Histone proteins are essential for chromatin formation, and histone gene expression is coupled to DNA synthesis. In metazoans, the histone RNA binding protein HBP/SLBP is involved in post-transcriptional control of histone gene expression. In vitro assays have demonstrated that human HBP/SLBP is involved in histone mRNA 3′ end formation and translation. We have inhibited human HBP/SLBP expression by RNA interference to determine its function during the mitotic cell cycle. Inhibition of HBP/SLBP expression resulted in the inhibition of histone gene expression and DNA synthesis, the inhibition of cell cycle progression in S phase and the inhibition of cell proliferation. These findings indicate that human HBP/SLBP is essential for the coordinate synthesis of DNA and histone proteins and is required for progression through the cell division cycle.
Progression through the mitotic cell cycle requires the duplication of DNA and histone protein content during S phase. Histone proteins are required for the packaging of DNA into chromatin. This is essential for chromosome maintenance and replication and the regulation of gene expression. In metazoans, histone proteins are provided by the expression of the multicopy replication-dependent histone genes. The expression of these genes is coordinated with DNA synthesis and is restricted to S phase by the modulation of mRNA levels, resulting in approximately 35- to 50-fold higher levels of histone mRNA during S phase (Schümperli, 1988; Marzluff and Duronio, 2002). The histone hairpin binding protein HBP/SLBP (hereafter referred to as HBP) is involved in the control of histone gene expression (Wang et al., 1996; Martin et al., 1997). HBP is an S-phase protein whose expression is controlled by translational activation of HBP mRNA in late G1 phase and HBP destruction at exit from S phase (Whitfield et al., 2000; Zheng et al., 2003). HBP binds to the highly conserved hairpin structure found in the 3′ untranslated region (3′UTR) of replication-dependent histone mRNA. The hairpin structure is required for histone-specific RNA 3′ end formation, translation and for the regulation of mRNA stability (Müller and Schümperli, 1997).
Biochemical studies have demonstrated that HBP is required for the cell cycle-regulated histone mRNA 3′ end formation. Histone mRNA ends are formed by the cleavage of pre-mRNA 3′ of the hairpin structure by an unknown nuclease. The nuclease is positioned by a complex composed of HBP (Wang et al., 1996; Martin et al., 1997), the U7 snRNP and a Zn-finger protein (reviewed by Müller and Schümperli, 1997; Dominski and Marzluff, 1999; Marzluff and Duronio, 2002). The complex interacts at two sequence elements with the premRNA: (i) the RNA binding protein HBP binds specifically to the conserved histone RNA hairpin structure (Michel et al., 2000; Battle and Doudna, 2001; Zanier et al., 2002) and (ii) U7 snRNP interacts with a sequence element downstream of the hairpin by base-pairing (Schaufele et al., 1986). After mRNA cleavage, HBP remains associated with histone mRNA and stimulates translation (Ling et al., 2002; Sanchez and Marzluff, 2002). It has been proposed that the limitation of HBP expression to S phase is instrumental for the restriction of histone gene expression to S phase (Whitfield et al., 2000; Zheng et al., 2003).
HBP is a single-copy gene in humans, Drosophila melanogaster and Caenorhabditis elegans and is essential for development in Drosophila and C. elegans (Sullivan et al., 2001; Kodama et al., 2002; Pettitt et al., 2002). Histone mRNA 3′ end formation is disturbed in Drosophila Hbp mutants, resulting in the inhibition of histone synthesis. Similarly, histone synthesis is inhibited in C. elegans lacking CDL-1, the C. elegans HBP orthologue. Lack of maternal HBP leads to developmental arrest at an early stage in both organisms after several cell cycles. Our knowledge of the function of human HBP is based on studies with cell free systems or is inferred from observations in other model organisms. The biological role of this protein in mitotic cells has not been directly addressed. We present the results of an investigation of human HBP function during the mitotic cell cycle using RNA interference (RNAi) to inhibit HBP expression. The inhibition of HBP expression resulted in the inhibition of histone gene expression and DNA synthesis, inhibited progression through the cell division cycle and prevented cell proliferation. Our observations demonstrate that HBP is an essential protein required for histone and DNA synthesis and is indispensable for cell cycle progression and cell proliferation.
