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Histone deacetylase inhibitor‐mediated cell death is distinct from its global effect on chromatin
Associated Data
Abstract
Romidepsin and vorinostat are histone deacetylase inhibitors (HDACis) that have activity in T‐cell lymphomas, but have not gained traction in solid tumors. To gain deeper insight into mechanisms of HDACi efficacy, we systematically surveyed 19 cell lines with different molecular phenotypes, comparing romidepsin and vorinostat at equipotent doses. Acetylation at H3K9 and H4K8 along with 22 other histone lysine acetylation and methylation modifications were measured by reverse phase proteomics array (RPPA), and compared with growth inhibition (IC50), and cell cycle arrest. These assays typically used to assess HDACi effect showed that acetylation and methylation of specific lysine residues in response to HDACis were consistent across cell lines, and not related to drug sensitivity. Using a treatment duration more reflective of the clinical exposure, cell death detected by annexin staining following a 6 h drug exposure identified a subset of cell lines, including the T‐cell lymphoma line, that was markedly more sensitive to HDAC inhibition. Kinetic parameters (Km values) were determined for lysine acetylation and for cell cycle data and were themselves correlated following HDACi exposure, but neither parameter correlated with cell death. The impact on cell survival signaling varied with the molecular phenotype. This study suggests that cellular response to HDACis can be viewed as two distinct effects: a chromatin effect and a cell death effect. All cells undergo acetylation, which is necessary but not sufficient for cell death. Cells not primed for apoptosis will not respond with cell death to the impact of altered histone acetylation. The divergent apoptotic responses observed reflect the variable clinical outcome of HDACi treatment. These observations should change our approach to the development of therapeutic strategies that exploit the dual activities of HDACis.
Highlights
- HDIs cause two distinct effects: a chromatin effect and a cell death effect.
- Acetylation after HDI is monotonous, found at multiple lysine residues.
- The impact on chromatin triggers apoptosis in only selected cell types.
- Short drug exposure models the divergent clinical responses.
- Further clinical development should take into account this differential effect.
1. Introduction
Histone deacetylase inhibitors (HDACis) constitute a class of targeted anticancer agents that inhibit histone deacetylases (HDACs) and effect chromatin modulation through altered binding of transcriptional co‐activator complexes. Studies have shown that HDACis alter approximately 7–10% of genes including those that control growth, differentiation, and apoptosis; genes are both up‐ and down‐regulated (Peart et al., 2005; Xu et al., 2007). In addition, HDACis have been shown to impair angiogenesis and metastasis; inhibit DNA repair while increasing the generation of reactive oxygen species (ROS); and modulate the mitogen‐activated protein kinase (MAPK) pathway (Khan and La Thangue, 2012; Rosato and Grant, 2003). While unrestrained histone acetylation results from HDAC inhibition, a myriad of cellular effects have been described. HDACis also promote acetylation of cytoplasmic proteins, altering function in some and in others, including several oncogenic proteins, inciting their degradation (Bali et al., 2005; Chen et al., 2009; Gu and Roeder, 1997; Gupta et al., 2012; Lane and Chabner, 2009; Zhang et al., 2003). Sorting out which of these effects is most important to accomplish cell death has been a perplexing problem for those working in the field.
Gene induction by HDACis has been tied to both cell cycle arrest and apoptosis. G1 arrest occurs via activation of the cyclin‐dependent kinase inhibitor p21 in a p53‐independent manner (Blagosklonny et al., 2002; Sandor et al., 2000) and downregulation of cyclins D and A. HDACis repress two genes involved in DNA synthesis, CTP synthase and thymidylate synthetase (Glaser et al., 2003), and as a result may block S‐phase progression. Finally, HDACis can mediate G2/M phase arrest by activating a G2‐phase checkpoint when the centromere is aberrantly acetylated (Robbins et al., 2005). Similarly, HDACis have been shown to induce apoptosis via the extrinsic and the intrinsic pathways. Some studies indicate a death receptor pathway, such as the induction of Fas or Fas ligand, TRAIL, DR‐4, DR‐5 (Kaminskyy et al., 2011; Nebbioso et al., 2005; Yeh et al., 2009); while other studies suggest that the mitochondrial apoptotic pathway is involved through decreasing expression of antiapoptotic proteins BCL‐2, BCL‐XL, MCL‐1 (Jiang et al., 2007; Newbold et al., 2008), and upregulating expression of the BH3‐domain proapoptotic proteins Bim, Bad, Bid, Bik, Puma, Noxa (Baumann et al., 2012; Xargay‐Torrent et al., 2011).
