- Open Access
Complex molecular mechanisms cooperate to mediate histone deacetylase inhibitors anti-tumour activity in neuroblastoma cells
Molecular Cancer volume 7, Article number: 55 (2008)
Histone deacetylase inhibitors (HDACi) are a new class of promising anti-tumour agent inhibiting cell proliferation and survival in tumour cells with very low toxicity toward normal cells. Neuroblastoma (NB) is the second most common solid tumour in children still associated with poor outcome in higher stages and, thus NB strongly requires novel treatment modalities.
We show here that the HDACi Sodium Butyrate (NaB), suberoylanilide hydroxamic acid (SAHA) and Trichostatin A (TSA) strongly reduce NB cells viability. The anti-tumour activity of these HDACi involved the induction of cell cycle arrest in the G2/M phase, followed by the activation of the intrinsic apoptotic pathway, via the activation of the caspases cascade. Moreover, HDACi mediated the activation of the pro-apoptotic proteins Bid and BimEL and the inactivation of the anti-apoptotic proteins XIAP, Bcl-xL, RIP and survivin, that further enhanced the apoptotic signal. Interestingly, the activity of these apoptosis regulators was modulated by several different mechanisms, either by caspases dependent proteolytic cleavage or by degradation via the proteasome pathway. In addition, HDACi strongly impaired the hypoxia-induced secretion of VEGF by NB cells.
HDACi are therefore interesting new anti-tumour agents for targeting highly malignant tumours such as NB, as these agents display a strong toxicity toward aggressive NB cells and they may possibly reduce angiogenesis by decreasing VEGF production by NB cells.
Histone deacetylase inhibitors (HDACi) are promising new anti-tumour agents due to their low toxicity toward normal cells and their ability to inhibit tumour growth in vivo. HDACi are currently under clinical trials and have activity in hematologic malignancies and solid tumours at doses that are well tolerated by patients [1–3].
HDACs regulate the expression and the activity of many proteins involved in cancer initiation and progression. HDACs affect gene expression by deacetylation of histones and transcription factors, and also deacetylate numerous other cellular proteins involved in cell growth, cell migration, apoptosis and differentiation [2, 4, 5]. Thus HDACi mediate their anti-tumour action by transcription-dependent and transcription-independent mechanisms. HDACi induce diverse responses in tumour cells, such as differentiation, cell cycle arrest, cell death by the activation of the intrinsic apoptotic pathway, the extrinsic apoptotic pathway, autophagic cell death, mitotic failure, senescence, and ROS facilitated cell death in tumour cells [2, 5, 6]. In addition, several HDACi affect tumour progression by their activities on angiogenesis and metastasis [4, 5, 7]. Indeed, some HDACi were shown to inhibit angiogenesis in vitro and in vivo, and to reduce the expression of pro-angiogenesis factors such as HIF-1α and VEGF [8, 9]. Particular response to HDACi vary with tumour cell type, the HDACi used, and the treatment modalities . For example, cell cycle arrest was described to occur in G1/S or in G2/M depending on the tumour cell types studied [5, 10, 11].
Neuroblastoma is the most common solid extracranial tumour in children and cause 15% of death from neoplasia in children [12, 13]. Therefore, there is an urgent clinical need for new therapeutic strategies, with improved therapeutic potential. Several reports have described the ability of HDACi such as CBHA, PB or BL1521 to induce cell cycle arrest in G1/S phase and caspase-dependent apoptosis in some NB cell lines [14–18]. The release of Bax from Ku70 following acetylation of Ku70 was shown to mediate HDACi-induced apoptosis in NB cells . Some studies have reported a reduction of NB tumour growth in vivo either on HDACi treatment alone or in combination with other treatment modalities [16, 19–22]. We have previously reported that subtoxic doses of HDACi sensitised NB cells to TRAIL-induced cell death by a caspases-dependent increase in the pro- to anti-apoptotic proteins ratio .
The present study dissects the detailed mechanisms of HDACi anti-tumour activity in NB cells, that revealed to be similar in both the S-type and N-type NB cells, in contrast to the chemotherapeutic drug Doxorubicin . The three HDACi, sodium butyrate (NaB), Trichostatin A (TSA) and suberoylanilide hydroxamic acid (SAHA) induced a cell cycle arrest in G2/M phase, followed by induction of the intrinsic apoptotic pathway, via the activation of the caspases cascade. Interestingly, HDACi increased the ratio between pro- to anti-apoptotic proteins by different mechanisms, either by caspases dependent cleavage or by degradation via the proteasome pathway. In addition, hypoxia-mediated VEGF secretion by NB cells was reduced by HDACi.