Materials and Methods
Constructs for RNA interference
The human U6 promoter region from -265 to +1 was PCR amplified from human DNA and inserted into pGEM-T Easy (Promega), resulting in plasmid pGEM-U6P. Constructs expressing shRNAs for RNA interference were derived from pGEM-U6P by PCR using the SP6 primer and a downstream primer encompassing the 3′ end of the U6 promoter, an inverted repeat encoding the shRNA, a TTTTT terminator signal and a MluI restriction site (Paddison et al., 2002). The PCR fragments were inserted into pGEM-T Easy and then either used directly, excised as cassette with MluI, or inserted as MluI fragment into the unique MluI site of pEGFP-C3 (Clontech). The shRNAs HP1, HP2, HP3 and cHP were expressed from the cassettes U6pHP1, U6pHP2, U6pHP3 and U6cHP, respectively. shRNAs HP1, HP2, HP3 target different regions of the HBP open reading frame and cHP was a control derived from HP1 (Fig. 1A). U6pT was used as a further control and contained the U6 promoter followed by the TTTTT terminator sequence.
Cell culture conditions
HeLa cells (a gift from N. Proudfoot, University of Oxford) were grown under standard conditions (5% CO2, 37°C) in DMEM supplemented with 10% fetal calf serum, 100 units/ml penicillin and 100 μg/ml streptomycin (Gibco-BRL).
RNA interference procedure
HeLa cells were seeded 60% confluent and grown until >90% confluent. Transfections were then carried out using lipofectamine 2000 (Life Technologies) according to the manufacturer's instructions. Transfection efficiency was monitored in parallel transfections with pEGFP-C3 (Clontech). EGFP expression was detected by fluorescence microscopy and was routinely between 50% and 70%. When RNA interference was done with pEGFP-derived plasmids, transfection efficiency was determined directly using EGFP expression as an indicator. Subsequently, cells were diluted 1:3 6-12 hours after transfection, and were then analysed at the indicated times post transfection. For treatment with hydroxyurea, HeLa cells were diluted 12 hours after transfection and then treated with 2 mM hydroxyurea (HU; Sigma) after a further 12 hours. After 16 hours HU treatment cells were washed with fresh medium and released into S phase. For mitotic arrest, cells were treated with 40 ng/ml nocodazole for 12 hours. Mitotic cells were harvested by shake-off, collected by centrifugation, washed once with PBS and released into fresh medium. Cells were transfected 1 hour after release, and washed with PBS 8 hours after release to remove unattached cells.
Antibodies and western blotting
Polyclonal rabbit anti-HBP antibodies were raised against peptide CLTEPLRDFSAMS coupled to KLH. Other antibodies used were mouse anti-tubulin monoclonal antibody (Sigma), rabbit polyclonal anti-cyclin A antibody (#06-138; Upstate Biotechnology). Secondary anti-rabbit and anti-mouse antibodies coupled to horseradish peroxidase were purchased from Sigma and Amersham Pharmacia Biotech. For protein analysis, HeLa cells were collected, washed once in phosphate-buffered saline (PBS), and lysed in 1% sodium dodecyl sulphate by boiling for 5 minutes. Lysates were fractionated by SDS-PAGE and transferred onto Hybond-P membrane (Amersham Pharmacia Biotech) by electroblotting. Probing with antibodies was done using standard protocols and detection was by chemiluminescence (ECL, Amersham Pharmacia Biotech). Between probing, blots were stripped using standard protocols. Recombinant HBP (rHBP) was expressed in insect cells using a baculovirus expression system as described previously (Martin et al., 2000).