It has been difficult to reconcile all the promising in vitro data with the clinical results. To date, the clinical data for HDACis have proven efficacy in T‐cell lymphomas, but not in various solid tumors in which they have been tested (Venugopal and Evans, 2011). The U.S. Food and Drug Administration has approved two HDACis, romidepsin and vorinostat, for the treatment of cutaneous T‐cell lymphoma and romidepsin for the treatment of peripheral T‐cell lymphoma (Bates et al., 2010; Olsen et al., 2007; Piekarz and Bates, 2009; Piekarz et al., 2011). In this study, we sought to identify differential activity between cell lines that might yield insights into the clinical observations, and also to determine potential differences between the HDACis romidepsin and vorinostat after correction for the well‐known difference in potency. We examined global histone changes, cell cycle arrest, and apoptosis after HDACi treatment in a series of nineteen cell lines with differing genetic lesions. We conclude that epigenetic effects on histone acetylation are homogenous between drugs and across cell lines, but that the ability to undergo rapid cell death in response to acetylation is cell context specific.
2. Materials and methods
2.1. Cell lines and drugs
Cell lines were obtained from American Type Culture Collection and the NCI Anticancer Drug Screen; the p21‐deficient HCT116 subline (HCT116 p21−/−) was a gift from Dr. Bert Vogelstein (Johns Hopkins University). Cell line validation was performed and DNA fingerprinting confirmed their identities. Cultures were replaced in less than 3 months. Cells were cultured in RPMI 1640 or IMEM (GIBCO, Grand Island, NY) supplemented with 10% fetal bovine serum (GIBCO, Grand Island, NY), 2 mM glutamine (BioFluids, Rockville, MD), and 100‐units/L penicillin‐streptomycin (BioFluids). MCF‐10A was grown in DMEM‐F12 medium (Mediatech, Inc., Herndon, VA) supplemented with 5% horse serum, 10 μg/ml insulin, 20 ng/ml epidermal growth factor, 0.5 μM/ml hydrocortisone (Sigma, St. Lois, MO), and 100‐units/L penicillin‐streptomycin (BioFluids). HDACis romidepsin and vorinostat were obtained from the Anticancer Drug Screen (Cancer Therapy Evaluation Program, NCI, NIH, Bethesda, MD) and Cayman Chemical (Ann Arbor, MI), dissolved in DMSO at 100 μg/ml and 100 mM, respectively, and stored in aliquots at −20 °C. Caspase Inhibitor Q‐VD‐OPh was obtained from R&D Systems (R&D Systems, Minneapolis, MN) and dissolved in DMSO at 10 mM.
2.2. Cell sensitivity assay
Cells were treated with the indicated concentrations of HDACis for 96 h. For suspension cells analysis of growth inhibition was performed by MTS assay using the Cell Titer 96 Aqueous One Solution (Promega, Madison, WI, USA), and for adherent cells growth inhibition was performed by MTT assay or using sulforhodamine B stain (Sigma, St. Lois, MO) according to the manufacturer's protocols.
2.3. Cell cycle analysis by flow cytometry
Cell cycle distribution was determined by analyzing DNA content after propidium iodide staining. Cells were harvested, fixed in 70% ice‐cold ethanol, washed with PBS, and stained with 50 μg/ml propidium iodide containing 200U/ml RNase A. DNA content was analyzed using a FACScan flow cytometer (Becton Dickinson, San Jose, CA). Data were collected with Cell Quest Pro software from no fewer than 10,000 cells and analyzed using FlowJo software (Tree Star, Inc, Ashland, OR). Once cell cycle parameters were determined, the delta or difference between treated and untreated control was calculated at each dose and for each parameter, and used in further analyses.
2.4. Annexin V assay
Apoptosis was measured using the annexin V‐fluorescein isothiocyanate (annexin V‐FITC) Apoptosis Detection Kit (BD Biosciences, San Diego, CA) according to the manufacturer's instructions. Cells were treated with 25 ng/ml (45 nM) romidepsin or 25 μM vorinostat for 6 h, washed, and incubated an additional 42 h in drug‐free medium. Following treatment, annexin positive cells were quantitated using FlowJo Software. The percentage of annexin positive cells was derived, and the delta between treated and untreated control determined.