NaB, SAHA, and TSA induce cell cycle arrest in G2/M phases in NB cells
The anti-tumour activity of three HDACi, NaB, SAHA, and TSA was first analysed in various S-type and N-type NB cells. We observed that these HDACi reduced NB cell viability in a dose-dependent manner (Fig. 1A). While SH-EP cells were the less sensitive NB cells, no significant differences in the sensitivity to HDACi could be observed between S-type and N-type cells or between MYCN amplified compared to MYCN single-copy cells (Table 1).
As HDACi are known to affect both cell survival and cell cycle progression, the effect of NaB, SAHA and TSA on cell cycle progression in NB cells was then measured in SH-EP, IMR32, LAN-1 and IGR-N91 cells. After 16 h of treatment, HDACi induced an accumulation of cells with 4n DNA content indicating a G2/M cell cycle arrest (Fig. 1B, and data not shown). In addition, the number of cells in S-phase was reduced following HDACi treatments (Fig. 1B). Cell cycle arrest was not inhibited by the addition of the pan-caspase inhibitor zVAD as illustrated with SH-EP cells (Fig. 1b). Thus, NaB, SAHA and TSA induce a caspases independent cell cycle arrest in G2/M phase in both S- and N-type NB cells.
HDACi induce caspases-dependent cell death
HDACi-mediated apoptosis induction was then investigated by the propidium iodide staining method in SH-EP, LAN-1 and IMR32 cells. The percentage of sub-G1 population of cells corresponding to apoptotic cells increased over time between 24 h to 48 h (Fig. 2A and 2B). Apoptotic cell death induced by HDACi was completely protected by the pan-caspases inhibitor zVAD (Fig. 2C). These data indicate that HDACi induce caspases-dependent cell death in both S- and N-type NB cells, and apoptosis occurs following cell cycle arrest in G2/M phase.
HDACi activate the intrinsic apoptotic pathway
To analyse if HDACi induce apoptosis by activating the mitochondrial pathway, we measured the disruption of the transmembrane mitochondrial potential (ΔΨm) (Fig. 3A). Treatment of SH-EP, LAN-1 and IMR32 cells either with NaB, SAHA or TSA induced a strong reduction of the ΔΨm in 60% to 80% of these cells after 48 h of treatment. Time-course experiments showed that the disruption of the ΔΨm was enhanced between 24 h to 48 h (Fig. 3B), which correlates with the timing of apoptosis induction observed in figure 2A and 2B. The depolarisation of the membrane is partially caspases dependent, as zVAD moderately protects from reduction of the ΔΨm (data not shown). These results indicate that HDACi induce the activation of the intrinsic apoptotic pathway in NB cells.
HDACi activate the caspases cascade
As apoptosis induced by HDACi was protected by zVAD, this suggests that HDACi activate the caspases cascade. Indeed, immunoblotting analyses revealed that NaB, SAHA and TSA induce the reduction of procaspases-2, -3 and -7 in SH-EP and IMR32 cells after 48 h of treatment, while procaspase-9 was unaffected (Fig. 4A). As apoptosis was shown to be dependent of caspases activity (Fig. 2C), the reduction of pro-caspases induced by HDACi is due to their activation by proteolytic cleavage rather than other down-regulation mechanisms. Time-course analysis of caspases cleavage indicated that it occurred between 16 h to 30 h (data not shown). To confirm the caspases activation mediated by HDACi, we measured caspase-3-like activity in SH-EP and IMR32 cells using the DEVD-pNA substrate. Caspase-3-like activity was induced in cells treated with NaB, SAHA, and TSA (Fig. 4B), indicating that these HDACi induce caspases activation in both S- and N-type NB cells.
HDACi inactivate anti-apoptotic proteins by distinct mechanisms
We have previously shown that subtoxic doses of HDACi in combination with TRAIL induced the inactivation of the anti-apoptotic proteins RIP, XIAP, Bcl-xL, and survivin, as well as the activation of Bid and BimEL in a caspases dependent manner . To analyse if toxic doses of HDACi induce similar effects, the expression level of these proteins were then investigated by immunoblotting. NaB and SAHA induced the reduction of the steady state level of the anti-apoptotic proteins XIAP, Bcl-xL, RIP, and survivin, and that of the pro-apoptotic proteins Bid and BimEL, as observed in SH-EP cells (Fig. 5A) and in IMR32 cells (Fig. 5A and data not shown). These effects were observed between 16 h to 30 h of treatments (data not shown) and all except survivin were caspases-dependent as they were protected by the addition of zVAD (Fig. 5A). Indeed, zVAD did not protect the HDACi-mediated decrease in survivin expression, but on the opposite further enhanced survivin downregulation (Fig. 5A). TSA induced the same effect on XIAP, RIP, and survivin as NaB and SAHA. In contrast, Bid and Bcl-xL were not affected by TSA and the reduction of BimEL was not protected by zVAD following TSA treatment.
