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PLoS One. 2010; 5(12): e14335.
Published online 2010 December 14. doi:  10.1371/journal.pone.0014335
PMCID: PMC3001870

Histone Deacetylase Inhibitors Downregulate Checkpoint Kinase 1 Expression to Induce Cell Death in Non-Small Cell Lung Cancer Cells

Rory Edward Morty, Editor



Histone deacetylase inhibitors (HDACis) are promising anticancer drugs; however, the molecular mechanisms leading to HDACi-induced cell death have not been well understood and no clear mechanism of resistance has been elucidated to explain limited efficacy of HDACis in clinical trials.

Methods and Findings

Here, we show that protein levels of checkpoint kinase 1 (Chk1), which has a major role in G2 cell cycle checkpoint regulation, was markedly reduced at the protein and transcriptional levels in lung cancer cells treated with pan-and selective HDACis LBH589, scriptaid, valproic acid, apicidin, and MS-275. In HDACi treated cells Chk1 function was impaired as determined by decreased inhibitory phosphorylation of cdc25c and its downstream target cdc2 and increased expression of cdc25A and phosphorylated histone H3, a marker of mitotic entry. In time course experiments, Chk1 downregulation occurred after HDACi treatment, preceding apoptosis. Ectopic expression of Chk1 overcame HDACi-induced cell death, and pretreating cells with the cdc2 inhibitor purvalanol A blocked entry into mitosis and prevented cell death by HDACis. Finally, pharmacological inhibition of Chk1 showed strong synergistic effect with LBH589 in lung cancer cells.


These results define a pathway through which Chk1 inhibition can mediate HDACi-induced mitotic entry and cell death and suggest that Chk1 could be an early pharmacodynamic marker to assess HDACi efficacy in clinical samples.


Histone deacetylase inhibitors (HDACis) represent a promising new class of compounds for the treatment of cancer [1]. Some HDACis show broad activity against multiple HDAC classes (scriptaid, LBH589), whereas others are class-or isotype selective (MS-275) [1], [2].

The precise mechanisms by which HDACis exert their cytotoxic effects are unknown; however, the antitumor effects of these drugs are thought to result from hyperacetylation of histones, demethylation of genomic DNA, and activation of genes that inhibit proliferation and induce apoptosis [1]. In addition to their epigenetic effects, HDACis have also been shown to have significant post-translational effects on non-histone proteins, including transcription factors p53, heat-shock protein 90 (HSP90), and α-tubulin [3]. Besides direct anti-tumorigenic effects, suppression of angiogenesis by HDACis might also have an impact on tumor growth inhibition [4].

An essential regulatory step for the G2/M cell cycle transition in eukaryotes is activation of the cdc2-cyclin B complex [5]. The proper regulation of cdc2 requires an activating phosphorylation on threonine-161 and inhibitory phosphorylations on threonine-14 and tyrosine-15 (Tyr15) [6]. The inhibitory phosphorylation on Tyr15 maintains the cdc2-cyclin B complex in an inactive state if there is incompletely replicated DNA or damaged DNA in the cell [7], [8]. Cdc2 activation through removal of its inhibitory phosphorylation by cdc25 phosphatases allows cells to enter the mitotic phase of the cell cycle [9]. Chk1 is a critical component of DNA replication, intra-S phase, G2/M phase, and mitotic spindle-assembly checkpoints [10]. In response to a variety of genotoxic stressors, Chk1 becomes activated by upstream kinases such as ATM and ATR, leading to increased proteosomal degradation of the phosphatase cdc25A and inhibition of cdc25C through serine-216 (Ser216) phosphorylation, collectively causing inactivation of cdc2 and consequently G2/M arrest [10][14].

Furthermore, combining HDACis with regulators of G2 checkpoint could improve efficacy and aid in overcoming resistance. In fact, direct pharmacologic inhibition or siRNA knockdown of Chk1 has been shown to cause checkpoint abrogation, cytokinetic regression, and multinucleation, as well as chromosome missegregation and chromosomal instability [15]. Therefore, Chk1 inhibitors, which effectively abrogate the S and G2 checkpoints, are being investigated in clinical trials either alone or in combination with cytotoxic agents [16][18] and could be effectively combined with HDACi to enhance cytotoxic effects.

Here, we demonstrate that HDACi treatment downregulates Chk1 protein expression, which in turn leads to unscheduled cdc2 activation, mitotic entry, and cell death in human lung cancer cells. The results of this study demonstrate that Chk1 downregulation and abrogation of G2 checkpoint are important regulatory steps in sensitivity and resistance to the cytotoxic effect of HDACi treatment in non-small cell lung cancer (NSCLC) cells. Our data suggest that Chk1 might be an early pharmacodynamic marker to predict and assess the efficacy of HDACis and Chk1 inhibitors may enhance cytotoxic effects of HDACis in clinical studies.


Treatment of NSCLC cells with HDACis causes G2/M cell cycle arrest and cell death

Previous studies have demonstrated that a pan-HDACi LBH589 (IC50 ranging between approximately 9 and 54 nmol/L) causes growth arrest and cell death in NSCLC cells [19]. To analyze the molecular mechanisms by which HDACis regulate cell cycle progression and cell death, asynchronously growing A549 (EGFR wild type, K-Ras mutant, and p53 wild type) and PC9 (EGFR mutant, K-ras wild type, and p53 mutant) [20][22] cells were treated with LBH589 (40 nM) for 24 hours and collected for flow cytometric analysis. Figure 1 shows that in PC9 and A549 cells LBH589 treatment produced a noticeable increase in the cells in the G2/M phase suggestive of a G2/M blockade and a significant reduction in S-phase cells. These results are in agreement with the previous reports that HDACis lead to G2/M arrest and apoptotic cell death in NSCLC cells [19].