2.5. Reverse phase protein array (RPPA)
Cells were lysed in 10 mM HEPES, pH 7.4, 1% LDS, containing protease (Sigma, St. Louis, MO) and phosphatase inhibitors (Roche Diagnostic, Indianapolis, IN), and then sonicated. Protein concentrations were determined using BCA protein assay (Pierce, Rockford, IL); the samples were adjusted to equal protein concentrations, and then printed onto nitrocellulose‐coated glass slides (Grace Bio‐Labs, Bed, USA) using a solid‐pin arrayer (Aushon Biosystems, Billirica, MA). Triplicate four‐point serial deposition curves were printed for each lysate. Primary antibody staining was done overnight at 4 °C, and probed using a secondary‐antibody amplification‐and‐detection system FITC tyramide (Perkin–Elmer, USA) at room temperature. For the origin and description of all antibodies used in this study see Supplementary Table S1.
Slides were imaged with the FLA‐8000 scanner (Fujifilm), and relative signal intensities were calculated using MicroVigene software (VigeneTech, Carlisle, USA). The average staining of the triplicate prints was used for statistical analysis. After adjusting for the negative control signal, each histone modification value was normalized to the total histone H3 level.
2.6. Immunoblot analysis
Cell pellets were suspended in RIPA buffer with protease inhibitor cocktail (Sigma, St. Louis, MO), phosphatase inhibitors (Roche Diagnostic, Indianapolis, IN), and trichostatin A inhibitor, and then sonicated for 40 s. Protein concentration was measured using the Bio‐Rad Protein Assay (Bio‐Rad Inc., USA). Denaturated protein (20 μg) was loaded onto precast 4–12% Bis‐Tris NuPAGE gels, subjected to electrophoresis, and transferred onto 0.2 μM pore size nitrocellulose membranes (Invitrogen, Carlsbad, CA). Membranes were stained with 0.1% Ponceau S (Sigma, St. Louis, MO) and checked for comparable loading. After blocking with Odyssey blocking buffer (LI‐COR Bioscience, Lincoln, NE) for 1h at room temperature, membranes were incubated with following primary antibodies: H3K9ac (Upstate Biotechnology, Lake Placid, NY), H3K18ac, H3K36me2, H3K79me2, H3pan, PARP, cleaved‐PARP, p‐Rb, p‐MEK 1/2, MEK 1/2, p‐ERK 1/2, ERK 1/2, p‐AKT, AKT, Bim, Cyclin D1 (Cell Signaling Technology, Danvers, MA), H3K4me3, H3K9me3 (Abcam, Cambridge, MA), H4K8ac, c‐Myc (Santa Cruz Biotechnology, CA), p21 (Calbiochem‐Millipore, Billerica, MA), Ac‐α‐tubulin, α‐tubulin (Sigma, St. Lois, MO), GAPDH (American Research Products, MA) overnight at 4 °C. Membranes were probed with the IRDye 800CW goat anti‐mouse or IRDye 680 goat anti‐rabbit secondary antibodies (LI‐COR, Lincoln, NE), visualized and quantified using Odyssey System (LI‐COR).
2.7. Data analysis
Data visualization, including dynamic principle component analysis (PCA), heat maps and unsupervised hierarchical clustering was performed in Qlucore Omics Explorer v.2.2 (Qlucore AB, Lund, Sweden). Correlations between protein marker expression and all other parameters (including cell cycle, growth, apoptosis, drug concentration, time, and phosphorylation) were analyzed using both the non‐parametric Spearman's rank correlation coefficient test for ordinal data, and linear regression for continuous data. (GraphPad Prism 5.0). P‐values less than 0.05 were considered significant. Graphical presentation and regression analyses were made using Sigmaplot 11 software (Systat Software, Inc. 1735 Technology Drive, Suite 430 San Jose, CA 95110 USA). For both cell cycle and proteomic histone modification data, dose response curves were used to determine the Km values. The data were fitted to a hyperbolic function, descending or ascending as appropriate. In some cases of the histone modification data, the fitting procedure failed to give a convergent solution since the data were too few or too scattered. The Km values from the convergent solutions for the individual histone modifications were then averaged to generate a final mean “Km marks” value that was used in correlation analyses. In a few cases, the cell cycle changes were insufficiently large to allow the extraction of the kinetic parameters.