We next investigated whether the reduction in survivin expression level mediated by HDACi results from its degradation by the proteasome using the proteasome inhibitor Lactacystin. Results shown in figure 5B indicate that Lactacystin strongly protected from a HDACi-mediated survivin down-regulation. This indicates that in NB cells, HDACi induce proteasome-mediated degradation of survivin, rather than caspases-dependent cleavage, as previously observed in co-treatment with subtoxic doses of HDACi and TRAIL .
HDACi reduce hypoxia-induced secretion of VEGF
Certain HDACi mediate their anti-tumour activity by acting on cell cycle progression and survival, but also by affecting tumour angiogenesis via the reduction of HIF-1 and VEGF expression [4, 5]. As NB are know to express high level of VEGF, we investigated whether NaB, SAHA and TSA had an effect on VEGF expression in NB cells. Results of ELISA assay show that the amount of secreted VEGF was strongly increased by hypoxia. Interestingly, NaB, SAHA and TSA significantly reduced hypoxia-mediated increase of VEGF secretion in both S-type (SH-EP) and N-type (LAN-1 and IMR32) NB cells (Fig. 6).
We have analysed in details the mechanisms of the antitumoral effect of the HDACi NaB, SAHA and TSA on human NB cells. All cell lines analysed were strongly sensitive to NaB (at mM concentration), or to SAHA and TSA (at microM concentration), as previously described for other tumour types . With the exception of SH-EP cells, which were the less sensitive cells, all other cell lines displayed a similar sensitivity to the HDACi. Thus, no correlation could be found between the NMYC status, or the S-type versus N-type of the cells, and their sensitivity to HDACi. This is in agreement with a previous work reporting that the HDACi BL1521, TSA, and 4BP displayed a similar toxicity toward NMYC amplified and unamplified cells . In contrast, other reports indicated that S-type cells were less sensitive to TSA than N-type cells , or that the NMYC amplified SMS-KCNR cells were more sensitive to MS-27-275 than the unamplified SK-N-AS cells . In addition, in contrast to a very recent report showing that p53 is involved in the sensitivity of SH-SY5Y and SK-N-BE NB cell lines to VPA and Butyrate, we did not find any correlation between p53 status and NB cell lines sensitivity to NaB, SAHA and TSA (Table 1). These conflicting results may be explained by the fact that certain HDACi may exert their antitumoral activity by distinct mechanisms, as they selectively inhibit different HDACs [5, 27]. Indeed, we have observed that TSA differently affected several pro- and anti-apoptotic proteins compared to NaB and SAHA.
Among the HDACi-activated antitumoral actions, cell cycle arrest has been described in many type of tumours [5, 10, 11], as well as in NB [15, 16, 18]. In contrast to a previous study indicating that the HDACI BL1521 induced cell cycle arrest in G1 phase in SK-N-AS and IMR32 cells , we have shown here that NaB, SAHA and TSA induce cell cycle arrest in the G2-M phase in both S-type and N-type NB cells. This is in accordance with a very recent report showing that Butyrate and VPA induce cell cycle arrest in the G2/M phase . The cell cycle arrest induced by HDACi was observed around 16 h, preceding apoptosis induction, which occurs from 24 to 48 h. The cyclin-dependent kinase inhibitor p21 (WAF1/CIP1) is one of the most common target genes of different HDACi, and was reported to be largely associated with cell cycle arrest in G1 and G2 phases . As previously described in NB cells [18, 28], we also observed the overexpression of p21 (WAF1/CIP1) following treatment with NaB, SAHA and TSA (data not shown), thus p21 overexpression may play a role in the observed G2/M cell cycle arrest. In contrast, the cell cycle arrest was independent on p53, as several NB cells analysed express mutated p53 protein (Table 1).
We have shown here that NaB, SAHA and TSA induced caspases dependent apoptosis by the activation of the intrinsic apoptotic pathway in NB cells, as previously described in different tumours [10, 11], and in NB cells for several HDACi [16, 29]. In contrast, the involvement of TRAIL and the TRAIL-receptor pathway in HDACi-induced apoptosis was shown to vary depending on tumour cell types . Our results demonstrated that in NB cell lines, apoptosis induced by NaB, SAHA and TSA did not required a functional death receptor pathway. Indeed, the N-type NB cell lines, that are deficient in the initiator caspases-8 and -10, displayed a sensitivity to HDACi similar to that of S-type NB cells expressing these caspases. In addition, the cell surface expression level of TRAIL and TRAIL-receptor was not increased by HDACi , and SH-EP cells overexpressing FLIP  displayed similar sensitivity to HDACi than control cells (data not shown). Altogether these findings indicate that the death receptor pathway is not involved in HDACi-induced apoptosis in NB cells, despite the fact that sub-toxic doses of HDACi can sensitise NB cells to TRAIL-mediated apoptosis . Interestingly, no difference in the mechanisms of antitumoral response induced by HDACi could be observed between S-type and N-type NB cell lines. This is in contrast to the cytotoxic effect of Doxorubicin, which induced caspases-dependent cell death in S-type NB cells and caspases-independent cell death in N-type NB cells .
