- Research article
- Open Access
- Open Peer Review
Decrease of Nibrin expression in chronic hypoxia is associated with hypoxia-induced chemoresistance in some brain tumour cells
BMC Cancer volume 19, Article number: 300 (2019)
Solid tumours are less oxygenated than normal tissues. This is called tumour hypoxia and leads to resistance to radiotherapy and chemotherapy. The molecular mechanisms underlying such resistance have been investigated in a range of tumour types, including the adult brain tumours glioblastoma, yet little is known for paediatric brain tumours. Medulloblastoma (MB) is the most common malignant brain tumour in children. We aimed to elucidate the impact of hypoxia on the sensitivity of MB cells to chemo- and radiotherapy.
We used two MB cell line (D283-MED and MEB-Med8A) and a widely used glioblastoma cell line (U87MG) for comparison. We applied a range of molecular and cellular techniques to measure cell survival, cell cycle progression, protein expression and DNA damage combined with a transcriptomic micro-array approach in D283-MED cells, for global gene expression analysis in acute and chronic hypoxic conditions.
In D283-MED and U87MG, chronic hypoxia (5 days), but not acute hypoxia (24 h) induced resistance to chemotherapy and X-ray irradiation. This acquired resistance upon chronic hypoxia was present but less pronounced in MEB-Med8A cells. Using transcriptomic analysis in D283-MED cells, we found a large transcriptional remodelling upon long term hypoxia, in particular the expression of a number of genes involved in detection and repair of double strand breaks (DSB) was altered. The levels of Nibrin (NBN) and MRE11, members of the MRN complex (MRE11/Rad50/NBN) responsible for DSB recognition, were significantly down-regulated. This was associated with a reduction of Ataxia Telangiectasia Mutated (ATM) activation by etoposide, indicating a profound dampening of the DNA damage signalling in hypoxic conditions. As a consequence, p53 activation by etoposide was reduced, and cell survival enhanced. Whilst U87MG shared the same dampened p53 activity, upon chemotherapeutic drug treatment in chronic hypoxic conditions, these cells used a different mechanism, independent of the DNA damage pathway.
Together our results demonstrate a new mechanism explaining hypoxia-induced resistance involving the alteration of the response to DSB in D283-MED cells, but also highlight the cell type to cell type diversity and the necessity to take into account the differing tumour genetic make-up when considering re-sensitisation therapeutic protocols.
Medulloblastoma (MB) is a malignant embryonal brain tumour originating from neural stem cells or granule-cell progenitors of the cerebellum, due to a deregulation of signalling pathways involved in neuronal development such as Wnt or Sonic Hedgehog (SHH) . It is one of the most common brain tumours in children accounting for 15–20% of all paediatric CNS tumours. MB is a heterogeneous cancer with distinct genetic variants, classified into 4 principal subgroups; Wnt, SSH, Group 3 and Group 4, based on their transcriptome [2, 3] reviewed in . More recent classification using genome wide DNA methylation and gene expression data resulted in the division of these 4 groups into 12 sub-groups . Treatment of MB generally involves surgery followed by a combination of radiotherapy and cytotoxic chemotherapy. In very young children, surgery is followed by chemotherapy alone due to the severe effects of radiation therapy on the developing brain . Recent studies have explored the use of proton beam therapy for MB, which triggers fewer detrimental side effects, as a result of reduction in irradiation of healthy brain tissue .
Despite a marked improvement in the 5-year survival rate for MB patients, 40% succumb to the disease, demonstrating the limitations of the current therapies. Group 3 MB have the worst overall survival (~ 50%) even after extensive treatment [2, 8, 9]. One reason for treatment failure is the resistance to chemo- or radiotherapeutic interventions. In both MB patients and MB cell lines such resistance has been observed and attributed to mutations in specific signalling pathways in the case of targeted therapies , or to mutations in the p53 signalling pathway [11,12,13,14,15]. For example, in the SHH group p53 mutations correlate with poor treatment outcome . In addition to the intrinsic mutations in cancer cells conferring resistance, extrinsic factors such as tumour hypoxia have been implicated in chemo- and radioresistance in a range of tumour types [17,18,19,20].
Tumour hypoxia is generated by irregular and tortuous vasculature formed within solid tumours, hence causing a poor delivery of oxygen and nutrients to cells. Hypoxia is associated with malignancy and tumour aggressiveness, by increasing tumour cell proliferation, metastasis and treatment resistance [21,22,23]. Hypoxic markers are, therefore, commonly associated with poor prognosis in many tumour types including breast cancer, glioblastoma and neuroblastoma [24,25,26]. Interestingly, carbonic anhydrase IX (CaIX), a robust marker of hypoxic tumours , is expressed in 23% of all MBs and is associated with poor prognosis , suggesting that tumour hypoxia impacts on MB progression and/or management. The critical impact of tumour hypoxia on drug resistance and malignancy has been reported for a large number of cancers. However, very little is known about the effect of hypoxia on MB beyond, for example, a recent study showing that the hypoxia inducible factor (HIF-1) can influence the ability of MB cells to proliferate .