3. Results
To study the effect of the HDACis romidepsin and vorinostat we selected immortalized breast cell line MCF‐10A, and 18 cancer cell lines derived from breast (MCF‐7, SK‐BR‐3, MDA‐MB‐231), prostate (PC3), lung (A549, H460, EKVX, H146, H526), and colon cancer (HCT116, HCT116 p21−/−, S1, SW620), melanoma (LOX‐IMVI, UACC‐62, MDA‐MB‐435), glioma (SF‐295), and T‐cell lymphoma (HUT‐78) with different molecular phenotypes. Known mutations are shown in Table 1.
Table 1
3.1. Analysis of growth inhibition by 96‐h assay shows a similar profile across cell lines
One of the most widely used tests for drug efficacy is the 96‐h growth inhibition/cytotoxicity assay. This assay is widely used to assess HDACi effects and we thus utilized it to examine differences between romidepsin and vorinostat and among the cell lines. The concentration at which growth is inhibited by 50% (IC50) was determined after 96 h incubation in equipotent dose ranges for both drugs. Table 1 shows IC50 values for the various cell lines, with the median IC50 for romidepsin (1.5 nM) and for vorinostat (2 μM) indicating an approximate 1000‐fold difference in potency. With the P‐glycoprotein‐over‐expressing S1 cell line excluded (Pgp is a known mechanism of resistance for romidepsin) (Robey et al., 2006; Xiao et al., 2005), the scatter plot in Figure 1 shows a similar profile for the cell lines (R = 0.75, P = 0.005), demonstrating indiscriminate anticancer activity for both drugs in the 96 h continuous exposure format, without differentiating between the two HDACis, after correction for the well‐known difference in potency between the two drugs.
3.2. Reverse phase proteomics array shows similar patterns for histone marks across cell lines
We next looked for differential effects at the histone level examining histone marks using a custom‐designed, reverse phase protein array (RPPA), a high‐throughput dot‐blot protein microarray containing 4992 spots per slide. The lysines on histone tails undergo post‐translational modification including acetylation and methylation. Acetylation, resulting from the unrestrained histone acetyltransferase activity that follows inhibition of the histone deacetylases, is classically an activating modification. Methylation occurs with one, two or three groups added to the lysine, and although typically repressive, methylation at H3K4 is known to be activating. We screened the protein array for 24 histone acetylation and methylation modifications in separate experiments for romidepsin and vorinostat at six equipotent concentrations (3‐fold serial dilutions of 0.1–30 ng/ml (0.2–54 nM) romidepsin, 0.1–30 μM vorinostat) at four different time points (8, 24, 48, 72h). Figure 2A displays graphically the induction of H3K9 acetylation in every cell line, while Figure 2B presents a heat map showing the common global effect on acetylation following romidepsin, despite minor differences in acetylation intensity among the cell lines. Results here are not clustered but arranged by cell line and concentration.
In Figure 2C, dose responses for several acetylated lysines are plotted, from which Km values (the concentrations required to achieve half‐maximal acetylation) were derived. Due to background staining in the RPPA, there was variability in the number of acetylation sites for which an accurate Km could be attained for each cell line. The Km values from the convergent solutions for the individual histone modifications were then averaged to generate a final value with its SD that was used in correlation analyses. The n and mean acetylation Km for each cell line is provided in Supplementary Table S2. Notably, Km values for the histone modifications were not at all correlated with the IC50 obtained from the growth inhibition assays (R = 0.0437, P = 0.863, n = 18 for romidepsin; and R = 0.095, P = 0.747, n = 14 for vorinostat).