In this study we have further analysed in details the mechanisms of apoptosis induction by NaB, SAHA and TSA. The three HDACi increased the ratio between pro- and anti-apoptotic proteins. While NaB and SAHA mediated the downregulation of RIP, XIAP, Bcl-xL and survivin, and the activation of Bid and BimEL, TSA only induced the downregulation of XIAP, RIP and survivin. Thus, different HDACi may act through distinct mechanisms to induce their antitumoral response in the same tumour cell type.
NaB and SAHA induced the caspases-dependent activation of Bid, as Bid reduction was protected by the pan-caspase inhibitor zVAD, which also occurs in N-type NB cells in absence of caspases-8 and -10 expression. This suggests that the activation of the intrinsic pathway proceeds via an amplification loop that is independent of caspases-8 and -10, but dependent of other caspases as disruption of the ΔΨm was partially protected by zVAD (data not shown). Bid was indeed reported to be the substrate of other caspases, such as caspase-2 or caspase-3 .
The activation of BimEL by caspase-3 was previously shown to induce a positive amplification loop by increasing the affinity of BimEL to Bcl-2 . Thus, BimEL may be activated by caspases-dependent cleavage by NaB and SAHA in NB cells, as previously observed by co-treatment with subtoxic doses of HDACi and TRAIL .
Interestingly, we have observed that the down-regulation of the anti-apoptotic proteins RIP, XIAP, Bcl-xL and survivin occurred by different mechanisms, either by caspases dependent cleavage or by degradation via the proteasome pathway. Indeed, in contrast to RIP, XIAP, and Bclx, the downregulation of survivin was not protected by the caspases inhibitor zVAD, which strikingly further increased survivin downregulation. In normal cells, survivin is expressed in a cell cycle-dependent manner, with an increased expression during the G2/M phase in normal cells  and survivin degradation is tightly regulated via the ubiquitin-proteasome pathway in a cell cycle dependent manner . In tumour cells in contrast, survivin expression is globally deregulated and is overexpressed in all cell-cycle phases . Thus, our observation that HDACi-mediated downregulation of survivin in NB cells despite G2/M phase cell cycle arrest was not surprising. Survivin downregulation was prevented by the proteasome inhibitor Lactacystin, indicating that NaB, SAHA and TSA mediated survivin degradation via the ubiquitin-proteasome pathway. This is in accordance with previous reports describing that the downregulation of survivin occurred via the proteasome pathway after induction with the HDACi chlamydocin in ovarian carcicoma cells  and with valproic acid in colon cancer . Interestingly, the downregulation of survivin induced by subtoxic doses of HDACi in combination with TRAIL occurred by caspases-dependent cleavages . Thus, the mechanisms of HDACi-mediated apoptosis may vary in the same cell lines depending on the doses or the addition of combined treatment. We have shown previously that the downregulation of survivin expression by siRNA sensitised NB cells to HDACi . This suggests that part of the antitumoral effect of HDACi in NB cells may be due to the downregulation of survivin via the proteasome pathway.
In addition to the role of HDACi in reducing tumour initiation by their effects on cell proliferation and survival, HDACi were found to repress angiogenesis in vitro and in vivo, and to reduce the expression of pro-angiogenic factors, such as HIF and VEGF [5, 8, 9]. VEGF is a key regulator of angiogenesis, by inducing endothelial cell proliferation and migration . Most NB cell lines and tumours express VEGF, and VEGF expression level correlates with tumour progression and poor prognostic [40, 41]. Moreover, blockade of VEGF function was shown to be associated with suppression of NB growth [42, 43]. We have shown here that NaB, SAHA and TSA strongly decrease the hypoxia-mediated induction of VEGF secretion in both S-type and N-type NB cells. This suggests that NaB, SAHA and TSA may be efficient to reduce NB growth in vivo by decreasing tumour angiogenesis in addition to tumour cell growth and survival. Indeed, HDACi-mediated reduction of VEGF expression by 4-phenylbutyrate, or decrease of tumour vasculature by MS-27-275 have been previously described in NB tumour xenograft model [16, 20].
By dissecting the molecular pathways involved in the HDACi-mediated toxicity in NB cells, we have identified the participation of a complex array of distinct mechanisms, that outline the complexity of the HDACi-mediated effects. In addition to the observation that NaB, SAHA and TSA are potent therapeutic agents against highly malignant NB cells, by affecting both cell cycle progression and survival, our study also underlines a possible antiangiogenic action of HDACi in NB. The effect of HDACi on VEGF production thus supports HDACi anti-tumour activity reported in human NB xenograft models [19, 20] and suggests a role for the microenvironment, that should be rapidly addressed in vivo. Altogether, our and others observations confirm the interest in HDACi as promising new treatment modalities for patients with recurrent high-risk neuroblastoma.