Figure 1
Effect of LBH589 on cell cycle distribution of A549 and PC9 cells.

As illustrated in Figure 2A, microscopic examination of cells treated with LBH589 produced a range of different nuclear morphologies, from binucleation to multinucleation. Taken together, these data show that LBH589 treatment causes cell death associated with abnormal mitosis and failed cytokinesis, which is suggestive of mitotic catastrophe, a type of cell death that occurs during mitosis and has previously been described in cells treated with the HDACi trichostatin A [23].

Figure 2
LBH589 treatment leads to mitotic abnormalities and cytokinesis failures.

Since cells in the G2- and M-phase could not be discriminated based on their differences in DNA content by flow cytometric analysis, we tested whether cells arrested in G2/M after HDACi treatment enter mitotic phase. For this purpose, we first performed immunofluorescence staining using the antibody against cleaved poly(ADP-ribose) polymerase (cPARP) and showed that LBH589 treatment causes apoptotic cell death in 78% of binucleated mitotic cells (Figure 2B). Next, in Western blot analysis we tested whether HDAC inhibition enhances histone H3 phosphorylation at serine-10, which takes place at the onset of mitosis. Figure 2C illustrates that LBH589 treatment caused histone H3 phosphorylation accompanied by increased histone acetylation and PARP cleavage, indicating that HDACi treatment causes NSCLC cells to enter mitosis and undergo cell death. To determine whether cell growth and viability changes observed after LBH589 treatment are a generalized effect of HDAC inhibition, we also used another pan-HDACi, scriptaid (1 µM), which produced biochemical changes indistinguishable from those presented above using LBH589 (Figure 3).

Figure 3
HDACi treatment specifically inhibits CHK1 expression and upregulates its downstream signaling proteins CDC25A, CDC25C, and CDC2, involved in G2 cell cycle checkpoint control.

HDAC inhibition results in activation of cdc25 and cdc2 proteins that are required for mitotic entry

Activation of the cdc2 protein kinase by the cdc25 protein phosphatases is a pivotal regulatory step for the G2/M transition in eukaryotes [9]. The dephosphorylation of cdc25C on Ser216 increases its activity during M-phase transition, leading to activation of the cdc2 kinase [10]. To investigate whether HDACi-induced mitotic entry and cell death are mediated by activation of the cdc25/cdc2 pathway, PC9, A549, H1299, H292, H358, H441 and HCC827 cells were treated with or without LBH589, and Western blot analysis was performed. Figure 3A shows HDACi treatment resulted in increased levels of PARP cleavage, a decrease in the inhibitory phosphorylation on cdc2 and 45–94% decrease (based on quantitative Western blot analysis) in total Chk1 across the 7 different NSCLC cell lines, with A549s showing the most significant decrease in Chk1 protein. These changes are all associated with an increase in histone acetylation. Further investigation of A549 and PC9 cells treated with pan HDACis (Figure 3B), LBH589 and scriptaid, showed activation of cdc25C and cdc2, as assessed by a decrease in their inhibitory phosphorylation on Ser216 and Tyr15, respectively, which were accompanied by increased histone H4 acetylation. No decrease was observed in the expression levels of total cdc25C and cdc2 proteins (Figure 3B). These results indicate that HDACi-induced mitotic entry is mediated by increased cdc25/cdc2 activity. Furthermore, HDACi treatment also increased the expression level of cdc25A, which is targeted by Chk1 for rapid degradation (Figure 3B). These data show that, in HDACi-treated cells, the biologic function of Chk1 was inhibited.

Besides phosphorylation at the Tyr15 position, another major mechanism regulating cdc2 activity and progression into mitotic phase of the cell cycle is its complex formation with cyclin B, a required cofactor for the cdc2 kinase activity. Thus, we next determined whether HDACi treatment affects cyclin B expression levels. As shown in Figure 3B, NSCLC cells treated with LBH589 or scriptaid displayed higher overall levels of cyclin B1 expression. Taken together with the decreased Tyr15 phosphorylation of cdc2, this finding implies a high cdc2-cyclin B activity in HDACi-treated cells, providing further support that cells treated with HDACis are capable to enter mitosis.

Inhibition of HDAC activity correlates with decreased Chk1 expression in NSCLC cells

The order and fidelity of the cell cycle are linked to the integrity of the Chk1 and cdc25 phosphatase pathways. Maintenance of the Chk1/cdc25 pathway is essential for cells to progress normally through an unperturbed cell division cycle and for cells to arrest in response to checkpoint activation [10].

To determine the role of Chk1 in HDACi-induced activation of cdc25C and cdc2, we analyzed changes in the levels of Chk1 protein in cells treated with HDACis. Immunoblot analysis revealed that treatment with LBH589 or scriptaid causes a significant decrease in the expression of Chk1 protein (Figure 3C). This inhibition appears to be specific since no change was observed in the expression of Chk2 protein, another regulator of DNA-damage checkpoint signaling pathway [10], [11].