Next, unsupervised clustering analyses were performed. Since the romidepsin and vorinostat RPPA experiments were performed separately, clustering analyses were performed separately. Unsupervised two‐way clustering of histone acetylation modifications revealed similar patterns across cell lines after 24 h of either romidepsin or vorinostat treatment (Supplementary Figure S2A and S2B). When methylation modifications were included and the data organized by concentration and subjected to one‐way clustering, the repressive modifications, as one might expect, generally separated from the activating modifications (Supplementary Figure S2C and S2D). Upon examining the time course of HDACi treatment on histone modifications (also referred to as marks) (Supplementary Figure S3), activating marks were found to have the highest expression after 8 and 24 h following HDACi treatment, decreasing with continued exposure to romidepsin. Minimal or no change was observed in repressive marks at 8 and 24 h. Unlike RNA induction, which increases with longer exposure to HDACis (Kitazono et al., 2001), the global acetylation increase appears to be self‐limited.
To validate the proteomic data and to look for further insight into the mechanism of HDACi effect, we performed immunoblot analysis of selected histone modifications in three cell lines with different molecular phenotypes treated for 24 h with romidepsin and vorinostat as shown in Figure 3A. As in the RPPA, the acetyl marks and the methyl activating mark H3K4me3 were induced with both HDACis, while repressive marks such as H3K9me3 did not change significantly (Figure 3B). The correlation between RPPA and Western blot analysis of histone proteins is consistent for both drugs with R = 0.78 for romidepsin and with R = 0.74 for vorinostat, P < 0.001, as shown in Figure 3C.
3.3. Analysis of cell cycle distribution reveals cell type‐specific responses to HDACI treatment
We performed cell cycle analysis on the nineteen cell lines after a 24 h treatment using 3‐fold serial dilutions of romidepsin (0.1–30 ng/ml, 0.2–54 nM) and vorinostat (0.1–30 μM), again adjusting for the difference in potency between romidepsin and vorinostat. As shown in Figure 4 and Supplementary Figures S4A–C, the effects of HDACI treatment were different among the cell lines, ranging from only minor changes in G1/S/G2‐M distribution as in MDA‐MB‐435 to mostly apoptosis in H146. As shown in Figure 4C, we found three basic patterns of cell cycle response to HDACis: (1) predominant G1 arrest (MCF‐10A, UACC‐62), (2) predominant G2 arrest (PC3, LOX‐IMVI, MDA‐MB‐231, MDA‐MB‐435, SW620, S1), including a subset with an increasing Sub‐G1 population indicative of apoptosis (MCF‐7, A549, EKVX, HCT116 p21−/−), and (3) cells undergoing apoptosis either without appearing to have entered cell cycle arrest or leaving cell cycle arrest very rapidly (H146, H526, HuT‐78, SK‐BR‐3, H460, HCT116). It is interesting to note that the cell cycle effect most often mentioned, G1 arrest, was least common among the 19 cell lines. Figure 4D shows that a cell cycle arrest pattern emerged when the general caspase inhibitor Q‐VD‐OPh was added to prevent cell death.
Notably, as in the RPPA, romidepsin and vorinostat again appear to have similar effects in the equipotent dose range used, a result supported by the high correlation coefficients for all cell cycle parameters (Supplementary Figure S4D). For example, the Pearson correlation coefficients between the two drugs, for all cell line parameters, exceeds 0.54 for G1 arrest in concentrations ≥ 3 ng/mL (5.4 nM) for romidepsin and ≥ 3 μM for vorinostat.
We also determined the Km – concentration of HDACi required to produce a half‐maximal cell cycle effect – in some cases measurable only for G2‐M arrest or Sub‐G1 increase. Examples of the plots for these Km determinations are shown in Figure 5A and Supplementary Figure 5. Often the decrease in G1 content that accompanied the G2‐M arrest could be fit to a curve and the Km calculated. Providing an internal validation of this quantitation, the Km's for the effect on G1 and G2‐M content were correlated for both romidepsin and vorinostat (R = 0.92, P = 0.0014, n = 8 for romidepsin; R = 0.95, P = 0.015, n = 5 for vorinostat). When the Km for drug effects on G2‐M and on Sub‐G1 were combined in plots against the Km's for G1 (Figure 5B), the overall correlation was R = 0.80, P = 0.0006, n = 13 for romidepsin. Similar observations were made for vorinostat (Figure 5C) when one outlier was excluded (R = 0.89, P = 0.002, n = 9). We also specifically evaluated the sub‐G1 region of DNA content in cells treated with the highest concentration of the drugs for 24 h, which shows a strong correlation in sub‐G1 between romidepsin and vorinostat (R = 0.96), but also discriminates between cell lines in that there are two major groupings of the cell lines in sub‐G1 effect (Figure 5D).