Total RNA was prepared using Trizol reagents (Gibco-BRL) according to the manufacturer's instructions. Normally 10-15 μg total RNA was fractionated by electrophoresis through glyoxal agarose gels and transferred onto Hybond-N membrane (Amersham Pharmacia Biotech) by capillary transfer and UV cross-linked to the membrane. mRNAs were detected by hybridisation with 32P-labelled DNA probes prepared by the random prime labelling method (Roche). Hybridisation was according to standard procedures (Church and Gilbert, 1984). Probes were the human HBP cDNA NcoI fragment (Martin et al., 1997), a histone H2BJ-fragment excised with BamHI and HindIII from plasmid H2B-CYFP (a gift from Dr I. Ellenberg, EMBL) and human histone H2AC, H3A, H4A and H1C DNA fragments spanning nucleotides 15-392, 1-380, 57-312, 1-619 of the open reading frame, respectively. The H2AC, H3A, H4A and H1C fragments were amplified by PCR, inserted into pGEM-T Easy and released by restriction with EcoRI. 32P-end-labelled oligonucleotide ACGGTATCTGATCGTCTTCGAACC was used to detect 18S rRNA. Between probings, blots were stripped using standard protocols. RNAs were visualised by autoradiography or using a Fujifilm FLA3000 Phosphoimager and analysed using Aida 2.0 software (Raytest GmbH).
To analyse cell cycle progression, cells were stained with propidium iodide (Spector et al., 1998). Control samples of asynchronous HeLa cells were used to define ranges for peaks with G0/G1 and G2/M-phase cells, and S-phase cells with intermediate DNA content were between these peaks. Sub-G1 cells were from 0 to the lower boundary of the G0/G1 range. The settings were transferred to the test samples and the percentage of cells in each phase was calculated using CellQuest software and is given as the percentage of the gated population of cells. To characterise DNA synthesis during S phase, DNA synthesis and DNA content were determined by pulse-labelling with BrdU for 30 minutes and by staining with 7-amino-actinomycin D, respectively, using the BrdU Flow Kit according to the instructions of the manufacturer (BD Biosciences). Data analysis was done using CellQuest software. FACS analysis was done with a FACS Calibur Cytometer at the Aberdeen University Flow Cytometry Facility.
Colony forming assay
Confluent HeLa cells were transfected with 5 μg DNA in 6-well plates. 12 hours after transfection, cells were detached and resuspended in 8 ml of medium. 0.5 ml of the cell suspension (containing 1.2×105 cells) was then seeded in wells of 24-well plates. After further 12 hours, G418 was added to a final concentration of 1.5 mg/ml. At the indicated times, cells were washed with PBS, fixed with ethanol for 2 minutes, stained with 0.2% crystal violet for 2 minutes and washed twice with PBS. 24-well plates were visualised using a Zeiss STEMI-2000-C dissection microscope and images were recorded using Optronics Magnafire-SP equipment (Optronics).
The functional characterisation of HBP in vitro has shown that HBP is a central regulator of histone gene expression in metazoans. To investigate the role of HBP during the mitotic cell cycle we prepared constructs for the inhibition of HBP expression by RNAi. We expressed short hairpin RNAs (shRNAs) (Paddison et al., 2002) HP1, HP2 and HP3 that target human HBP mRNA for degradation by RNAi from cassettes composed of the U6 promoter, the sequence coding for the shRNA and an RNA polymerase III terminator sequence. The cassettes were produced by PCR amplification from pGEM-U6P, a pGEM vector containing the U6 RNA promoter and the amplification products were re-inserted into pGEM-T Easy. For the PCR amplification we used the SP6 primer as upstream primer, in combination with downstream primers that overlapped the end of the U6 promoter region and encompassed the shRNA coding sequence followed by a termination signal for RNA polymerase III and a MluI restriction site. For transfection into HeLa cells we used either the pGEM-T Easy derivatives, the cassettes excised with MluI or the MluI fragments inserted into pEGFP-C3. The structure of these cassettes is shown in Fig. 1A. We used several shRNAs to exclude the possibility that our results were due to off-target effects of a particular construct (Jackson et al., 2003; Scacheri et al., 2004) and the regions of the HBP/SLBP mRNA targeted by the shRNAs as well as the shRNA sequences are shown in Fig. 1A. As additional controls we used either the U6 promoter cassette (Up6), a U6 promoter-terminator cassette (U6pT) that lacks any shRNA sequence, or a construct expression cHP, a variant of HP1 that is changed by point mutations at two positions and is therefore not targeting the HBP mRNA any more.