HDACis, including LBH589, have been reported to functionally inactivate HSP90 through protein acetylation, leading to depletion of the client proteins such as AKT and c-RAF [22]. Interestingly, Chk1 protein has also been reported to be an HSP90 client [24], [25], suggesting that inactivation of HSP90 by HDACis might be responsible for degradation of Chk1 observed in our experiments. To test this possibility, we analyzed whether Chk1 downregulation coincides with decreased expression of AKT and c-RAF in extracts prepared from cells treated with LBH589 or scriptaid. As illustrated in Figure 3C, no changes were observed in the expression levels of AKT or c-RAF proteins under the conditions where LBH589 and scriptaid caused Chk1 downregulation.

To further demonstrate the cytotoxic effects of HDACi treatment on NSCLC cells we measured apoptotic cell death using Annexin V detection. As shown in Figure 3D, PC9 and A549 cells showed a measured increase in the amount of annexin positive cells indicating that treatment with HDACi results in significant increase in cells undergoing apoptosis.

To determine whether selective HDACis also cause Chk1 inhibition, A549 and PC9 cells were treated with MS-275 that selectively inhibits HDAC1, and to lesser extent HDAC3. As illustrated in Figure 3E, MS-275 (0.5 µM) produced changes in the expression of Chk1, phosphorylated cdc2 (Tyr15), and cPARP similar to results observed with LBH589 and scriptaid. Two other class I HDACis valproic acid (1 mM) and apicidin (400 nM) also produced identical results (Figure 3E). These data demonstrate that HDACi-mediated Chk1 downregulation is not drug dependent and class I HDACs are likely mediators of the HDACi effect on Chk1 downregulation in NSCLC cells.

Chk1 abrogation precedes initiation of apoptosis by LBH589

Chk1 has been reported to be subject to caspase-mediated degradation in cells undergoing apoptotic cell death [26]. Consequently, we analyzed in time course experiments whether downregulation of Chk1 protein observed in HDACi-treated cells is the cause or the consequence of apoptotic cell death. As shown in Figure 4A, treatment of A549 cells with LBH589 led to a 70% decrease in Chk1 protein within 1 hour of treatment, based on quantitation of western blots, which was accompanied by decreased phospho-cdc25C (Ser216) and phospho-cdc2 (Tyr15) levels consistent with functional inactivation of Chk1 activity. Of importance, these changes occurred before detectable caspase activation, as evidenced by PARP cleavage that was first observed at 12 hours of treatment. A similar time course profile was observed in PC9 cells treated with LBH589 or scriptaid (data not shown).

Figure 4
A, HDACi-mediated decrease in CHK1 precedes apoptosis.

Collectively, these results support a model where inhibition of Chk1 expression by HDACis leads to cell death through unscheduled activation of the mitosis-promoting kinase cdc2 in NSCLC cells.

HDACi treatment leads to the transcriptional downregulation of Chk1

To determine whether HDACi treatment regulates Chk1 expression at the transcriptional level in NSCLC cells, we performed real-time PCR. As illustrated in Figure 4B, quantitative RNA analysis revealed more than a 50% reduction in Chk1 mRNA levels in A549 cells 24 hours after LBH589 (40 nM) treatment. This finding demonstrates that HDACi treatment leads to transcriptional repression of Chk1 in NSCLC cells.

Ectopic expression of Chk1 overcomes LBH589-induced apoptosis

To determine the importance of Chk1 downregulation in HDACi-induced apoptotic cell death, we aimed to determine whether ectopic expression of Chk1 can overcome cell death triggered by LBH589. Therefore, A549 cells were transiently transfected with a Chk1 plasmid encoding a GFP-tagged Chk1 fusion protein. As shown in Figure 4C, transient expression of ectopic Chk1 protein suppressed LBH589-induced apoptosis, as detected by PARP protein cleavage. Additionally, in cells expressing ectopic Chk1, LBH589 treatment failed to activate cdc2, as assessed by Tyr15 dephosphorylation (Figure 4C), while no changes were observed in HDACi-induced histone acetylation. Similar data were obtained with a Flag-tagged Chk1 expression plasmid in NSCLC cells (Figure 4C). These results indicate that Chk1 downregulation plays an essential role in HDACi-mediated cell death.

Chk1 downregulation correlates with apoptotic cell death in primary NSCLC cells treated with LBH589 ex vivo

To verify the downregulation of Chk1 in clinically relevant tumor samples, tumor cells collected from NSCLC patient tumors were treated ex vivo with LBH589. Total proteins were extracted, and drug-mediated changes in the expression of Chk1, histone acetylation, and PARP cleavage were analyzed by Western blot. As illustrated in Figure 4D, ex vivo treatment of cells with LBH589 (40 nM) caused increased histone H4 acetylation in all tumor samples, whereas, LBH589 treatment increased PARP cleavage in only 2 of 5 samples, which closely correlates with Chk1 downregulation. These results support the findings presented above with NSCLC cell lines and suggest that decreased Chk1 and phospho-cdc2 (Tyr15) levels may be sensitive pharmacodynamic markers for HDACi efficacy in patient tumor samples to predict and assess patient response to HDACi treatment in clinical studies.

HDACi-mediated cell death requires mitotic entry

The data presented above support a model where failure of Chk1-mediated checkpoint activation plays an essential role in HDACi-mediated cell death. Thus, we hypothesize that blockade of mitotic entry would diminish the sensitivity of cancer cells to the cytotoxic effects of HDACi treatment. To test this hypothesis, A549 cells were pretreated with a potent cdc2 inhibitor, purvalanol A [27], to block entry into mitosis. Flow cytometric analysis illustrates that 40 nM LBH589 for 24 hours caused a significant increase of cells in G2/M and an approximately 20-fold increase of the sub-G1 peak (hypodiploid cells) after 24 hours of treatment, consistent with increased cell death. The increase in the sub-G1 population after LBH589 treatment, however, was significantly reduced by pretreatment of cells with purvalanol A (Figure 5), indicating that mitotic blockade causes resistance to the cytotoxic effects of LBH589. To confirm this observation, we performed Western blot analysis with extracts prepared from A549 cells exposed to LBH589 with or without purvalanol A pretreatment. Figure 5 illustrates that purvalanol A pretreatment inhibited LBH589-induced apoptotic cell death, as measured by cPARP, providing further support that HDACi-induced cell death largely requires entry into mitosis.