3.4. An assay that discriminates among the cell lines and between drugs
Given that romidepsin is administered over 4 h and vorinostat administered in a single daily oral dose, and that both drugs have half‐lives under 3 h, we concluded that long exposures do not mirror clinical HDACi dosing and utilized a short‐term assay for apoptosis detection, with cells exposed to HDACi for 6 h, and harvested after an additional 42 h incubation in drug‐free medium before staining for annexin positivity (Yu et al., 2007). A representative histogram quantitating annexin staining is shown in Figure 6A; in Figure 6B results for all cell lines treated at 25 ng/ml (45 nM) romidepsin and 25 μM vorinostat are graphed (excluding two cell lines that do not stain for annexin). This method provided for the first time a clear spectrum of HDACi sensitivity across the cell lines and identified some differential activity between the two HDACis. Although romidepsin's and vorinostat's efficacy by annexin assay were correlated (R = 0.69, P = 0.0022, n = 17), romidepsin was generally four times more potent in the induction of apoptosis, despite the use of concentrations assessed as equipotent as in the cell cycle and growth inhibition assays (Figure 6C). As might be expected from the uniform pattern of acetylation observed in Figure 2, romidepsin's and vorinostat's efficacy, as determined in this annexin assay, were not correlated with the absolute difference in H3K9ac, P = 0.94 and P = 0.56, respectively (Figure 6D and 6E), nor was annexin staining correlated with median Km values for the histone modifications (For romidepsin, P = 0.46, for vorinostat, P = 0.87). Including in the analysis only those 12 cell lines for which the annexin signal for romidepsin was less than 30% improved the correlation between the Km for histone modification and those for the cell cycle parameters, for example the Pearson correlation coefficient between the Km for the histone marks and the Km for the G2‐M arrest was R = 0.75, P = 0.019, n = 9 (a tighter correlation than the R = 0.629, P = 0.05 correlation noted in the entire group) (Supplementary Figure 6A and B), suggesting, as did the sub‐G1 fraction data, that a separate subset of cell lines exists in which rapid cell death occurs apart from the epigenetic effects.
3.5. Differential sensitivity of cancer cell lines to HDACi treatment depends on cell context
Because we have previously noted an interaction of HDACi and the MAPK pathway (Chakraborty et al., 2013; Ieranò et al., 2012), we examined the effect of HDACis on selected signaling proteins by immunoblot analysis using the same cells, doses, and exposures as in Figure 3. Two of the cell lines, MDA‐MB‐231 and A549, share common mutations, KRAS and CDKN2A, while the PC3 cell line has a PTEN mutation, and is relatively resistant to HDACi effect (Table 1). We compared the ratio of phosphorylated and total MEK1/2, ERK1/2, and AKT in MDA‐MB‐231, A549 and PC3 cells. Because phosphorylated AKT was relatively lower in MDA‐MB‐231 cells, results were calibrated to the MDA‐MB‐231 cells as shown in Figure 7A and B. Although basal levels of phosphorylated MEK1/2, ERK1/2 and AKT were different across these cell lines, both drugs inhibited phosphorylation in all of these cells. The analysis of other signaling proteins showed decreasing expression of p‐Rb, c‐Myc, cyclin D1, but induction of p21 and the apoptosis‐related molecules c‐PARP and Bim following treatment with HDACis (Figure 7C). Altogether, these results indicate that the cell death response to HDACi is more variable than the molecular effects of the HDACi. There is one point of divergence between romidepsin and vorinostat. It known that romidepsin has a relatively lower potency against HDAC6, which acetylates non‐histone proteins such as α‐tubulin, β‐catenin, Hsp90 and others (Crabb et al., 2008; Robey et al., 2011; Zhang et al., 2003). We confirmed this, showing a marked induction of α‐tubulin acetylation following treatment with vorinostat but not with romidepsin (Figure 7C).