To detect HBP expression we used a polyclonal rabbit anti-HBP serum raised against a C-terminal epitope of human HBP. Fig. 1B shows that the anti-HBP serum recognised endogenous HBP migrating with the mobility of a ∼42 kDa protein in HeLa cell extract. Recognition of HBP was specific as this protein was not detected when the incubation with the primary antibody was omitted or when the primary antibody was preincubated with the antigen peptide. Other bands were non-specific as they appeared with all combinations of primary and secondary antibodies. To test for the inhibition of endogenous HBP expression, 90% confluent HeLa cells were subjected to HBP RNAi by transfection with U6pHP1, U6pHP3 or with the controls U6p and U6pT in pGEM, or subjected to a mock transfection procedure without DNA. The cells were then diluted to allow for growth and after 24 hours protein extracts were analysed by probing western blots with anti-HBP serum. Fig. 1C,D shows that HBP levels were clearly reduced in U6pHP1- and U6pHP3-treated cells, compared to mock-transfected and control-transfected cells. As RNAi inhibits gene expression by targeting mRNA for degradation, we investigated the effect of our treatment on HBP mRNA levels by transfecting HeLa cells with the U6pHP1, U6pHP2 or U6pHP3 cassettes or the control U6pT and U6pcHP cassettes. RNA samples were prepared 24 hours after transfection and analysed by northern blotting. Fig. 2A shows a near twofold reduction of HBP expression in U6pHP1-, U6pHP2- and U6pHP3-treated cells compared to cells treated with the two control cassettes, indicating that the cassettes are sufficient to specifically inhibit HBP expression. As HBP is implicated in S-phase-specific histone gene expression, we also investigated the effect on the expression of histone H3 and found that histone H3 mRNA levels were reduced to a similar extent as HBP expression (Fig. 2A). To investigate this link between HBP expression and histone gene expression in more detail we compared HBP and core histone and linker histone mRNA levels in U6pHP1 and control treated cells. HBP mRNA levels in cells subjected to RNA interference were reduced by ∼50% 24 hours and 48 hours after transfection when compared to the mock-transfected or U6pT-transfected controls (Fig. 2B,C). The treatment with U6pHP1 led to a corresponding reduction of histone H2A, H2B, H3, H4 and H1 mRNA levels and was similar to the transfection efficiency in these experiments (60%). We conclude that the expression of HBP is a prerequisite for histone gene expression.
Histone gene expression is required for cell division. To test whether HBP expression is also required for cell proliferation we performed colony-forming assays. The U6pT, U6pcHP, U6HP1, U6pHP2 and U6HP3 cassettes were inserted as MluI fragments (Fig. 1A) into the vector pEGFP-C3 at the unique MluI restriction site that lies outside the regions required for neomycin phosphotransferase gene and EGFP expression and DNA replication (Fig. 3A). The resulting plasmids carry the neomycin resistance gene, which allows for the selection of transfected cells using G418. Fig. 3B shows that G418 selection effectively killed mock-transfected cells within 3 days. HeLa cells transfected with pEGFP-Up6T and -U6pcHP, on the other hand, were able to grow and formed clearly visible colonies within 3 days that grew further in the next 4 days, indicating that the introduction of the cassette and the expression of the control hairpin did not prevent cell division. In contrast, treatment with pEGFP-Up6HP1, -U6pHP2 or -U6pHP3 resulted in a pronounced inhibition of proliferation and no colony growth was observed in these cultures. But some cells persisted up to the 7-day time point in these cultures and inspection by microscopy showed that these were mostly single cells that were unable to undergo cell division (data not shown). As only transfected cells survive the treatment with G418, this indicates that the inhibition of HBP by shRNA expression from the pEGFP plasmids carrying the resistance gene resulted in a specific inhibition of cell proliferation. These data indicate that HBP is required for progression through the cell division cycle. We therefore tested the effect of inhibition of HBP expression on cell cycle progression and observed a reduction in the S-phase cell population in asynchronous cells (data not shown).
