol. 2010;8(5):885–900.
Andersen CL, Jensen JL, Orntoft TF. Normalization of real-time quantitative reverse transcription-PCR data: a model-based variance estimation approach to identify genes suited for normalization, applied to bladder and colon cancer data sets. Cancer Res. 2004;64(15):5245–50.
Zhou Z, Thomsen R, Kahns S, Nielsen AL. The NSD3L histone methyltransferase regulates cell cycle and cell invasion in breast cancer cells. Biochem Biophys Res Commun. 2010;398(3):565–70.
Zhou Z, Kahns S, Nielsen AL. Identification of a novel vimentin promoter and mRNA isoform. Mol Biol Rep. 2009;37(5):2407–13.
Antoniou MN, Skipper KA, Anakok O. Optimizing retroviral gene expression for effective therapies. Hum Gene Ther. 2013;24(4):363–74.
Nojima T, Dienstbier M, Murphy S, Proudfoot NJ, Dye MJ. Definition of RNA polymerase II CoTC terminator elements in the human genome. Cell Rep. 2013;3(4):1080–92.
Hoque M, Ji Z, Zheng D, Luo W, Li W, You B, et al. Analysis of alternative cleavage and polyadenylation by 3′ region extraction and deep sequencing. Nat Methods. 2013;10(2):133–9.
Berglund P, Landberg G. Cyclin e overexpression reduces infiltrative growth in breast cancer: yet another link between proliferation control and tumor invasion. Cell Cycle. 2006;5(6):606–9.
Adachi N, Lieber MR. Bidirectional gene organization: A common architectural feature of the human genome. Cell. 2002;109(7):807–9.
Trinklein ND, Aldred SF, Hartman SJ, Schroeder DI, Otillar RP, Myers RM. An abundance of bidirectional promoters in the human genome. Genome Res. 2004;14(1):62–6.
Yang MQ, Koehly LM, Elnitski LL. Comprehensive annotation of bidirectional promoters identifies co-regulation among breast and ovarian cancer genes. PLoS Comput Biol. 2007;3(4):e72.
Koyanagi KO, Hagiwara M, Itoh T, Gojobori T, Imanishi T. Comparative genomics of bidirectional gene pairs and its implications for the evolution of a transcriptional regulation system. Gene. 2005;353(2):169–76.
Li YY, Yu H, Guo ZM, Guo TQ, Tu K, Li YX. Systematic analysis of head-to-head gene organization: evolutionary conservation and potential biological relevance. PLoS Comput Biol. 2006;2(7):e74.
Yang MQ, Taylor J, Elnitski L. Comparative analyses of bidirectional promoters in vertebrates. BMC Bioinformatics. 2008;9 Suppl 6:S9.
Lin JM, Collins PJ, Trinklein ND, Fu Y, Xi H, Myers RM, et al. Transcription factor binding and modified histones in human bidirectional promoters. Genome Res. 2007;17(6):818–27.
Yang MQ, Elnitski LL. Diversity of core promoter elements comprising human bidirectional promoters. BMC Genomics. 2008;9 Suppl 2:S3.
Wakano C, Byun JS, Di LJ, Gardner K. The dual lives of bidirectional promoters. Biochim Biophys Acta. 2012;1819(7):688–93.
Weinmann AS, Yan PS, Oberley MJ, Huang TH, Farnham PJ. Isolating human transcription factor targets by coupling chromatin immunoprecipitation and CpG island microarray analysis. Genes Dev. 2002;16(2):235–44.
Oberley MJ, Inman DR, Farnham PJ. E2F6 negatively regulates BRCA1 in human cancer cells without methylation of histone H3 on lysine 9. J Biol Chem. 2003;278(43):42466–76.
Cheng B, Li T, Rahl PB, Adamson TE, Loudas NB, Guo J, et al. Functional association of Gdown1 with RNA polymerase II poised on human genes. Mol Cell. 2012;45(1):38–50.
Zhou Z, Kahns S, Nielsen AL: Identification of a novel vimentin promoter and mRNA isoform. Mol Biol Rep 2010;37(5):2407-13. doi: 10.1007/s11033-009-9751-8.
Thliveris AT, Clipson L, Sommer LL, Schoenike BA, Hasenstein JR, Schlamp CL, et al. Regulated Expression of Chromobox Homolog 5 Revealed in Tumors of Apc(Min) (/+) ROSA11 Gene Trap Mice. G3. 2012;2(5):569–78.
Krishnan M, Singh AB, Smith JJ, Sharma A, Chen X, Eschrich S, et al. HDAC inhibitors regulate claudin-1 expression in colon cancer cells through modulation of mRNA stability. Oncogene. 2010;29(2):305–12.
Luo W, Ji Z, Pan Z, You B, Hoque M, Li W, et al. The conserved intronic cleavage and polyadenylation site of CstF-77 gene imparts control of 3′ end processing activity through feedback autoregulation and by U1 snRNP. PLoS Genet. 2013;9(7):e1003613.
Shi Y. Alternative polyadenylation: new insights from global analyses. RNA. 2012;18(12):2105–17.