Figure 5
Purvalanol A (Pur A) pretreatment diminishes the cytotoxic effect of LBH589 in A549 cells.

HDAC and Chk1 inhibitors show a synergistic effect in NSCLC cells

Our results showed that HDACi treatment targets Chk1 to induce inappropriate mitotic entry and thereby exerts its cytotoxic effects on tumor cells. The diminished sensitivity of cells to HDACi treatment observed in A549 cells ectopically expressing Chk1 (Figure 4C) suggests that activation of Chk1 and its downstream signaling pathway, which control the G2 check point, may cause resistance to HDACi therapy. Thus, it is plausible that Chk1 inhibitors may potentiate cytotoxic effects of HDACis in tumor cells that are resistant to HDACis. To test this possibility, A549 cells were treated with LBH589 and a Chk1 inhibitor (UCN-01) for 24 hours. Figure 6A shows that, at low concentrations, neither LBH589 (4 nM) nor UCN-01 (250 nM) alone can cause PARP cleavage in A549 cells, whereas the combination of these two drugs drastically increased PARP protein cleavage, suggesting a potential synergy. To corroborate the synergistic interaction between HDAC and Chk1 inhibitors, we next performed median dose effect analysis. For this purpose, A549 cells were exposed to increasing concentrations of LBH589, UCN-01 or the combination of these drugs in a fixed ratio. Cell viability was assessed using CT-Blue assay, and the effect was analyzed using median effect analysis. As shown in Figures 6B and 6C, exposure of cells to the combination of LBH589 and Chk1 inhibitors exerted a strong synergistic effect. Using these same methods, a synergistic interaction was also seen between LBH589 and a novel Chk1 inhibitor AZD7762 [28] in NSCLC cells that resulted in a CI value of 0.76 indicative of a moderately synergistic effect (data not shown).

Figure 6
LBH589 and Chk1 inhibitor treatment shows a synergistic effect in NSCLC cells.

The data presented above suggest that drugs inhibiting the activity of proteins that negatively regulate the function of cdc2-cyclin B complex may enhance the G2 checkpoint abrogation and cytotoxic effects of HDACis in tumor cells.


Previous studies have shown that HDACi-induced cell death is associated with aberrant mitosis and disruption of the cell cycle checkpoints [29][34]. However, the molecular mechanisms by which HDACi treatment leads to mitotic cell death is not well understood. Here, we demonstrated that HDACi treatment of human NSCLC cells leads to downregulation of total Chk1 protein levels. We showed that this downregulation is biologically relevant by demonstrating a concomitant decrease in the levels of the inhibitory phosphorylation of key cell-cycle regulatory proteins cdc25c and cdc2. The decreased levels of total Chk1 protein preceded induction of apoptosis and histone acetylation, demonstrating that Chk1 downregulation is an early event in HDACi mode of action and that it plays a pivotal role in drug-mediated cell death.

Chk1 expression has been shown to fluctuate during the cell cycle [35]. However, since Chk1 is mainly expressed at the S to M phase of the cell cycle at both the RNA and protein levels [35], it is unlikely that HDACi-mediated inhibition of Chk1 is a consequence of growth arrest in G2/M phase. RT-PCT experiments demonstrated that transcriptional inhibition of Chk1 plays an important role in HDACi-mediated regulation of Chk1 protein. The mechanism by which HDACis regulate the transcriptional expression of Chk1 is unknown and remains to be elucidated.

Treatment of tumor cells with pan HDACis has been reported to cause acetylation of Hsp90 through inhibition of HDAC6 and depletion of several Hsp90 client proteins including AKT and c-RAF [22], [36], [37]. Our results showed that under the conditions where LBH589 induced Chk1 downregulation, no inhibition was observed in the expression levels of AKT and c-RAF. Furthermore, selective HDAC inhibitors valproic acid, apicidin and MS-275 with no known inhibitory effects on HDAC6 were able to inhibit Chk1 expression. Taken together, these results suggest that inhibition of Chk1 expression in HDACi-treated cells is likely not mediated by inactivation of HSP90 protein, but is rather due to repression of CHK1 expression.

One of the major challenges in the development of HDACis is the definition of the clinically relevant endpoints to assess drug efficacy in patient tumors at the early stage of treatment to predict clinical outcome. In the present study, we showed that downregulation of total Chk1 protein levels correlates much more strongly with induction of cytotoxic effect rather than with histone hyperacetylation in both cell lines and in primary NSCLC cells obtained from patient tumors ex vivo. Together, these findings suggest that downregulation of Chk1 and Tyr15 phosphorylation of cdc2 levels may be sensitive and clinically relevant pharmacodynamic markers of efficacy of HDACis.