Cell culture and reagents
The S-type NB cells SH-EP, CA2E, and SK-N-AS and the N-type NB cells LAN-1, IMR32, SH-SY-5Y, IGRN-91, IGRN-B8 were grown in DMEM medium supplemented with 2 mM L-glutamine, 100 U/ml Penicillin, 0.1 mg/ml streptomycin, and 10% of FCS. Sodium butyrate (Fluka) was dissolved in H2O and stored at -20°C. SAHA (Biovision) and TSA (Sigma) were dissolved in DMSO and store at -20°C. Cells were treated with the caspases inhibitor zVAD-fmk (100 μM, Bachem) or with Lactacystin (10 μM, Alexis Corporation) when indicated.
Cell viability assays
Cells (1–2.5*104/well in 96-well-plates; 100 μl) were plated 24 h before treatment and incubated with HDACi for 48 h. Assays were performed in quadruplicates. Viability was measured using the MTS/PMS cell proliferation kit from Promega according to manufacturer's instructions. Percentage of cell viability as compared to untreated controls was calculated.
Apoptosis and cell cycle analyses by the propidium iodide staining method
Cells were washed twice with ice-cold PBS, resuspended in 1 ml of ice-cold PBS, and fixed with 3 ml of 100% ice-cold ethanol for 1 h at 4°C. For staining with propidium iodide (PI), cells were washed twice in ice-cold PBS, resuspended in 0.2 ml of PBS containing 200 μg/ml RNaseA and 10 μg/ml propidium iodide and incubated for 30 min at room temperature. The stained cells were analyzed using a FACScan flow cytometer (Becton Dickinson).
Whole cell extracts were prepared as already described . Protein extracts (50 μg) were loaded on 12% SDS-PAGE and transferred on nitrocellulose membranes. Blots were saturated with 5% skim milk, 0.1% Tween 20 in TBS and revealed using mouse monoclonal antibodies to detect caspase-2 (Apotech Corporation), caspase-3, caspase-7, RIP, XIAP (BD Transduction Laboratories), and β-actin (Sigma). Polyclonal rabbit antibodies were used to detect caspase-9 (Cell Signaling), Bid, Bcl-xL (BD Transduction Laboratories), Bim (Imgenex), and survivin (R&D systems). Binding of the first antibody was revealed by incubation with either goat anti-mouse IgG-HRP (Jackson ImmunoResearch) or goat anti-rabbit IgG-HRP (Nordic Immunological Laboratories). Bound antibodies were detected using the Lumi-light western blotting substrate (Roche) according manufacturer's instructions.
Caspase-3 like activities were measured using the caspases-3 colorimetric protease assay kit from MBL. Cytosolic lysates were prepared after HDACi treatments according to manufacturer instructions. Two hundred μg of protein extracts were incubated with 200 μM of DEVD-pNA colorimetric substrate for 3 h at 37°C. Cell lysates were incubated with 10 μM of caspase inhibitor (zDEVD-fmk) for 30 min before addition of caspase substrate to control the specificity of caspase-3 like activation. Hydrolysed pNA was detected using a microtiter plate reader at 405 nm. Background absorbance from cell lysates and buffers were subtracted from the absorbance of stimulated and unstimulated samples before calculation of relative caspases activities.
Analysis of mitochondrial transmembrane potential
The disruption of mitochondrial membrane potential ΔΨm was analysed by staining the cells with the fluorescent dye JC-1 (Calbiochem) according to manufacturer's protocol. Loss of ΔΨm resulting in reduction of red aggregates was measured by flow cytometry using the FL2 channel (550–650 nm) (FACScan, Becton Dickinson). Results are given in percentage of cells with low ΔΨm compared to untreated controls.
Cells (2.5*106 SH-EP. 3.5*106 LAN-1 and IMR32) were platted in 75 cm2 dishes the day before induction. Cells were treated with HDACi under normoxic condition or under hypoxia (1% O2) for 24 h. Cell free supernatant were collected and whole cell extracts were prepared by incubating cell pellets in lysis buffer (50 mM Tris-HCl pH 7.4, 150 mM NaCl, 10 mM EDTA, 0.25% Triton X-100, 0.1% NP-40) supplemented protease inhibitor cocktail tablets (complete mini, Roche) for 10 min in ice. Homogenates were centrifuged 20 min. at 16'000 g and supernatant were collected. Protein concentration was measured using the micro BCA protein assay kit (Pierce). Soluble VEGF was measured in 50 μl of supernatants in duplicates using the VEGF DuoSet ELISA kit (R&D system) according to manufacturer's instructions.
histone deacetylase inhibitors
suberoylanilide hydroxamic acid
Tumour Necrosis Factor-related apoptosis-inducing ligand
cellular Flice inhibitory protein.
