|The anticancer effects of chaetocin are independent of programmed cell death and hypoxia, and are associated with inhibition of endothelial cell proliferation.|
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|PMID: 22187030 Owner: NLM Status: MEDLINE|
|BACKGROUND: We previously reported that chaetocin has potent and selective anti-myeloma activity attributable to reactive oxygen species (ROS) induction imposed by inhibition of the redox enzyme thioredoxin reductase; we now detail its effects in solid tumours.
METHODS: Cellular assays, transcriptional profiling and the NCI60 screen were used to assess the effects of chaetocin in solid tumour and endothelial cells.
RESULTS: NCI-60 screening demonstrated chaetocin to even more potently inhibit proliferation in solid tumour than in haematological cell lines; transcriptional profiling revealed a signature consistent with induction of inflammatory response and cell death pathways. Chaetocin induced ROS, oxidative damage to cellular proteins and apoptosis, with 2-10 nM IC(50)s (24 h exposures) in all tested solid tumour cell lines. The pan-caspase inhibitor zVAD-fmk did not block chaetocin-induced cell death despite inhibiting mitochondrial membrane depolarisation and apoptosis. Further, Molt-4 rho(0) cells lacking metabolically functional mitochondria were readily killed by chaetocin; in addition chaetocin-induced cytotoxicity was unaffected by autophagy inhibitors or hypoxia and consequent HIF-1α upregulation. Moreover, chaetocin inhibited SKOV3 ovarian cancer xenografts producing less vascular tumours, and inhibited human umbilical vein endothelial cell proliferation.
CONCLUSION: Chaetocin has intriguing and wide-ranging in vitro and in vivo anticancer effects, and is an attractive candidate for further preclinical and clinical development.
|C R Isham; J D Tibodeau; A R Bossou; J R Merchan; K C Bible|
|Type: Journal Article; Research Support, N.I.H., Extramural Date: 2011-12-20|
|Title: British journal of cancer Volume: 106 ISSN: 1532-1827 ISO Abbreviation: Br. J. Cancer Publication Date: 2012 Jan|
|Created Date: 2012-01-18 Completed Date: 2012-03-02 Revised Date: 2013-06-26|
Medline Journal Info:
|Nlm Unique ID: 0370635 Medline TA: Br J Cancer Country: England|
|Languages: eng Pagination: 314-23 Citation Subset: IM|
|Department of Oncology, Mayo Clinic, 200 First Street SW, Rochester, MN 55905, USA.|
|APA/MLA Format Download EndNote Download BibTex|
Antineoplastic Agents / pharmacology*
Apoptosis / drug effects*
Cell Hypoxia / drug effects*
Cell Line, Tumor
Cell Proliferation / drug effects*
Endothelium, Vascular / drug effects*, pathology
Gene Expression Profiling
Hypoxia-Inducible Factor 1, alpha Subunit / metabolism
Piperazines / pharmacology
RNA, Messenger / genetics
Reactive Oxygen Species
Vascular Endothelial Growth Factor Receptor-1 / metabolism
Xenograft Model Antitumor Assays
|CA125750/CA/NCI NIH HHS; R01 CA125750-05/CA/NCI NIH HHS|
|0/Antineoplastic Agents; 0/HIF1A protein, human; 0/Hypoxia-Inducible Factor 1, alpha Subunit; 0/Piperazines; 0/RNA, Messenger; 0/Reactive Oxygen Species; 28097-03-2/chaetocin; EC 188.8.131.52/Vascular Endothelial Growth Factor Receptor-1|
Journal ID (nlm-ta): Br J Cancer
Publisher: Nature Publishing Group
Copyright © 2012 Cancer Research UK
Revision Received Day: 31 Month: 10 Year: 2011
Accepted Day: 07 Month: 11 Year: 2011
Print publication date: Day: 17 Month: 01 Year: 2012
Electronic publication date: Day: 20 Month: 12 Year: 2011
Volume: 106 Issue: 2
First Page: 314 Last Page: 323
PubMed Id: 22187030
Publisher Item Identifier: bjc2011522
|The anticancer effects of chaetocin are independent of programmed cell death and hypoxia, and are associated with inhibition of endothelial cell proliferation Alternate Title:Effects of chaetocin in solid tumours|
|C R Isham1|
|J D Tibodeau1|
|A R Bossou1|
|J R Merchan2|
|K C Bible1*|