Despite their promise as an emerging cancer therapy, in clinical trials, the effectiveness of HDACis has been limited, and no clear mechanism of resistance has been elucidated [1]. Our present results provide a possible insight into the mechanism of HDACi action and resistance. We showed that ectopic expression of Chk1 and prevention of mitotic entry by a cdc2 inhibitor purvalanol A diminished LBH589-induced cell death. These findings suggest that the level of Chk1 expression or activation status of enzymes regulating the M-phase entry, such as cdc25 and cdc2-cyclin B complex, may play an important role in determining sensitivity or resistance of tumor cells to HDACis. The data presented here suggest a model where mitotic entry is a required step for HDACi-mediated cell death. Additionally, cellular mechanisms that block Chk1 downregulation and/or bypass Chk1 and directly act on G2 checkpoint control to prevent cells from entering mitotic phase would cause resistance to HDACis. For example, Chk1 has been shown to be highly expressed in NSCLC tumors [38], which may confer resistance to HDACi-induced mitotic entry and cell death. Thus, in tumors with increased Chk1 activity, rational combinations of HDACis with drugs that simultaneously inhibit Chk1 and its downstream signaling pathways controlling G2/M cell cycle checkpoint may augment the cytotoxic effects of HDACis.

HDACis have been shown to synergize with DNA damaging agents [1]. However, the molecular mechanisms of this synergy have not well been understood. Since Chk1 is crucial for the G2 checkpoint activation and survival after treatment with DNA damaging agents, we speculate that inhibition of Chk1 might provide a molecular explanation for the enhancement of tumor sensitivity to chemotherapeutic agents by HDACis. Further studies are required to elucidate the precise role of Chk1 in the synergistic interaction of HDACis with the cytotoxic therapies to enhance their therapeutic efficacy in cancer treatment.

Here, we provide evidence that HDAC and Chk1 inhibitors show strong synergistic interaction in NSCLC cells, providing the foundation for future clinical translation with HDACis and Chk1 inhibitors that are currently in clinical studies for anticancer therapy. We expect that validation of Chk1 and its downstream effectors involved in G2/M checkpoint control as clinically relevant biomarkers of treatment efficacy could provide tools applicable to the enrichment of clinical trials and, hopefully, individualized tailoring of therapy of NSCLC.

Materials and Methods

Cell culture and experimental treatments

A549, H1299, H358, H441, H292, HCC827 (ATCC, Manassas, VA) and PC9 cells (provided by Dr. Matt Lazzara, University of Pennsylvania, Philadelphia, PA) were grown in RPMI supplemented with 5% fetal calf serum (FCS), 1% (v/v) penicillin-streptomycin, and 1% (v/v) L-glutamine at 37°C in a 5% CO2 incubator. Stock solutions of the Chk1 inhibitors UCN-01 (EMD Biosciences, San Diego, CA) and AZD7762 (Selleck Chemical), HDACis scriptaid (BioMol International, Plymouth Meeting, PA), LBH589 (Novartis, Basel, Switzerland), apicidin (EMD Biosciences, San Diego, CA) and MS-275 (Selleck Chemical) were dissolved in DMSO and added to the media at the indicated concentrations. Stock solution of the HDACi valproic acid (EMD Biosciences) was dissolved in water and added to the media at the indicated concentrations. Control cells were treated with vehicle alone.

Ex vivo assays of primary NSCLC samples

Tumor cells were collected by fine needle aspiration technique, as previously described [39], from surgically resected Moffitt Cancer Center patient tumors. The tissue studies were approved by our Institutional Review Board at the University of South Florida. Briefly, tumor cells were obtained with sterile 23-gauge needles, and all samples were confirmed to be enriched for cancer cells by microscopic assessment. Approximately 25,000 tumor cells were treated in duplicate with vehicle (control) or LBH589 (40 nM) in a humidified 5% CO2 incubator at 37°C for 18 hours. No fibroblast or endothelial cell growth was observed. Following treatment, non-adherent and adherent cells (only a few, collected by scraping) were pooled together and centrifuged at 500×g for 5 minutes at 4°C. After they were washed with PBS, cells were lysed in 100 µL of ice-cold lysis buffer [50 mmol/L Tris-HCl, 0.25 mol/L NaCl, 0.1% (v/v) Triton X-100, 1 mmol/L EDTA, 50 mmol/L NaF, and 0.1 mmol/L Na3VO4 (pH 7.4)] containing protease and phosphatase inhibitors (Roche Molecular Biochemicals, Indianapolis, IN) and analyzed by Western blot.


Mouse total Chk1, mouse total Chk2, rabbit cdc2 Y15P, rabbit cdc25c S216P, rabbit acetylated histones H3 and H4 (acetyl-H3 or acetyl-H4), rabbit total cdc2, rabbit total cdc25c, rabbit total cdc25a, rabbit total histone H3, rabbit cPARP, rabbit total AKT, rabbit H3 S10P, and rabbit total c-RAF antibodies were obtained from Cell Signaling Technology (Watertown, MA). Rabbit cyclin B1 antibody was obtained from AbCam (Cambridge, MA).

Western blot analysis

Both adherent and detached cells in tissue culture wells were collected in 15-mL conical tubes and centrifuged at 4°C for 5 minutes at 1000 rpm in an Eppendorf 5810R centrifuge. The supernatant was removed, and the cell pellet was rinsed with ice-cold TBS, after which RIPA lysis buffer was added. Samples were sonicated, vortexed on ice every 10 minutes for 30 minutes, and then transferred to 1.5-mL microcentrifuge tubes and centrifuged for 10 minutes at 13,000 rpm at 4°C in an Eppendorf 5417R microcentrifuge. We used the Pierce BCA assay kit to determine protein concentrations, following manufacturer's protocol (Thermo Fisher Scientific, Rockford, IL). Samples were heated to 95°C for 10 minutes prior to resolving on an SDS-PAGE using a 4% stacking/10% resolving gel and transferred to a polyvinylidene difluoride membrane using a semi-dry transfer device (BioRad Industries, Hercules, CA). The membrane was blocked for 1 hour at room temperature in Pierce Superblock (Thermo Fisher Scientific) and probed for various antibodies. Enhanced chemiluminescent detection was performed following manufacturer's protocols (Thermo Fisher Scientific). Quantitation of Western Blots was done using AlphaEase FC software (Cell Biosciences, Inc., Santa Clara, CA).