Villar-Garea A, Esteller M: Histone deacetylase inhibitors: understanding a new wave of anticancer agents. Int J Cancer. 2004, 112: 171-178. 10.1002/ijc.20372
Marks PA: Discovery and development of SAHA as an anticancer agent. Oncogene. 2007, 26: 1351-1356. 10.1038/sj.onc.1210204
Dokmanovic M, Clarke C, Marks PA: Histone deacetylase inhibitors: overview and perspectives. Mol Cancer Res. 2007, 5: 981-989. 10.1158/1541-7786.MCR-07-0324
Glozak MA, Seto E: Histone deacetylases and cancer. Oncogene. 2007, 26: 5420-5432. 10.1038/sj.onc.1210610
Xu WS, Parmigiani RB, Marks PA: Histone deacetylase inhibitors: molecular mechanisms of action. Oncogene. 2007, 26: 5541-5552. 10.1038/sj.onc.1210620
Secrist JP, Zhou X, Richon VM: HDAC inhibitors for the treatment of cancer. Curr Opin Investig Drugs. 2003, 4: 1422-1427.
Lindemann RK, Gabrielli B, Johnstone RW: Histone-deacetylase inhibitors for the treatment of cancer. Cell Cycle. 2004, 3: 779-788.
Deroanne CF, Bonjean K, Servotte S, Devy L, Colige A, Clausse N, Blacher S, Verdin E, Foidart JM, Nusgens BV, Castronovo V: Histone deacetylases inhibitors as anti-angiogenic agents altering vascular endothelial growth factor signaling. Oncogene. 2002, 21: 427-436. 10.1038/sj.onc.1205108
Kim MS, Kwon HJ, Lee YM, Baek JH, Jang JE, Lee SW, Moon EJ, Kim HS, Lee SK, Chung HY, Kim CW, Kim KW: Histone deacetylases induce angiogenesis by negative regulation of tumor suppressor genes. Nat Med. 2001, 7: 437-443. 10.1038/86507
Marks P, Rifkind RA, Richon VM, Breslow R, Miller T, Kelly WK: Histone deacetylases and cancer: causes and therapies. Nat Rev Cancer. 2001, 1: 194-202. 10.1038/35106079
Johnstone RW: Histone-deacetylase inhibitors: novel drugs for the treatment of cancer. Nat Rev Drug Discov. 2002, 1: 287-299. 10.1038/nrd772
Maris JM, Matthay KK: Molecular biology of neuroblastoma. J Clin Oncol. 1999, 17: 2264-2279.
Brodeur GM: Neuroblastoma: biological insights into a clinical enigma. Nat Rev Cancer. 2003, 3: 203-216. 10.1038/nrc1014
Coffey DC, Kutko MC, Glick RD, Swendeman SL, Butler L, Rifkind R, Marks PA, Richon VM, LaQuaglia MP: Histone deacetylase inhibitors and retinoic acids inhibit growth of human neuroblastoma in vitro. Med Pediatr Oncol. 2000, 35: 577-581. 10.1002/1096-911X(20001201)35:6<577::AID-MPO18>3.0.CO;2-3
Ouwehand K, de Ruijter AJ, van BC, Caron HN, van Kuilenburg AB: Histone deacetylase inhibitor BL1521 induces a G1-phase arrest in neuroblastoma cells through altered expression of cell cycle proteins. FEBS Lett. 2005, 579: 1523-1528. 10.1016/j.febslet.2005.01.058
Tang XX, Robinson ME, Riceberg JS, Kim DY, Kung B, Titus TB, Hayashi S, Flake AW, Carpentieri D, Ikegaki N: Favorable neuroblastoma genes and molecular therapeutics of neuroblastoma. Clin Cancer Res. 2004, 10: 5837-5844. 10.1158/1078-0432.CCR-04-0395
Subramanian C, Opipari AW, Bian X, Castle VP, Kwok RP: Ku70 acetylation mediates neuroblastoma cell death induced by histone deacetylase inhibitors. Proc Natl Acad Sci U S A. 2005, 102: 4842-4847. 10.1073/pnas.0408351102
De los SM, Zambrano A, Aranda A: Combined effects of retinoic acid and histone deacetylase inhibitors on human neuroblastoma SH-SY5Y cells. Mol Cancer Ther. 2007, 6: 1425-1432. 10.1158/1535-7163.MCT-06-0623
Coffey DC, Kutko MC, Glick RD, Butler LM, Heller G, Rifkind RA, Marks PA, Richon VM, La Quaglia MP: The histone deacetylase inhibitor, CBHA, inhibits growth of human neuroblastoma xenografts in vivo, alone and synergistically with all-trans retinoic acid. Cancer Res. 2001, 61: 3591-3594.