1Department of Oncology, Mayo Clinic, 200 First Street SW, Rochester, MN 55905, USA
2Sylvester Comprehensive Cancer Center, University of Miami School of Medicine, 1475 NW 12th Avenue (D-1), Miami, FL 33136, USA
Chaetocin is a natural product produced by Chaetomium spp. and related fungi (Sekita et al, 1981; Freire et al, 2000) with its structure elucidated in 1970 (Hauser et al, 1970) indicating an unusual bridged disulphide diketopiperazine core. We became interested in chaetocin initially because of its unique chemical structure, discovering that it has potent and selective in vitro, ex vivo and in vivo anti-myeloma activity attributable to its ability to impose cellular oxidative stress (Isham et al, 2007). Subsequently, we discovered that chaetocin serves as a competitive substrate (with respect to thioredoxin) and an inhibitor of the redox enzyme thioredoxin reductase, apparently thereby accounting for its ability to induce cellular oxidative stress and kill tumour cells, as we were unable to define other effects of chaetocin on reactive oxygen species (ROS) or ROS remediation systems to otherwise account for observed effects (Tibodeau et al, 2009). Chaetocin has also been found by others to inhibit histone methyltransferase SU(VAR)3–9 (Greiner et al, 2005) and HIF-1a signalling (Kung et al, 2004; Lee et al, 2011)—with interest in the compound sufficient to prompt its recent total synthesis (Iwasa et al, 2010; Kim and Movassaghi, 2010). As chaetocin serves as a potent inducer of cellular ROS, apparently consequent to its ability to inhibit thioredoxin reductase-mediated ROS remediation, we postulated that chaetocin might not only have activity in myeloma, but also in solid tumours, as the imposition of cellular ROS has been postulated to represent an attractive candidate therapeutic strategy in solid tumours (Fang et al, 2007). We had initially anticipated that its effects might be greatest in haematological tumours, but NCI-60 screening unexpectedly indicated chaetocin to be even more potent in solid tumours, prompting the present more extensive studies.
Chaetocin (Sigma, St Louis, MO, USA) was supplied to the National Cancer Institute for evaluation in the 60 human tumour cell line tumour panel, which they performed as previously described (Monks et al, 1991).
Total RNA was purified from both A549 and OCI-MY-5 cells treated with chaetocin for 24 h using TRIzol (Invitrogen, Carlsbad, CA, USA) reagent followed by RNeasy kit (Qiagen, Valencia, CA, USA). The resulting purified RNA was submitted to the Advanced Genomic Technology Centre Microarray Shared Resource at Mayo Clinic for RNA integrity analysis on the Agilent 2100 Bioanalyzer (Agilent Technologies, Palo Alto, CA, USA), reverse transcription, labelling and hybridisation to Affymetrix human U133 Plus 2.0 arrays (Affymetrix, Santa Clara, CA, USA). Affymetrix arrays were scanned with the GeneChip 3000 Scanner (Affymetrix). Significant data sets were generated using GeneSpring (Agilent Technologies) and by our statisticians. Common top pathways were generated from the data sets using GeneGo (St Joseph, MI, USA).
Cells were cultured in the following media: A549, U2OS, HCT116, and HeLa in RPMI 1640 containing 5% FBS; OCI-MY5 in RPMI 1640 containing 10% FBS; PC-3 cells in F12 medium containing 10% FBS; SKOV3 in McCoy's 5a containing 10% FBS; HEPG2 in Dulbecco's modified Eagle's Medium (DMEM) containing 10% FBS and MCF7 cells in Iscove's modified essential medium containing 5% FBS. All media contained 100 U ml−1 penicillin G and 100 μg ml−1 streptomycin. Cell lines were passaged twice weekly and maintained at 37 °C (95% air, 5% CO2). For hypoxia experiments, HEPG2 and SKOV3 cells were maintained at 37 °C instead in an atmosphere containing 94% N2, 1% O2 and 5% CO2. OCI-MY5 cells were kindly provided by Dr Diane Jelinek (Mayo Clinic, Rochester, MN, USA). All other cell lines were originally obtained from ATCC (Chicago, IL, USA).