Determination of Annexin V Positive Cells by Flow Cytometry

A549 or PC9 NSCLC cells were seeded in 6-well plates at a density of (4×105) cells/well. Cells were treated the next day with 40 nM LBH589 and collected 24 hours later for analysis using the BD Annexin V-FITC/7-AAD Flow Cytometry kit (BD Bioscience, San Jose, CA, 559763) per manufacturer's protocol. Cells were trypsinized with 0.05% w/v trypsin (Invitrogen Corp, Carlsbad, CA, 25300) and centrifuged for 5 minutes at 1000 rpm at 4°C in an Eppendorf Model 5417R centrifuge. Cell pellets were then rinsed 1x with ice-cold 1x DPBS and centrifuged again for 5 minutes at 1000 rpm and 4°C. Cells were then re-suspended in 1x Annexin V Binding Buffer at a concentration of 1×106 cells/mL. An aliquot of 100 uL of this cell suspension was then stained by addition of 5 uL Annexin V-FITC solution and 10 uL 7-AAD solution and allowed to incubate for 15 minutes on ice in the dark. Positive control cells were prepared by heating an aliquot of cells to 98°C for 2 minutes. Separate aliquots of cells were prepared for Annexin V-FITC only controls and 7-AAD only controls. Aliquots of healthy, untreated cells were added to these controls post-heating to obtain a representative profile of healthy and unhealthy populations for gating. After the 15 minute incubation was completed, 400 uL of Annexin V Binding Buffer was added to each sample and mixed. Samples were analyzed within 30 minutes on a BD FACScan instrument with FLOWJO software to determine the percentage of Annexin V positive cells.

Transfection experiments

The pGFP-CHK1 plasmid was purchased from Dana Farber/Harvard Cancer Center DNA Resource Core. The pFLAG-CHK1 plasmid was provided by Dr. Helen M. Piwnica-Worms, Washington University, St. Louis, MO. All transfections were carried out in 6-well culture plates maintained at 37°C in a 5% CO2 incubator. Twenty-four hours before transfection, 5×105 A549 cells were seeded in each well. Cells were transfected with 1 µg plasmid DNA using Lipofectamine with Plus Reagent (Invitrogen, Carlsbad, CA) according to the manufacturer's protocols. Twenty-four hours post-transfection, cells were treated with HDACi for 24 hours prior to collection for Western blot analysis. Untransfected control cells were collected 48 hours post-transfection.

Cell growth and viability assays

A549 cells were treated with LBH589 and UCN-01 alone or in combination at a constant ratio for 72 hours. Cell viability was measured by the CT-Blue assay (Promega). The combined effects of LBH589 and UCN-O1 were quantified using a combination index (CI) method developed by Chou and Talalay [40]. This method involves plotting dose-effect curves for each agent and their combination, using a median-effect equation: fa/fu  = (D/Dm)m, where D is dose of drug, Dm is dose required for a 50% effect (equivalent to IC50), fa and fu are affected and unaffected fractions, respectively (fa  = 1 - fu), and m is the exponent signifying the sigmoidicity of the dose-effect curve. The computer software Xlfit version 4.3.1 (ID Business Solutions) was used to calculate the values of Dm and m. The CI used for the analysis of the drug combinations was determined by the isobologram equation for mutually nonexclusive drugs that have different modes of action: CI  = (D)1/(Dx)1+ (D)2/(Dx)2+ [(D)1(D)2]/[(Dx)1(Dx)2], where (D)1 and (D)2 are relative concentrations of drugs 1 and 2 and x is the percentage of inhibition. CI <1, CI  = 1, and CI >1 indicate synergism, additive effects, and antagonism, respectively.

Cell cycle analysis

After they were rinsed with PBS, A549 or PC9 cells were collected at various time points after HDACi treatment and fixed in 70% ethanol while vortexing. Fixed cells were stored overnight at −20°C. The following day, cells were washed twice in PBS and treated with RNase A at 37°C for 30 minutes. Propidium iodide was then added to the cells, and cells were allowed to incubate in the dark for 1 hour at room temperature. Cells were then analyzed by flow cytometry using a fluorescence-activated cell sorter (BD Bioscience, San Jose, CA), Cell-Quest and FlowJo analysis software.


A549 cells were grown to 50% confluence on sterile glass coverslips in 6-well plates. Twenty-four hours after they were seeded, cells were treated with 40 nM LBH589 for 24 hours. Cells were then fixed in ice-cold 4% (w/v) p-formaldehyde in PBS for 15 minutes and permeabilized with 0.15% Triton X-100 for 30 minutes. Cells were then blocked with 5% bovine serum albumin (Thermo Fisher Scientific) in PBS for 1 hour at room temperature and probed with rabbit cPARP antibody (Cell Signaling Technology) at a dilution of 1[ratio]50 overnight at 4°C. After they were washed three times in PBS, cells were incubated for 1 hour at room temperature with AlexaFluor 596 conjugated goat anti-rabbit secondary antibody (Molecular Probes, Eugene, OR) at a dilution of 1[ratio]200. Coverslips were then mounted on slides using Vector Mount containing DAPI nuclear stain (Molecular Probes). We viewed slides with a Zeiss-inverted microscope, analyzed with Axiovert software.