We then analysed cell cycle progression using HeLa cells arrested in mitosis by treatment with nocodazole. 1 hour after release from nocodazole, cells were transfected with either pGEM-U6pHP1 or pGEM-U6pT or mock transfected. The cell cycle distribution was then analysed 8, 10, 12, 14, 16 and 26 hours after release. Cell cycle progression of transfected cells was identical up to 16 hours and therefore only selected time points are shown in Fig. 4. A substantial proportion of mock-treated cells had entered S phase 16 hours after release. Most cells had gone through mitosis 26 hours after release and were no longer synchronised. Up to the 16-hour time point, cells treated with both U6pHP1 or Up6T cassettes were similarly delayed compared to the mock-treated cells, presumably because of the transfection with DNA. At the final 26-hour time point, the proportion of S-phase and G2/M-phase cells in U6pHP1-treated cells was reduced compared to the U6pT-treated cells, indicating that progression into S phase was inhibited. This was accompanied by an accumulation of sub-G1 cells. Sub-G1 cells were also observed in control-transfected cells, but as the proportion of sub-G1 cells was significantly higher in cells transfected with U6pHP1, we conclude that inhibition of HBP expression led to cell death.
This led us to investigate the effect of inhibition of HBP expression on S-phase progression. Cells were transfected with pGEM-U6pHP1 or pGEM-U6pHP3 or the control plasmids pGEM-U6pT and pGEMU6cHP and then arrested by addition of hydroxyurea (HU). HU treatment arrests cells at G1/S-phase transition or during S phase and inhibits histone gene expression, but has no adverse effect on HBP expression (Whitfield et al., 2000). Subsequent to the arrest, cells were released and cell cycle progression was monitored. As shown in Fig. 5, RNAi with U6pHP1 and U6pHP3 delayed progression through S phase compared to the two control treatments, and ∼1.5 times more cells had still G0/G1-phase DNA content 7 hours after release. To follow cell cycle progression in more detail, we compared the progression of cells transfected with either U6pHP1 or U6pT plasmids at shorter intervals after release from block with HU. Fig. 6 shows that the majority of U6pT-transfected cells were in mid-S phase 3 hours after release and had progressed to late S phase in the following 5 hours. 16 hours after release, the majority of cells had advanced to late S phase, G2/M phase or G0/G1 phase. In comparison, cell cycle progression of most U6pHP1-transfected cells was delayed for up to 5 hours. At 8 hours the majority of cells were approaching mid-S phase, and after 16 hours a significant fraction of cells remained that had S-phase DNA content. During this time we did not observe significant cell death caused by HBP RNAi (data not shown), indicating that the changes in cell cycle progression were not due to HBPRNAi-mediated cell death. To determine whether the cell cycle progression of U6pHP1-treated cells was associated with a change in HBP expression we tested HBP levels at selected time points. As shown in Fig. 6C, HBP expression was inhibited at all time points tested up to 16 hours, indicating that the cells entered S phase despite a lack of HBP expression. This suggests that inhibition of HBP expression delays, but does not prevent cell cycle progression into S phase in HeLa cells. In addition we investigated the expression of cyclin A as a marker for transition into S phase. Fig. 6C shows that cyclin A expression was equal in the 0-hour samples, but then increased in the control-treated samples, compatible with the progression through S phase observed. After 8 hours, cyclin A levels were similar in U6pHP1- and U6pT-treated cells, and the increase in cyclin A in U6pHP1-treated cells was in agreement with the cell cycle progression observed. Cyclin A is also involved in mitosis. At the 16-hour time point, cyclin A levels in U6pT-treated cells were high, presumably