MOLT-4 cells lacking mtDNA were produced by culture in DMEM containing 4500 mg l−1 glucose and 1 m pyruvate supplemented with 5% FBS, 50 μg ml−1 uridine, and 50 ng ml−1 ethidium bromide. Cells are allowed to grow for 3–4 weeks in the presence of ethidium bromide in order to isolate cells that completely lack mtDNA. After the confirmation of mtDNA depletion (by either withdrawing uridine from the medium and observing cell death, by western blotting of proteins, including COX I and COX II, or by measuring the oxygen consumption of selected versus parental cells), cells were maintained in DMEM supplemented with 5% FBS and 50 μg ml−1 uridine so as to retain the mtDNA-dead phenotype.
Briefly, 500 cells obtained by trypsinisation from stock flasks of subconfluent cells were plated into each of the triplicate sets of 35 mm tissue culture plates and allowed to adhere overnight. Cells were then treated for the indicated times with diluent, chaetocin or as otherwise specified. Where indicated, cells were preincubated with N-acetyl cysteine (NAC; Sigma) 30 min before drug addition. After drug removal and washing twice with media, cells were allowed to proliferate in a drug-free medium for 7–10 days; thereafter plates were washed, stained with Coomassie blue, and colonies were counted on an imager using GeneTools software (Syngene, Frederick, MD, USA).
Cellular oxidative stress was assessed utilising 5,6-chloromethyl-2′,7′-dichlorodihydrofluorescein diacetate (CM-DCF) as a cell permeable fluorescent probe with FACS analysis. Briefly, cells were treated with the indicated drug for 24 h, the media was removed, and the cells were then incubated in warm PBS containing 6 μ probe at 37 °C for 1 h. The probe was then removed and warm media was added back to the cells for 10 min. The cells were then trypsinised, sedimented, and resuspended in cold PBS before flow microfluorimetry using a FACScan flow cytometer (Becton Dickinson, Mountain View, CA, USA) with a 488 nm laser. Fluorescence emission was observed through a 530/30 nm filter, and 20 000 events were analysed using CellQuest software (Verity Software House, Topsham, ME, USA). In separate experiments, the tested compounds were found not to directly interact with the probe in vitro, as no fluorescence emission was observed at a 1 : 10 dye:compound ratio.
Protein lysates were prepared in CelLytic buffer (Sigma) containing 50 m DTT from HeLa cells treated with various doses of chaetocin for 24 h, with a 30 min preincubation with NAC where indicated. Protein concentrations of the lysates were measured by BCA assay (Thermo Fisher Scientific Inc., Rockford, IL, USA) and 20 μg of protein was used for the OxyBlot Protein Oxidation Detection assay (Chemicon International, Temecula, CA, USA). Samples were denatured with 6% SDS incubated with the provided DNPH solution to derivatise any carbonyl groups for 15 min, and the reaction was stopped with the provided neutralisation solution. The samples were then run on a 10% Bis-Tris SDS–PAGE gel and transferred to a nitrocellulose membrane. Resulting membranes were blocked for 1 h in 1% BSA, then incubated for 1 h with primary antibody specific to DNP residues, and then incubated with an HRP-conjugated secondary antibody for 1 h. Pierce West Pico chemiluminescent detection reagent (Thermo Fisher Scientific Inc.) was added and membranes were exposed to the film.
Cells for transmission electron microscopy were released by trypsinisation, washed twice with PBS, fixed for 1 h with Trump's fixative (1% glutaraldehyde and 4% formaldehyde in 0.1 phosphate buffer (pH 7.2)), treated with phosphate-buffered 1% 0504, stained en bloc with 2% uranyl acetate for 30 min at 60 °C and embedded in Spurr's resin. Sections (90 nm) were cut on a Reichert Ultracut E or S Ultramicrotome (Leica, Inc., Vienna, Austria), collected on 200-mesh copper grids, stained with lead citrate, and examined and photographed with a JOEL 1200 EXII electron microscope (Tokyo, Japan) operating at 60 kV.