Jaboin J, Wild J, Hamidi H, Khanna C, Kim CJ, Robey R, Bates SE, Thiele CJ: MS-27-275, an inhibitor of histone deacetylase, has marked in vitro and in vivo antitumor activity against pediatric solid tumors. Cancer Res. 2002, 62: 6108-6115.
Michaelis M, Suhan T, Cinatl J, Driever PH, Cinatl J: Valproic acid and interferon-alpha synergistically inhibit neuroblastoma cell growth in vitro and in vivo. Int J Oncol. 2004, 25: 1795-1799.
Cinatl J, Cinatl J, Driever PH, Kotchetkov R, Pouckova P, Kornhuber B, Schwabe D: Sodium valproate inhibits in vivo growth of human neuroblastoma cells. Anticancer Drugs. 1997, 8: 958-963. 10.1097/00001813-199711000-00007
Muhlethaler-Mottet A, Flahaut M, Balmas BK, Auderset K, Meier R, Joseph JM, Gross N: Histone deacetylase inhibitors strongly sensitise neuroblastoma cells to TRAIL-induced apoptosis by a caspases-dependent increase of the pro- to anti-apoptotic proteins ratio. BMC Cancer. 2006, 6: 214- 10.1186/1471-2407-6-214
Hopkins-Donaldson S, Yan P, Bourloud KB, Muhlethaler A, Bodmer JL, Gross N: Doxorubicin-induced death in neuroblastoma does not involve death receptors in S-type cells and is caspase-independent in N-type cells. Oncogene. 2002, 21: 6132-6137. 10.1038/sj.onc.1205879
de Ruijter AJ, Kemp S, Kramer G, Meinsma RJ, Kaufmann JO, Caron HN, van Kuilenburg AB: The novel histone deacetylase inhibitor BL1521 inhibits proliferation and induces apoptosis in neuroblastoma cells. Biochem Pharmacol. 2004, 68: 1279-1288. 10.1016/j.bcp.2004.05.010
Subramanian C, Jarzembowski JA, Opipari AW, Castle VP, Kwok RP: CREB-binding protein is a mediator of neuroblastoma cell death induced by the histone deacetylase inhibitor trichostatin A. Neoplasia. 2007, 9: 495-503. 10.1593/neo.07262
Dokmanovic M, Marks PA: Prospects: histone deacetylase inhibitors. J Cell Biochem. 2005, 96: 293-304. 10.1002/jcb.20532
Condorelli F, Gnemmi I, Vallario A, Genazzani AA, Canonico PL: Inhibitors of histone deacetylase (HDAC) restore the p53 pathway in neuroblastoma cells. Br J Pharmacol. 2008, 153: 657-668. 10.1038/sj.bjp.0707608
Glick RD, Swendeman SL, Coffey DC, Rifkind RA, Marks PA, Richon VM, La Quaglia MP: Hybrid polar histone deacetylase inhibitor induces apoptosis and CD95/CD95 ligand expression in human neuroblastoma. Cancer Res. 1999, 59: 4392-4399.
Minucci S, Pelicci PG: Histone deacetylase inhibitors and the promise of epigenetic (and more) treatments for cancer. Nat Rev Cancer. 2006, 6: 38-51. 10.1038/nrc1779
Flahaut M, Muhlethaler-Mottet A, Auderset K, Bourloud KB, Meier R, Popovic MB, Joseph JM, Gross N: Persistent inhibition of FLIP(L) expression by lentiviral small hairpin RNA delivery restores death-receptor-induced apoptosis in neuroblastoma cells. Apoptosis. 2006, 11: 255-263. 10.1007/s10495-006-3435-9
Yin XM: Bid, a BH3-only multi-functional molecule, is at the cross road of life and death. Gene. 2006, 369: 7-19. 10.1016/j.gene.2005.10.038
Chen D, Zhou Q: Caspase cleavage of BimEL triggers a positive feedback amplification of apoptotic signaling. Proc Natl Acad Sci U S A. 2004, 101: 1235-1240. 10.1073/pnas.0308050100
Li F, Ambrosini G, Chu EY, Plescia J, Tognin S, Marchisio PC, Altieri DC: Control of apoptosis and mitotic spindle checkpoint by survivin. Nature. 1998, 396: 580-584. 10.1038/25141
Zhao J, Tenev T, Martins LM, Downward J, Lemoine NR: The ubiquitin-proteasome pathway regulates survivin degradation in a cell cycle-dependent manner. J Cell Sci. 2000, 113 Pt 23: 4363-4371.