reflecting the high proportion of G2/M phase cells in this sample. Although the cell cycle analysis of HBP RNAi-treated sample revealed that ∼50% of cells were in S phase at this time point, cyclin A levels were markedly lower in these cells. The molecular mechanism resulting in the low cyclin A levels in these cells is not clear but we believe that this is linked to an inefficient progression through S phase in HBP RNAi-treated cells. Cyclin A expression and histone gene expression are required for DNA synthesis and are inhibited by HBP RNAi. We therefore decided to test whether HBP expression is required for DNA synthesis. We observed that HBP RNAi resulted in an approximate twofold reduction of DNA synthesis in asynchronous HeLa cells (data not shown). To investigate this in more detail we tested whether U6pHP1-treated cells arrested by treatment with HU were able to resume normal DNA synthesis upon removal of HU. DNA synthesis was measured by pulse labelling with BrdU and DNA content was analysed by staining with 7-amino-actinomycin D followed by FACS analysis. The data in Table 1 shows the percentage of cells that incorporated BrdU and the percentage of cells with S-phase DNA content. The ratio of these two values is a measure of DNA synthesis activity during S phase. As shown in Table 1 DNA synthesis is at similarly low level immediately after removal of HU in both U6pHP1 and control-treated cells. However, at later time points the delayed cell cycle progression of cells lacking HBP is accompanied by two- to sixfold lower DNA synthesis, demonstrating that the inhibition of HBP expression results in the inhibition of DNA synthesis.
|Time (hours) .||.||% Cells synthesising DNA (A) .||% Cells with S phase DNA content (B) .||A/B* .|
|Time (hours) .||.||% Cells synthesising DNA (A) .||% Cells with S phase DNA content (B) .||A/B* .|
Cells were transfected with either pGEM-U6pT or pGEM-U6pHP1, treated with HU and subsequently released and analysed as described in Materials and Methods. *The A/B ratio is an indicator of DNA synthesis activity in S-phase cells. Results are representative of two independent experiments.
We used RNA interference to investigate the role of human HBP during the mitotic cell cycle. We demonstrate that the expression of shRNAs that target HBP mRNA for degradation inhibited HBP expression, and this inhibition resulted in (i) the reduction of histone gene expression, (ii) the inhibition of DNA synthesis; (iii) the inhibition of cell cycle progression during S phase; and (iv) the inhibition of cell proliferation. This indicates that the expression of HBP is required for cell division and is a prerequisite for histone and DNA synthesis, two coordinated processes essential for normal cell cycle progression.
We observed these effects independently with two or three shRNAs targeting different regions of the HBP open reading frame, indicating that the effects are due to the inhibition of HBP expression and not caused by off-target activity of a particular shRNA. As we used transient transfection, our experimental protocol was limited by the transfection efficiency of the cells used. However, we were routinely able to transfect between 50% and 70% of cells and therefore conclude that the corresponding reductions in histone and HBP mRNA levels, the clear effects on cell cycle progression and the severe inhibition of DNA synthesis observed were caused by the inhibition of HBP expression.
The analysis of cell cycle progression by FACS revealed in some but not all experiments a rapid accumulation of sub-G1 cells, indicating that the inhibition of HBP RNAi can result in cell death (Fig. 4). We also observed sub-G1 cells when incubation time was extended further in experiments using HU to arrest cells. Our data are compatible with cell death being a consequence of the inhibition of cell cycle progression in cells lacking HBP. However, we are currently not sure about the nature of the cell death observed.