4. Discussion
We report a systematic approach to understanding the mechanism of action of HDACis. We examined 18 human cancer cell lines with different molecular phenotypes, and one immortalized breast cell line, and analyzed the effect of romidepsin or vorinostat treatment at multiple concentrations and at different time points on growth inhibition and cell death, cell cycle distribution, histone modification, and protein expression. We selected two FDA‐approved HDACis, with different structures and HDAC affinity profiles and compared them across cell lines and with each other, generating insights into mechanism of HDACi activity. These studies show that HDACis induce similar global effects, including growth inhibition and acetylation – across cell lines and between drugs. Cell cycle perturbations were largely similar for romidepsin and vorinostat. Cell death assays detecting annexin expression demonstrated that a subset of cell lines is markedly more sensitive to death following a short exposure to the HDACi.
The most widely used assays for testing HDACi efficacy are a continuous (96‐h) cytotoxicity/growth inhibition assay, histone acetylation, and cell cycle effects. In the 96‐h cytotoxicity assays, we found the HDACis had nearly identical effects after taking into account the 1000‐fold lower IC50 values for romidepsin compared to vorinostat. When histone modifications were examined by reverse phase proteomic assay, it appeared that the global effect across cell lines was similar, with almost all cell lines responding with acetylation of the 13 different marks tested, suggesting that cell lines respond similarly to both HDACis with comparable degrees of histone acetylation. In vitro studies of inhibition of the most prevalent HDAC enzymes showed that romidepsin is by far the most potent agent in development and that its most prominent effect was inhibition of the Class I HDACs: HDAC 1, 2, 3, and 8 (Bradner et al., 2010). Vorinostat, in contrast, is able to inhibit Class II HDACs at concentrations near those required to inhibit the Class I enzymes. We were able to confirm the effect of vorinostat but not romidepsin on the Class II enzymes by showing α‐tubulin acetylation following the former, but not the latter. This suggests that the HDAC6 inhibition by vorinostat, as manifested by α‐tubulin acetylation in vitro, is not responsible for the clinical activity of romidepsin and vorinostat against T‐cell lymphomas. Indeed, HDAC6 inhibition may effectively be an off‐target effect for vorinostat in the therapy of in T‐cell lymphoma. However, in a different clinical context in which the HDAC6‐regulated Hsp90 chaperone function may be critical, such as HER2 amplification, HDAC6 inhibition by vorinostat could be of value.
Given the differences in HDAC specificity, we were surprised to find how similar were the effects of the two HDACis on cell cycle beginning at 3 ng/ml (5.4 nM) romidepsin and 3 μM vorinostat. However, not all cell lines responded similarly to treatment with the HDACis. In contrast to previously published observations, most of the cell lines fail to show a clear G1 cell cycle arrest (Sandor et al., 2000; Zhang et al., 2005). These variations are likely due to the different status of cell cycle checkpoints in different cell lines (Kastan and Bartek, 2004). Consistent with this, inhibition of caspase to prevent cell death revealed a G2 arrest in cells typically responding with apoptosis rather than cell cycle arrest.
The consistent effects on acetylation and cell cycle are similar to numerous reports in the literature showing HDACi activity in virtually any cell line tested (Crabb et al., 2008; Gravina et al., 2012; Imre et al., 2006; Marrocco‐Tallarigo et al., 2009; Mitić and McKay, 2005; Palmieri et al., 2009). Yet, this is in conflict with clinical observations in which HDACis as single agents are active to date exclusively in T‐cell lymphomas and other hematologic malignancies. We hypothesized that this discordance was due to the long exposure durations typically tested in cell culture, very different from the 2–3 h half‐life of the HDACis in patients (Piekarz et al., 2011, 2009). We showed that a short exposure to romidepsin followed by measurement of cell death by annexin positivity was a more discriminating assay in showing differences between cell lines than the continuous 96‐h assay. Some cell lines were completely insensitive in this assay, something not observed with the 96‐h growth inhibition assay. We also found romidepsin to be a more effective inducer of apoptosis in the annexin assay than vorinostat, despite equalization of potency based on cell cycle analysis. Interestingly, when we examined correlations between annexin and cell cycle arrest or histone modification, such correlations were only readily observed in those cell lines that did not show rapid cell death.
From these studies emerged a recognition of two distinct HDACi effects. The ubiquitous global effect on acetylation is in contrast to the differential annexin sensitivity observed after a 6 h exposure and also in contrast to the differential sensitivity seen in the clinic. The data suggest that the effects of HDACis, while in a spectrum, can be viewed as of two principle types. The first HDACi effect is a Type I effect that primarily affects chromatin and includes histone acetylation, altered gene expression, cell cycle arrest, and growth inhibition. This effect will lead to cell death if the exposure to the HDACi persists long enough. This is the effect studied when HDAC inhibitors were viewed primarily as differentiating agents (Richon et al., 1996). If we need to optimize expression of a target gene for a drug combination, it is likely that lower doses and longer exposure will be most effective (Amiri‐Kordestani et al., 2013; Kitazono et al., 2001).