Altieri DC: Validating survivin as a cancer therapeutic target. Nat Rev Cancer. 2003, 3: 46-54. 10.1038/nrc968
S. DS, Bruwiere H, Verhulst T, Steller U, Andries L, Wouters W, Janicot M, Arts J, Van HJ: Inhibition of histone deacetylases by chlamydocin induces apoptosis and proteasome-mediated degradation of survivin. J Pharmacol Exp Ther. 2003, 304: 881-888. 10.1124/jpet.102.042903
Huang X, Guo B: Adenomatous polyposis coli determines sensitivity to histone deacetylase inhibitor-induced apoptosis in colon cancer cells. Cancer Res. 2006, 66: 9245-9251. 10.1158/0008-5472.CAN-06-0887
Ferrara N, Gerber HP, LeCouter J: The biology of VEGF and its receptors. Nat Med. 2003, 9: 669-676. 10.1038/nm0603-669
Meister B, Grunebach F, Bautz F, Brugger W, Fink FM, Kanz L, Mohle R: Expression of vascular endothelial growth factor (VEGF) and its receptors in human neuroblastoma. Eur J Cancer. 1999, 35: 445-449. 10.1016/S0959-8049(98)00387-6
Eggert A, Ikegaki N, Kwiatkowski J, Zhao H, Brodeur GM, Himelstein BP: High-level expression of angiogenic factors is associated with advanced tumor stage in human neuroblastomas. Clin Cancer Res. 2000, 6: 1900-1908.
Kim ES, Serur A, Huang J, Manley CA, McCrudden KW, Frischer JS, Soffer SZ, Ring L, New T, Zabski S, Rudge JS, Holash J, Yancopoulos GD, Kandel JJ, Yamashiro DJ: Potent VEGF blockade causes regression of coopted vessels in a model of neuroblastoma. Proc Natl Acad Sci U S A. 2002, 99: 11399-11404. 10.1073/pnas.172398399
Segerstrom L, Fuchs D, Backman U, Holmquist K, Christofferson R, Azarbayjani F: The anti-VEGF antibody bevacizumab potently reduces the growth rate of high-risk neuroblastoma xenografts. Pediatr Res. 2006, 60: 576-581. 10.1203/01.pdr.0000242494.94000.52
Hopkins-Donaldson S, Bodmer JL, Bourloud KB, Brognara CB, Tschopp J, Gross N: Loss of caspase-8 expression in highly malignant human neuroblastoma cells correlates with resistance to tumor necrosis factor-related apoptosis-inducing ligand-induced apoptosis. Cancer Res. 2000, 60: 4315-4319.
Nakamura Y, Ozaki T, Niizuma H, Ohira M, Kamijo T, Nakagawara A: Functional characterization of a new p53 mutant generated by homozygous deletion in a neuroblastoma cell line. Biochem Biophys Res Commun. 2007, 354: 892-898. 10.1016/j.bbrc.2007.01.057
Goldschneider D, Horvilleur E, Plassa LF, Guillaud-Bataille M, Million K, Wittmer-Dupret E, Danglot G, de TH, Benard J, May E, Douc-Rasy S: Expression of C-terminal deleted p53 isoforms in neuroblastoma. Nucleic Acids Res. 2006, 34: 5603-5612. 10.1093/nar/gkl619
Tweddle DA, Malcolm AJ, Bown N, Pearson AD, Lunec J: Evidence for the development of p53 mutations after cytotoxic therapy in a neuroblastoma cell line. Cancer Res. 2001, 61: 8-13.
Goldschneider D, Blanc E, Raguenez G, Barrois M, Legrand A, Le RG, Haddada H, Benard J, Douc-Rasy S: Differential response of p53 target genes to p73 overexpression in SH-SY5Y neuroblastoma cell line. J Cell Sci. 2004, 117: 293-301. 10.1242/jcs.00834
We thank C. Ruegg for providing us the equipment to performed cell culture in hypoxia. This work was supported by grants from the Faculty of Biology and Medicine of the University of Lausanne, the Novartis, the FORCE and the Swiss Research Kind und Krebs Foundations.
The authors declare that they have no competing interests.
AMM performed all major experimental work, participated in the design, the coordination of the study and drafted the manuscript, KBB participated in all cell culture experiments and performed the immunoblots, caspases activity assays, KA participated in VEGF measurement and in cells stimulation with drugs, MF developed the SH-EP FLIP cells, RM participated in cell treatments with HDACIs, JMJ and NG were involved in the overall design of the study and helped to draft the manuscript.
Authors’ original submitted files for images
Below are the links to the authors’ original submitted files for images.
Rights and permissions
Open Access This article is published under license to BioMed Central Ltd. This is an Open Access article is distributed under the terms of the Creative Commons Attribution License ( https://creativecommons.org/licenses/by/2.0 ), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.
About this article
Cite this article
Mühlethaler-Mottet, A., Meier, R., Flahaut, M. et al. Complex molecular mechanisms cooperate to mediate histone deacetylase inhibitors anti-tumour activity in neuroblastoma cells. Mol Cancer 7, 55 (2008). https://doi.org/10.1186/1476-4598-7-55
- Cell Cycle Arrest
- Survivin Expression
- Sodium Butyrate