Harvested and washed cell suspensions fixed with methanol/acetic acid (3 : 1) were mixed in equal parts with 1 μg ml−1 Hoechst 33 258 (Sigma) solubilised in 50% glycerol and 50 m Tris pH 7, with the induction of apoptosis assessed using fluorescence microscopy by examining cells for apoptotic morphological changes, expressing the number of apoptotic cells at a percentage of 200 total counted cells.
Chaetocin-treated A549 cells were sedimented, washed with PBS, resuspended in medium, stained with TMRM (Tetramethylrhodamine methyl ester, Invitrogen; 50 n, 45 min, 37 °C), placed on ice for 5 min and immediately subjected to flow microfluorometry using a FACScan flow cytometer (Becton Dickinson, 488 nm laser). Fluorescence emission was observed through a 585/42 nm filter, and 20 000 events were analysed using CellQuest software (Verity Software House).
After maintaining and treating the cells as indicated, cold PBS was immediately added, plates were washed twice in cold PBS and adherent cells were lysed in CelLytic lysis buffer (Sigma) containing protease inhibitors (Roche, Indianapolis, IN, USA). As HIF1α is subject to nuclear translocation, samples were sonicated for all experiments assessing HIF1α. Total cellular protein was analysed by BCA assay to facilitate equal sample loading, and lysates were electrophoresed on 7.5% SDS–PAGE gels and transferred onto nitrocellulose. Immunoblotting for HIF1α (Abcam, Cambridge, MA, USA), vascular endothelial growth factor receptor (VEGFR-1; Cell Signaling), phosphorylated VEGFR-1 (anti-phospho-Flt-1 Tyr1213; Millipore, Temecula, CA, USA) and actin were then performed.
Mouse experiments followed institutional guidelines and were approved by the Institutional Animal Care and Use Committee (IACUC). Briefly, SKOV3 cells were harvested, washed twice and resuspended in PBS (2.5 million cells per 100 μL). Female athymic nu/nu mice (5–6 weeks old) purchased from Harlan Laboratories, Inc. (Indianapolis, IN, USA) were anaesthetised using isoflurane, and were injected subcutaneously in the flank with 100 μl of SKOV3 inoculum. After measurable 4–5 mm tumours were formed, the mice were randomly assigned to control or experimental groups: 0.2 mg kg−1 IP 5 × per week of chaetocin (in 0.17% DMSO, 20% polyethylene glycol 400; remainder 0.9% NaCl). Tumours were measured with calipers three times weekly, and tumour volumes were calculated using the formula: volume=A × B × B/2, (where A was the longest tumour dimension and B the smallest).
A total of 4 × 103 HuVECs (Lonza, Walkersville, MD, USA) in 100 μl medium with 1% FBS, penicillin (100 U ml−1), and streptomycin (100 μg ml−1) was placed into each well of a 96-well plate, treated with chaetocin at indicated concentrations, and incubated at 37 °C for 72 h. Either βFGF (PeproTech, Rocky Hill, NJ, USA; 20 ng ml−1) or EGM-2 medium (containing hEGF, VEGF, hFGF-B, R3-IGF-1; Lonza) was used to induce HuVEC proliferation as indicated. After the 72-h incubation, WST-1 (10 μl; Roche, Mannheim, Germany) was added to each well, and after a 3-h incubation at 37 °C, absorbance at 450 nm was determined for each well with a microplate reader (Bio-Rad Laboratories, Hercules, CA, USA). Data presented are the average of triplicate experiments.
In preliminary studies, we examined the effects of chaetocin on cancer cell proliferation using the NCI-60 screen (Monks et al, 1991). Although we had previously found chaetocin to have potent anti-myeloma activity, interestingly, NCI-60 results indicated even more potent inhibition of solid tumour than haematological cell line proliferation by chaetocin (Figure 1). Follow-up colony formation assays confirmed the potent antineoplastic effects of chaetocin in a wide range of solid tumour cell lines, with 2–10 n IC50s (24 h exposure) in all assayed lines (Figure 2A). As short as 4 h chaetocin exposure produced near maximal growth-inhibitory effects in A549 cells (Figure 2B).
Consistent with prior observations in myeloma cells and cell lines (Isham et al, 2007) glutathione (GSH) or its cell permeable precursor NACdramatically attenuated chaetocin-induced (i) reduction in colony formation (Figure 2A), (ii) induction of ROS (Figure 2C), and (iii) oxidation of cellular proteins (Figure 2D) without either GSH or NAC directly reducing chaetocin itself (Tibodeau et al, 2009), implicating the induction of cellular oxidative stress/ROS by chaetocin as critical to its observed in vitro solid tumour antineoplastic activity.