Quantitative reverse transcription-PCR

RNA was isolated using the RNeasy kit (Qiagen 74104). First strand cDNA was synthesized from 1 µg of RNA using Bio-Rad iScript cDNA synthesis kit (Bio-Rad, 170-8891) in 20 ul reaction volume. Real-time PCR was performed using Bio-Rad iQ SYBR Green Supermix (Bio-Rad, 170-8882) on a MyiQ Single Color Real-time PCR detection system. 1 ul of cDNA was used in each 25 ul PCR reaction. The following primers were used: CHK1 forward, 5′-TGC TCA GAG ATT CTT CCA TC-3′; CHK1 reverse, 5′-AAC GCT CAC GAT TAT TAT ACC-3′; GAPDH forward, 5′-GAG TCA ACG GAT TTG GTC GT-3′; GAPDH reverse, 5′-TTGATTTTGGAGGGATCTCG-3′. GAPDH was served as internal control.


Competing Interests: The authors have declared that no competing interests exist.

Funding: The work was funded in part by the Moffitt Cancer Center SPORE grant in lung cancer. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Lane AA, Chabner BA. Histone deacetylase Inhibitors in cancer therapy. J Clin Oncol. 2009;10:5459–68. [PubMed]
2. Khan N, Jeffers M, Kumar S, Hackett C, Boldog F, et al. Determination of the class and isoform selectivity of small-molecule histone deacetylase inhibitors. Biochem J. 2008;409:581–589. [PubMed]
3. Yu X, Guo ZS, Marcu MG, Neckers L, Nguyen DM, et al. Modulation of p53, ErbB1, ErbB2, and Raf-1 expression in lung cancer cells by depsipeptide FR901228. J Natl Cancer Inst. 2002;94:504–513. [PubMed]
4. Deroanne CF, Bonjean K, Servotte S, Devy L, Colige A, et al. Histone deacetylases inhibitors as anti-angiogenic agents altering vascular endothelial growth factor signaling. Oncogene. 2002;21:427–436. [PubMed]
5. Coleman TR, Dunphy WG. Cdc2 regulatory factors. Curr Opin Cell Biol. 1994;6:877–882. [PubMed]
6. Morgan DO. Cyclin-dependent kinases: engines, clocks, and microprocessors. Annu Rev Cell Dev Biol. 1997;13:261–291. [PubMed]
7. Ohi R, Gould KL. Regulating the onset of mitosis. Curr Opin Cell Biol. 1999;11:267–273. [PubMed]
8. O'Connell MJ, Walworth NC, Carr AM. The G2-phase DNA-damage checkpoint. Trends Cell Biol. 2000;10:296–303. [PubMed]
9. Elledge SJ. Cell cycle checkpoints: preventing an identity crisis. Science. 1996;274:1664–1672. [PubMed]
10. Bartek J, Lukas J. Chk1 and Chk2 kinases in checkpoint control and cancer. Cancer Cell. 2003;3:421–429. [PubMed]
11. Zhou BB, Bartek J. Targeting the checkpoint kinases: chemosensitization versus chemoprotection. Nat Rev Cancer. 2004;4:216–225. [PubMed]
12. Zhao H, Piwnica-Worms H. ATR-mediated checkpoint pathways regulate phosphorylation and activation of human Chk1. Mol Cell Biol. 2001;21:4129–4139. [PMC free article] [PubMed]
13. Sorensen CS, Syljuasen RG, Falck J, Schroeder T, Ronnstrand L, et al. Chk1 regulates the S phase checkpoint by coupling the physiological turnover and ionizing radiation-induced accelerated proteolysis of Cdc25A. Cancer Cell. 2003;3:247–258. [PubMed]
14. Peng CY, Graves PR, Thoma RS, Wu Z, Shaw AS, et al. Mitotic and G2 checkpoint control: regulation of 14-3-3 protein binding by phosphorylation of Cdc25C on serine-216. Science. 1997;277:1501–1505. [PubMed]
15. Peddibhotla S, Lam MH, Gonzalez-Rimbau M, Rosen JM. The DNA-damage effector checkpoint kinase 1 is essential for chromosome segregation and cytokinesis. Proc Natl Acad Sci U S A. 2009;106:5159–5164. [PubMed]
16. Sausville EA, Arbuck SG, Messmann R, Headlee D, Bauer KS, et al. Phase I trial of 72-hour continuous infusion UCN-01 in patients with refractory neoplasms. J Clin Oncol. 2001;19:2319–2333. [PubMed]
17. Dees EC, Baker SD, O'Reilly S, Rudek MA, Davidson SB, Aylesworth C, et al. A phase I and pharmacokinetic study of short infusions of UCN-01 in patients with refractory solid tumors. Clin Cancer Res. 2005;11:664–671. [PubMed]
18. Ashwell S, Janetka JW, Zabludoff S. Keeping checkpoint kinases in line: new selective inhibitors in clinical trials. Expert Opin Investig Drugs. 2008;17:1331–1340. [PubMed]
19. Edwards A, Li J, Atadja P, Bhalla K, Haura EB. Effect of the histone deacetylase inhibitor LBH589 against epidermal growth factor receptor-dependent human lung cancer cells. Mol Cancer Ther; 2007;6:2515–2524. [PubMed]
20. Mitsudomi T, Steinberg SM, Nau MM, Carbone D, D'Amico D, et al. p53 gene mutations in non-small-cell lung cancer cell lines and their correlation with the presence of ras mutations and clinical features. Oncogene. 1992;7:171–180. [PubMed]