Inhibition of HBP expression resulted in the repression of histone gene expression. The mechanism leading to this repression is not known. It can be accounted for by a lack of transcription or a defect in RNA 3′ end formation resulting in mRNA decay in HBP RNAi-treated cells. In yeast, defects in mRNA 3′ end formation destine mRNAs for decay by the nuclear exosome (Hilleren et al., 2001) and there is evidence for the existence of a similar process in mammalian cells (Moore, 2002). However, such a rapid degradation of misprocessed histone mRNA, resulting from the inhibition of HBP expression, would be in contrast to the situation in Drosophila embryos where a lack of HBP has been found to result in longer polyadenylated mRNA that was formed by using a polyadenylation signal downstream of the hairpin for end formation (Lanzotti et al., 2002). Alternatively, it is possible that transcription was inhibited by a feedback mechanism linking histone and DNA synthesis. Such a feedback mechanism was first proposed to account for reduction of histone mRNA when cells cease DNA synthesis (Butler and Mueller, 1973; Sariban et al., 1985; Peltz and Ross, 1987). Finally, our data do not exclude the formal possibility that HBP is required for cell cycle progression in late G1 phase, independent of histone gene expression.
Our experiments demonstrate a stringent requirement of cell cycle progression for HBP expression. HBP RNAi inhibited cell cycle progression into and through S phase (Figs 4, 5, 6) and resulted in a severe reduction of DNA synthesis (Table 1). This is in contrast to the more relaxed requirement for HBP during the early development of Drosophila and C. elegans where several cell cycles occurred in the absence of HBP (Sullivan et al., 2001; Kodama et al., 2002; Pettitt et al., 2002). However, the cell divisions in these animal models were not normal and nuclei were enlarged, compatible with a decondensation of chromatin caused by the lack of histones. It is probable that these cell cycles occurred because of a relaxed cell cycle control during early development of the model animals. In contrast, in mitotic cells the requirement for HBP, presumably in its role as regulator of histone gene expression, is such that cell cycle progression is immediately affected, reflecting the more stringent control of cell cycle progression in mitotic cells.
Coupling of DNA and histone synthesis has been previously reported, but the molecular links between these two processes are not well understood. It is well documented that the inhibition of DNA synthesis results in a rapid inhibition of histone gene expression (Heintz et al., 1983; Graves and Marzluff, 1984; Baumbach et al., 1984). This led to the proposal of an auto-regulatory feedback mechanism that controls histone mRNA abundance in response to excess histones that accumulate when cells stop DNA synthesis (Butler and Mueller, 1973; Heintz et al., 1983; Sariban et al., 1985; Peltz and Ross, 1987). More recently, it was demonstrated that the inhibition of DNA synthesis due to ionising irradiation resulted in the inhibition of histone gene expression in a p53/p21-dependent manner (Su et al., 2004). However, the requirement of DNA synthesis for histone gene expression has been more difficult to explore. Recent work has demonstrated that the transcription activator of histone genes NPAT/p220 is required for the transition from G1 into S phase (Wei et al., 2003; Ye et al., 2003). Furthermore, the inhibition of histone gene transcription by overexpression of the repressor HIRA resulted in the inhibition of DNA synthesis (Nelson et al., 2002). This inhibition was overcome when histone mRNA levels were increased by the overexpression of HBP (Nelson et al., 2002). Our work demonstrates that HBP expression is a prerequisite for both histone and DNA synthesis. It identifies a new link between the machinery controlling histone gene expression and DNA synthesis and future experiments will address the nature of the molecular mechanisms linking these two processes. In conclusion, we have demonstrated that human HBP is an essential protein required for histone gene expression, DNA synthesis, cell cycle progression and cell proliferation.
We thank Carl Smythe for helpful suggestions and discussion. We are grateful to Olivier Urwyler and Orestys Argyros for the preparation of constructs, and the Aberdeen University FACS Facility for help and advice. The work was supported by the Wellcome Trust, the EC Framework 5 programme, the University of Aberdeen and Tenovus Scotland.