As one tool to further examine the cellular effects of chaetocin in solid tumours, we utilised transcriptional profiling targeting identification of transcripts consistently altered by chaetocin across both myeloma and solid tumour cell lines. Interestingly, when comparing the transcriptional profiling results attained in response to identical chaetocin exposures (100 n × 24 h, Affymetrix platform) in the A549 non-small cell lung cancer vs the OCI-MY5 myeloma cell line, it was notable that many more significantly altered transcripts arose in OCI-MY5 compared with A549 cells (Figure 3A). Of the two results, only 48 transcripts were similarly and significantly altered in both cell lines (Table 1); these were analysed using GeneGo software to help elaborate pathways and biological processes altered by chaetocin treatment over control diluent/DMSO treatment (Figure 3B and C). Transcripts related to inflammatory response and cell death/apoptosis pathways were most commonly altered, presumably indicating cellular response to chaetocin-induced oxidative stress as well as compensatory survival signalling pathway activation.
Electron microscopy demonstrated the induction of complex structural changes in A549 cells treated with chaetocin (400 n, 24 h exposure) that included apoptotic morphology (chromatin condensation on the nuclear periphery in early apoptotic cells (EA) and pro-apoptotic bodies (AB) in late apoptotic cells), as well as occasional double membrane vacuole (DM) formation and filled autophagic vacuoles (AV), indicating autophagy (Figure 4A). These results raised questions as to on which cell death pathway(s) may chaetocin cytotoxicity depend, prompting further and more detailed experiments.
In order to study whether chaetocin-induced ROS induction and cell death might be dependant upon intact apoptotic pathways, experiments were next carried out using an apoptosis inhibitor. Although, as expected, apoptosis was dramatically reduced by co-treatment with the pan-caspase inhibitor zVAD-fmk (Figure 4B); chaetocin-induced cell death was only minimally affected (Figure 4C). In parallel, zVAD-fmk also greatly attenuated mitochondrial membrane depolarisation induced by chaetocin (Figure 4D), but not ROS induction (Figure 4E), altogether indicating that chaetocin-induced cellular oxidative stress and cell death are largely independent of apoptosis induction. This is consistent with the hypothesis that chaetocin induces cellular ROS in a manner independent of mitochondrial ROS release occurring in response to mitochondrial membrane depolarisation in conjunction with the induction of apoptosis.
As chaetocin treatment led to the formation of both single and bimembrane vacuoles in A549 cells (Figure 4A), suggesting that autophagic pathways might be induced, we also examined the effects of the autophagy inhibitors 3-methyladenine or SP600125 on chaetocin-induced cell death in A549 cells. Neither the PI3 kinase and autophagic inhibitor 3-methyladenine nor the Jun kinase and autophagic inhibitor SP600125 attenuated chaetocin-induced cell death or apoptosis (Figure 4B and C); furthermore, we observed no discernible alterations in MAP-LC3 or Beclin-1 protein level in response to chaetocin treatment (data not shown). Collectively these data indicate that the induction of autophagy, as well as apoptosis, appear not required for the in vitro antineoplastic effects of chaetocin.
As it is known that mitochondria are a major source of cellular ROS, and as chaetocin potently induces ROS (Figure 2C) and was observed to induce mitochondrial membrane depolarisation (Figure 4D), we also examined whether chaetocin-induced cell death and/or ROS induction might be dependant upon metabolically functional mitochondria. Neither the cytotoxic effects nor the induction of ROS by chaetocin differed in response to treatment of parental Molt-4 or Molt-4 rho0 cells with metabolically inactive mitochondria (Figure 5A and B), bolstering other data (Figure 4C and E) in support of the hypothesis that the ability of chaetocin to induce ROS and cell death in vitro appear not to require metabolic ROS production or release from mitochondria despite the ability of chaetocin to induce mitochondrial membrane depolarisation and apoptosis (Figure 4A, B and D). These data are consistent with our prior report indicating that chaetocin does not itself directly induce oxidative stress, but instead apparently triggers cellular ROS accumulation by inhibition of the redox enzyme thioredoxin reductase (Tibodeau et al, 2009).