21. Kashii T, Mizushima Y, Monno S, Nakagawa K, Kobayashi M. Gene analysis of K-, H-ras, p53, and retinoblastoma susceptibility genes in human lung cancer cell lines by the polymerase chain reaction/single-strand conformation polymorphism method. J Cancer Res Clin Oncol. 1994;120:143–148. [PubMed]
22. Jia LQ, Osada M, Ishioka C, Gamo M, Ikawa S, et al. Screening the p53 status of human cell lines using a yeast functional assay. Mol Carcinog. 1997;19:243–253. [PubMed]
23. Noh EJ, Lim DS, Jeong G, Lee JS. An HDAC inhibitor, trichostatin A, induces a delay at G2/M transition, slippage of spindle checkpoint, and cell death in a transcription-dependent manner. Biochem Biophys Res Commun. 2009;378:326–331. [PubMed]
24. Leung-Pineda V, Huh J, Piwnica-Worms H. DDB1 targets Chk1 to the Cul4 E3 ligase complex in normal cycling cells and in cells experiencing replication stress. Cancer Res. 2009;69:2630–2637. [PMC free article] [PubMed]
25. Feng JM, Zhu H, Zhang XW, Ding J, Miao ZH. Proteasome-dependent degradation of Chk1 kinase induced by the topoisomerase II inhibitor R16 contributes to its anticancer activity. Cancer Biol Ther. 2008;7:1726–1731. [PubMed]
26. Matsuura K, Wakasugi M, Yamashita K, Matsunaga T. Cleavage-mediated activation of Chk1 during apoptosis. J Biol Chem. 2008;283:25485–25491. [PubMed]
27. Gray NS, Wodicka L, Thunnissen AM, Norman TC, Kwon S, et al. Exploiting chemical libraries, structure, and genomics in the search for kinase inhibitors. Science. 1998;281:533–538. [PubMed]
28. Zabludoff SD, Deng C, Grondine MR, Sheehy AM, Ashwell S, et al. AZD7762, a novel checkpoint kinase inhibitor, drives checkpoint abrogation and potentiates DNA-targeted therapies. Mol Cancer Ther. 2008;7:2955–2966. [PubMed]
29. Qiu L, Kelso MJ, Hansen C, West ML, Fairlie DP, et al. Anti-tumour activity in vitro and in vivo of selective differentiating agents containing hydroxamate. Br J Cancer. 1999;80:1252–1258. [PMC free article] [PubMed]
30. Taddei A, Maison C, Roche D, Almouzni G. Reversible disruption of pericentric heterochromatin and centromere function by inhibiting deacetylases. Nat Cell Biol. 2001;3:114–120. [PubMed]
31. Robbins AR, Jablonski SA, Yen TJ, Yoda K, Robey R, et al. Inhibitors of histone deacetylases alter kinetochore assembly by disrupting pericentromeric heterochromatin. Cell Cycle. 2005;4:717–726. [PubMed]
32. Qiu L, Burgess A, Fairlie DP, Leonard H, Parsons PG, et al. Histone deacetylase inhibitors trigger a G2 checkpoint in normal cells that is defective in tumor cells. Mol Biol Cell. 2000;11:2069–2083. [PMC free article] [PubMed]
33. Warrener R, Beamish H, Burgess A, Waterhouse NJ, Giles N, et al. Tumor cell-selective cytotoxicity by targeting cell cycle checkpoints. FASEB J. 2003;17:1550–1552. [PubMed]
34. Stevens FE, Beamish H, Warrener R, Gabrielli B. Histone deacetylase inhibitors induce mitotic slippage. Oncogene. 2008;27:1345–1354. [PubMed]
35. Kaneko YS, Watanabe N, Morisaki H, Akita H, Fujimoto A, et al. Cell-cycle-dependent and ATM-independent expression of human Chk1 kinase. Oncogene. 1999;18:3673–3681. [PubMed]
36. Kovacs JJ, Murphy PJ, Gaillard S, Zhao X, Wu JT, et al. HDAC6 regulates Hsp90 acetylation and chaperone-dependent activation of glucocorticoid receptor. Mol Cell. 2005;18:601–607. [PubMed]
37. Bali P, Pranpat M, Bradner J, Balasis M, Fiskus W, et al. Inhibition of histone deacetylase 6 acetylates and disrupts the chaperone function of heat shock protein 90: a novel basis for antileukemia activity of histone deacetylase inhibitors. J Biol Chem. 2005;280:26729–26734. [PubMed]
38. Garber ME, Troyanskaya OG, Schluens K, Petersen S, Thaesler Z, et al. Diversity of gene expression in adenocarcinoma of the lung. Proc Natl Acad Sci U S A. 2001;98:13784–13789. [PubMed]
39. Rubio-Viqueira B, Mezzadra H, Nielsen ME, Jimeno A, Zhang X, et al. Optimizing the development of targeted agents in pancreatic cancer: tumor fine-needle aspiration biopsy as a platform for novel prospective ex vivo drug sensitivity assays. Mol Cancer Ther. 2007;6:515–523. [PubMed]
40. Chou TC, Talalay P. Quantitative analysis of dose-effect relationships: the combined effects of multiple drugs or enzyme inhibitors. Adv Enzyme Regul. 1984;22:27–55. [PubMed]

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