Tian B, Pan Z, Lee JY. Widespread mRNA polyadenylation events in introns indicate dynamic interplay between polyadenylation and splicing. Genome Res. 2007;17(2):156–65.
Elkon R, Drost J, van Haaften G, Jenal M, Schrier M, Oude Vrielink JA, et al. E2F mediates enhanced alternative polyadenylation in proliferation. Genome Biol. 2012;13(7):R59.
This work was supported by The Lundbeck Foundation, Familien Hede Nielsens Fond, Direktør Jacob Madsen & Hustru Olga Madsens Fond, Fabrikant Einar Willumsens Mindelegat, Marie og Børge Kroghs Fond, and Fonden til Lægevidenskabens Fremme. We thank Toke Elbæk Linnet and Dennis Bruun Christensen for the scientific contribution to the hereby presented results.
The authors declare that they have no competing interests.
JVN and ALN designed the experiments. JVN, KRJ, RT, and TD conducted the experiments. AB and BSS collected and prepared the tissue samples from breast cancer patients. JVN and ALN analyzed the data obtained from the experiments. JVN and ALN wrote the manuscript. All authors read and approved the manuscript.
Sequences for primers used in RT-qPCR. (DOCX 17 kb)
Expression data extracted from Affymetrix microarray experiments. (DOCX 17 kb)
CBX1 and CBX3 and correlation of expression analyses. A) Schematized view of CBX3 and hnRNPA2B1 (not drawn to scale). Arrows indicate direction of transcription. The coding region is indicated by black colouring. pA indicates the localization of poly-A signals. A2UCOE represents localization of the characterized insulator element. B) Correlation analysis of CBX3 and hnRNPA2B1 expression in the NCI-60 breast cancer cell panel. The analysis presented as heat map was performed using the CellMiner database, http://discover.nci.nih.gov/cellminer/, with red symbolizing positive and blue negative correlation. C) Correlation analysis of CBX1, CBX3, CBX5, hnRNPA1 and hnRNPA2B1 expression in the NCI-60 breast cancer cell panel. The analysis presented as correlation coefficients estimated using the CellMiner database with red numbering symbolizing significant expression correlation. D) Schematized view of CBX1 and neighboring SNX11 (not drawn to scale). Arrows indicate direction of transcription. The coding region is indicated by black coloring. The position of a promoter overlapping CpG island is shown. (PDF 380 kb)
TSA effects on CBX1, CBX3 and CBX5 expression. A) mRNA expression analysis of the CBX1, CBX3 and CBX5 response towards TSA. Relative expression levels of CBX mRNA in MCF7 and MDA-MB-231 cells after 24 h treatment with TSA or control DMSO. Relative expression was calculated from RT-qPCR using GAPDH expression for normalization. For all panels, bars represent mean values with standard deviations. B) Immunofluorescence analysis of HP1α (upper panels) or DAPI staining in MDA-MB-231 cells either untreated or TSA treated for 24 h. C) Zooming in on a representative immunofluorescence analysis of HP1α in MDA-MB-231 cells with arrows pointing on heterochromatic spots. (PDF 914 kb)
RNA stability analysis of HP1α-V3 and STET. A-B) mRNA decay analysis of HP1α-V3, STET and C-MYC following Actinomycin D treatment in MCF7 (A) and MDA-MB-231 cells (B). Cells were treated with Actinomycin D and harvested at indicated time points. Relative expression was calculated from RT-qPCR using GAPDH expression for normalization. C) Knockdown efficiency of siRNA mediated knockdown of RRP6 and RRP40 mRNA in MCF7 and MDA-MB-231 cells, respectively. Expression of HP1α-V3, STET and amplicon A1 RNA after RRP6 and RRP40 siRNA mediated knockdown in MCF7 and MDA-MB-231 cells, respectively. Relative expression was calculated from RT-qPCR using GAPDH expression for normalization. For all panels, bars represent mean values with standard deviations. (PDF 574 kb)
Expression analysis of hnRNPA1, HP1α-V3 and STET in breast cancer biopsies normalized to normal breast biopsies. A-E) Based on a standard curve of serial dilutions of cDNA with known concentrations, quantification was determined from single measurements with the second derivate max method by the LightCycler software. Relative expression was calculated using HMBS for normalization. To correct for diversity of baseline expression between patients, expression of each carcinoma sample was further normalized to the corresponding normal breast tissue sample of that patient. Results are presented as log-transformed values of HMBS and normal breast tissue normalized data. N indicates the number of samples with measurements above limit of detection. For all panels, bars represent mean values with standard deviations. ** P < 0.01; one-way ANOVA with Tukey’s multiple comparison. For datasets with significantly different standard deviations between means non-parametric Kruskal-Wallis test with Dunn’s multiple comparison was performed. (PDF 333 kb)
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Vad-Nielsen, J., Jakobsen, K.R., Daugaard, T. et al. Regulatory dissection of the CBX5 and hnRNPA1 bi-directional promoter in human breast cancer cells reveals novel transcript variants differentially associated with HP1α down-regulation in metastatic cells. BMC Cancer 16, 32 (2016). https://doi.org/10.1186/s12885-016-2059-x
- Cell invasion
- Transcriptional regulation