As chaetocin-induced cell death is dependant upon its ability to induce the production of cellular oxidative species (e.g., Figure 2), we became concerned that such effects might be attenuated under hypoxic conditions whereby oxygen tension was reduced and HIF-1α was induced. This concern turned out to be unfounded, as we observed slightly enhanced, not attenuated, induction of cell death by chaetocin under in vitro hypoxic conditions whereby HIF-1α was potently induced (Figure 5C). In addition, of interest is that in vitro cytotoxicity of chaetocin was observed to be robust even in the absence of detectable HIF-1α (Figure 5C), seemingly in deference to a prior report indicating that chaetocin-induced antitumour effects are dependant upon the presence of functional HIF-1α (Lee et al, 2011).
As chaetocin demonstrated potent in vitro antineoplastic effects in solid tumour cell lines not attenuated by hypoxia-stimulated HIF-1α induction, we hypothesised that chaetocin might also have in vivo antineoplastic effects in solid tumours, akin to those observed in myeloma (Isham et al, 2007). Although we had previously found chaetocin at low dosages to be well tolerated when intraperitoneally administered in mice (Isham et al, 2007), in preparation for the present in vivo experiments, we first carefully assessed the potential deleterious effects of chaetocin in animals not bearing tumours when treated with escalating chaetocin doses and administration schedules.
To establish the maximally tolerated dosage in response to intraperitoneal chaetocin administration, an IACUC-approved approach akin to that used in human dosage-escalation studies was applied, incrementing doses and the frequency of intraperitoneally administered chaetocin in a stepwise manner so as to gradually increase chaetocin dose-density and enhance the detection of early signs of toxicities. The only observed toxicities from the administration of higher chaetocin dose-density in mice related to evidence of peritoneal irritation associated with IP administration (adhesions, and upon occasion bloody ascites); no evidence of adverse effects of chaetocin treatment on solid organs was noted, and observed peritoneal changes were not observed to have influenced animal feeding behaviour or activity level. Observed peritoneal irritation seemed related primarily to the quantity of chaetocin administered with each IP injection; this accounts for our shift to a 5 × per week administration schedule, allowing us to define the maximally tolerated IP dosing as 0.2 mg kg−1 5 × per week in mice.
Compared with diluent control treatment, chaetocin treatment (0.2 mg kg−1 IP 5 × per week) significantly delayed the growth of established SKOV3 tumours (Figure 6A), with minimal evidence of toxicities observed in treated animals. We noted in parallel that excised tumours from chaetocin-treated animals were less vascular in comparison with diluent control tumours (Figure 6B), raising the question of whether anti-angiogenic effects might be in part contributory to observed in vivo efficacy, and leading to additional experiments.
Seeking a potential explanation for why chaetocin-treated tumours were seemingly less vascular, and realising that phospho-VEGFR-1 level would be expected to represent a surrogate marker for the extent of VEGF activity in xenograft tumours, we examined tumour levels of both total and phospho-VEGFR-1 in homogenate of excised xenografts. Although the mean tumour total VEGFR-1 protein level (assessed by immunoblotting of tumour lysates normalised to paired tumour actin levels) was significantly reduced in chaetocin-treated tumours relative to diluent-treated controls, the corresponding mean phospho-VEGFR-1 level did not differ between the groups (Figure 6C), suggesting that the observed differences in tumour vascularity were not likely attributable to differential VEGFR-1 activation. In parallel, we also examined HIF-1α protein levels in treated vs control tumour lysates and additionally in treated vs control SKOV3 cells in vitro; in each instance HIF-1α was barely detectable, providing no indication that HIF-1α was required for the antitumour effects of chaetocin in vitro or in vivo in the utilised SKOV3 model systems.
Seeking an alternative potential explanation for the attenuated vascularity observed in SKOV3 tumours excised from chaetocin-treated animals, we went on to examin the effects of chaetocin on the proliferation of HuVECs. Chaetocin potently attenuated HuVEC proliferation stimulated by either interleukin or EGM2 endothelial cell growth medium (Figure 6D and E), suggesting that the anti-proliferative effects of chaetocin on tumour microvasculature might alternatively be a contributor to the observed attenuated vascularity and in vivo effects of chaetocin (Figure 6A and B), and raising the intriguing possibility that chaetocin may function in vivo not only by targeting tumour directly, but perhaps also in part by simultaneously targeting endothelial cells in the tumour microenvironment.