At the other end of the spectrum, the second HDACi effect is the ability of HDACis to rapidly invoke cell death in some cell types – in our assay, induced by a brief 6‐h exposure to the HDACis. It may be useful to separate this Type II cell death effect from the Type I primarily chromatin effect, and make a goal of future drug development shifting from Type I to Type II, unless we specifically seek a particular gene induction effect. The HDAC enzyme target remains the same in both response types, and our data suggest that it is not the magnitude of acetylation but rather the susceptibility to apoptosis that determines the sensitivity. We propose that the 6‐h exposure, which more closely replicates the clinical exposure duration for most HDACis, induces a burst of global acetylation that we hypothesize is the initiating event that induces cell death in apoptosis‐susceptible cells, such as T‐cell lymphomas. This burst of acetylation may be recognized by cells as DNA damage – Conti et al. reported stalling of replication forks (and hypothesized a comparable effect on transcription) that resulted in DNA double strand breaks (Conti et al., 2010). If this is a key mechanism, then the DNA damage is triggering apoptosis in susceptible cells, based on cell context. This would explain not only the clinical results with rapid destruction of malignant T‐cells (Piekarz et al., 2001), but would also explain the widely observed susceptibility to combinations with agents that target various apoptosis proteins. Multiple studies have shown that HDACi sensitivity is impacted by the presence or absence of proteins modulating apoptosis – presence of Bak and Bax (Ieranò et al., 2012; Shao et al., 2010), a requirement for Bim (Chakraborty et al., 2013; Yang et al., 2009), and downregulation of proapoptotic BCL2A1 (Bolden 2013). Different molecular contexts will differentially impact the expression and function of the proteins involved in apoptosis.
Taken together, the data suggest that different cellular contexts determine the response to a ubiquitous and fairly consistent epigenetic effect. Supporting this argument are correlations observed in a pathway analysis of gene expression data correlating with panobinostat sensitivity in 500 cell lines of the Cancer Cell Line Encyclopedia. As shown in Supplementary Figure S7, 124 genes were correlated with panobinostat sensitivity. A search for upstream regulators for those 124 genes found multiple proteins associated with the MAPK pathway among the top hits. In turn, we compared HDACi sensitivity to mutations conferring MAPK pathway activation among the 19 cell lines and found those to be more sensitive to HDAC inhibitor than cell lines with mutations in the PI3K or p53 pathways (Supplementary Figure S7). If acetylation‐induced DNA damage is confirmed as the dominant mechanism of action of HDACis, clinical studies can then focus on approaches to modify sensitivity in specific molecular phenotypes. Together these studies point to a need to select specific molecular phenotypes for sensitivity to the HDACis and then to identify relevant combinations as a way forward in the development of these epigenetic therapies.
Conflicts of interest
The authors have no conflicts of interest to declare and no financial interests to report. Dr. Bates received research funding from Celgene Pharmaceuticals (CRADA #01683) through a Cooperative Research and Development Agreement with the National Cancer Institute.
Supporting information
The following is the supplementary data related to this article:
Supplementary data
Acknowledgments
This work was supported by the Intramural Research Program of the National Cancer Institute. The authors would like to thank Dan Sackett for advice over many phases of this project, and Julian Bahr for assisting in data acquisition.
Supplementary data 1.
Supplementary data related to this article can be found at http://dx.doi.org/10.1016/j.molonc.2014.05.001.
Notes
Luchenko Victoria L., Litman Thomas, Chakraborty Arup R., Heffner Aaron, Devor Christopher, Wilkerson Julia, Stein Wilfred, Robey Robert W., Bangiolo Lois, Levens David, Bates Susan E., (2014), Histone deacetylase inhibitor‐mediated cell death is distinct from its global effect on chromatin, Molecular Oncology, 8, doi: 10.1016/j.molonc.2014.05.001. [PMC free article] [PubMed] [Google Scholar]
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