Presented results importantly demonstrate that chaetocin has substantial activity in solid tumour models and not just in multiple myeloma as we had previously reported. It is particularly intriguing that the antineoplastic effects of chaetocin in solid tumour cell lines (assessed in the NCI-60 screen, Figure 1) are in fact almost uniformly superior to those seen in multiple myeloma and other haematological tumours; this was unanticipated. Moreover, it is noteworthy that observed solid tumour activity translates in vivo, as chaetocin potently inhibited SKOV3 ovarian cancer xenografts (Figure 6A and B). Consequently, chaetocin would seem to represent at least as promising a candidate that is therapeutic in solid tumours as in myeloma.
Present studies also add important knowledge related to the effects of chaetocin in relation to programmed cell death (PCD) pathways in solid tumours. As in multiple myeloma, chaetocin potently induces cellular oxidative stress/ROS in solid tumour cell lines that is required for in vitro antineoplastic efficacy, as blocking ROS production by NAC co-treatment abrogates the in vitro cytotoxic effects of chaetocin (e.g., Figure 2A) without directly reducing chaetocin (Tibodeau et al, 2009). Interestingly, although chaetocin induces mitochondrial membrane depolarisation and apoptosis, chaetocin-induced ROS and cell death appear nonetheless not dependant upon these phenomena (Figure 4). Likewise, although chaetocin induces morphological changes, including vacuole formation, that might be interpreted as associated with autophagy, autophagy also appears not to contribute to chaetocin-induced cytotoxicity, as autophagy inhibitors similarly do not block chaetocin-induced cell death (Figure 4). Considered collectively, our results indicate that chaetocin can kill cancer cells apparently by the induction of necrotic cell death, largely independent of reliance on intact PCD pathways. We interpret these results as quite promising and important as they suggest that chaetocin has potential to therefore be effective in killing cancer cells even harbouring defective PCD pathways that might otherwise render them resistant to other therapeutics.
In this regard, we hypothesise that the imposition of intracellular ROS by chaetocin by inhibition of thioredoxin reductase (Isham et al, 2007; Tibodeau et al, 2009) serves as a catastrophic cellular insult that can kill cells by necrosis even if apoptotic and autophagic pathways are disregulated. However, as the induction of cellular ROS might be expected to kill normal as well as malignant cells, the question arises as to why chaetocin might have anti-tumour selectivity, killing cancer cells whereas sparing normal cells—as we have clearly demonstrated to be the case in both myeloma (Isham et al, 2007), as well as also in the case of the SKOV3 solid tumour model (Figure 6). Our hypothesis in this regard is that cancer cells often display increased levels of basal cellular ROS relative to normal cells, in part because of the shift from energy production via the Krebs cycles instead of glycolysis (the ‘Warburg effect') in cancer cells. In this scenario, because of the higher basal ROS levels in cancer cells, the imposition of cellular oxidative stress would more likely overwhelm ROS remediation systems in cancer cells than in normal cells, thereby potentially rendering cancer cells more sensitive than normal cells to redox-targeted agents like chaetocin (Fang et al, 2007). In this respect, our prior work (Tibodeau et al, 2009) indicates that chaetocin in fact serves to inhibit and disable thioredoxin reductase, a critical enzyme in the remediation of cellular ROS.
Also, potentially important are the results indicating that hypoxia and associated HIF-1α upregulation do not attenuate the in vitro antineoplastic effects of chaetocin (Figure 5C). These findings point to the possibility that the anticancer effects of chaetocin may remain largely intact in the hypoxic solid tumour microenvironment, a desirable property indeed with regard to a candidate solid tumour therapeutic. Of importance also is that although another group reported that functional HIF-1α is required for the antitumour effects of chaetocin in some systems (Lee et al, 2011), this did not seem to be the case in our experiments (e.g., Figure 5C).
Results indicating that chaetocin may not only target tumour cells directly but also indirectly by its antiangiogentic effects on tumour microvasculature (Figure 6) are also noteworthy. In particular, we found chaetocin to attenuate tumour-associated vascularity in vivo and to have potential to act directly in the tumour microenvironment, as chaetocin inhibits HuVEC proliferation (Figure 6D and E). These findings intriguingly suggest that chaetocin not only has direct effects on tumour but potentially also additional effects on the tumour microenvironment, that may combine together to produce observed in vivo efficacy.
Although our studies go a long way in clarifying the effects of chaetocin on solid tumour cells in vitro, questions still remain related to its actions in the tumour microenvironment and the extent to which these extra-tumour effects may contribute to observed in vivo activity. In particular, the effects of chaetocin in the setting of tumour hypoxia require more clarification. Although our experiments failed to demonstrate any effects of chaetocin on phospho-VEGFR-1 levels in vivo (suggesting that VEGF activity in treated and untreated SKOV3 tumours was similar), the results of others indicate instead that disruption of HIF-1α signalling may nevertheless have an important role in the in vivo effects of chaetocin under at least some circumstances. In particular, Kung et al (2004) were the first to implicate thiodioxopiperazines as candidate inhibitors of HIF-1α signalling, discovering in an unbiased high-throughput screen that the structurally related thiodioxopiperazine chaetomin attenuates HIF-1α-directed transcription by disrupting HIF-1α/p300 binding interactions in vivo in a HepG2 xenograft model. While the studies reported herein were ongoing, Lee et al (2011) have additionally implicated intact HIF-1α signalling as critical to the effects of chaetocin itself in at least some circumstances, demonstrating that chaetocin inhibits tumour growth in vivo in a HIF-1α(+/+) fibrosarcoma xenograft model that is abrogated in a corresponding HIF-1α(−/−) model, hence implicating chaetocin-altered splicing of HIF-1α pre-mRNA as contributory to in vivo effects in this model system (Iwasa et al, 2010).
Seemingly in contrast, our results instead demonstrate that chaetocin is cytotoxic in many tumour cell lines under normoxic in vitro conditions where HIF-1α is not upregulated or detectable (e.g., Figures 2A and 5C), clearly indicating that HIF-1α is not required for its in vitro cytotoxicity. We have established instead that, at least in vitro, chaetocin-induced cytotoxicity is dependant upon the ability of chaetocin to potently induce ROS (e.g., Figure 2), apparently via competitive inhibition of thioredoxin reductase (Tibodeau et al, 2009). Other contributors to in vivo effects undoubtedly also exist. In particular, the inhibition of HuVEC proliferation by chaetocin (Figure 6D and E) suggests that chaetocin may additionally act directly on endothelial cells in the tumour microenvironment. Furthermore, chaetocin also inhibits histone methyltransferase SU(VAR)3–9 (Greiner et al, 2005). It seems therefore likely that the multiple effects of chaetocin may combine to contribute to its in vivo activity, perhaps varying dependant upon tumour and tumour microenvironment contexts and accounting for apparently disparate observations in different model systems.
Collectively, chaetocin appears to represent an interesting and promising compound for further preclinical and clinical development in both myeloma and solid tumours. Its ability to kill cancer cells even in the presence of (i) inhibitors of apoptosis or autophagy, (ii) metabolically inactive mitochondria, or (iii) hypoxia are particularly intriguing, as is its potential to target not only just tumour cells but potentially also the tumour microenvironment by attenuation of endothelial cell proliferation.
This work is published under the standard license to publish agreement. After 12 months the work will become freely available and the license terms will switch to a Creative Commons Attribution-NonCommercial-Share Alike 3.0 Unported License.
We wish to thank Candace Kostelec for editorial assistance and Bruce Morlan for statistical assistance, the Electron Microscopy, Flow Cytometry, and Advanced Genomic Technology Center Microarray Shared Resource Core Laboratories of Mayo Clinic for technical help, the laboratory of Dr Debabrata (Dev) Mukhopadhyay for assistance with hypoxia studies, and the National Cancer Institute for kindly assessing chaetocin using the NCI-60 screen. The presented work was funded in part by CA125750.
The authors declare no conflict of interest.
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Keywords: thioredoxin, reactive oxygen species, apoptosis, hypoxia, angiogenesis.
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