Here we demonstrate that chronic hypoxia (> 4 days) triggers resistance in a common MB cell line, D283-MED, to cell death induced by etoposide or X-ray irradiation. The effect of chronic hypoxia on chemo- and radio-sensitivity was comparable to that observed in a classic glioblastoma cell line (U87MG). To understand the mechanisms underlying the observed resistance in the D283-MED MB cells, we assessed changes in global gene expression driven by a long-term hypoxic exposure using a transcriptomic approach. We identified that the DNA double strand break (DSB) sensing machinery MRE11/RAD50/NBN, known as the MRN complex, was largely repressed. The MRN complex is recruited to sites of double-strand breaks as part of the Homologous Recombination Repair (HRR) and Non-Homologous End Joining (NHEJ) pathways. We further explored the consequences of such downregulation on the subsequent activation of the DNA damage response and apoptotic signalling pathways. Upon chronic hypoxia, we observed a reduced activation by etoposide of Ataxia Telangiectasia Mutated (ATM), a serine/threonine kinase recruited to double strand breaks. This was associated with reduced p53 stabilisation and transcriptional activity. Overall, this study demonstrates that the dampening of the DNA damage response to DSB triggered by chronic hypoxia strongly contributes to treatment resistance in hypoxic conditions in MB cells.
Etoposide (E1383) was from Sigma. Tissue cell culture mediums were supplied by Gibco Life Technologies and foetal calf serum from Harlan Seralab (UK). Cyclophilin A (Ab3563), anti-mouse (Ab6808), MRE11 (ab214), ATM (ab3240), ATM serine 1981 (ab81292) and Vinculin (ab129002) antibodies were from Abcam. p53 BC-12 (sc-126) and NBN (sc-8589) antibodies were from Santa Cruz. p53 serine 15 (PC386) antibody was from CalBiochem. Anti-rabbit (7074) antibody was from Cell Signalling. Cy3-anti mouse antibody was from sigma (C2181).
D283-MED and U87MG were purchased from ATCC. MEB-Med8A cells were kindly provided by Prof T. Pietsch (University of Bonn, Germany). D283-MED were maintained in modified Eagle’s medium (MEM) with 10% FCS, 1% non-essential amino acid and 1% sodium pyruvate. MEB-Med8A cells were maintained in Dulbecco’s MEM (DMEM) with 10% FCS. U87MG cells were maintained MEM with 10% FCS and 1% sodium pyruvate. Cells were typically cultured and maintained at 37 °C and 5% CO2 in a humidified incubator. For hypoxic conditions (1% O2) cells were manipulated and incubated in a hypoxic workstation (Don Whitley Scientific, UK). All cells were regularly tested for mycoplasma infection.
Quantitative real time PCR (qPCR)
RNA was extracted with RNeasy Mini kit (Qiagen, Germany). 1 μg of RNA were used for cDNA synthesis using SuperScript® VILO kit according to the manufacturer’s protocol (Invitrogen). Quantitative qPCR was performed as described in . Primers sequences were as follows: Cyclophilin A: Forward: GCTTTGGGTCCAGGAATGG; Reverse: GTTGTCCACAGTCAGCAATGGT; MDM2: Forward: GCAAATGTGCAATACCAACA; Reverse: CTTTGGTCTAACCAGGGTCTC; PUMA: CCTGGAGGGTCCTGTACAAT; Reverse: CACCTAATTGGGCTCATCT; p21: GACTCTCAGGGTCGAAAACG; Reverse: TAGGGCTTCCTCTTCCAGAA; NBN AGAATTGGCTTTTCCCGAACT; Reverse: CAAGAAGAGCATGCAACCA. MRE11 Forward: TCAGTCAAGCTCCTCTGGGA; Reverse: AGTCCAGCAGTGGGAATTTCT; RAD50: TGCTTGTTGAACAGGGTCGT; Reverse: TCACTGAATGGTCCACGCTC. Fold change was calculated based on the threshold of amplification cycle for each reaction using the 2-CT method , where target genes were normalised to cyclophilin A and the control.
D283-MED cells were cultured in 10 cm dishes. Reverse transcriptome amplification of extracted RNA was conducted using Transplex® Whole Transcriptome Amplification kit (Sigma) from 3 different replicate per time point. NimbleGen 12x135k format array slide was utilised for the microarray experiment, whereby each transcript was represented by 3 probes. Statistical analysis of data was conducted using Matlab (script written by Damon Daniels, University of Manchester), with clustering based on k-means. All microarray raw and normalised data are available on NCBI: http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE106959).
Kaplan Meier plots
The R2: Genomics Analysis and Visualization platform (http://r2.amc.nl) was used to interrogate the Cavalli medulloblastoma dataset. Overall patient survival with high and low expression of the hypoxic genes VEGF, GLUT1 and CA9 was explored using the R2 platform and Kaplan Meier plots were generated.
For irradiation treatment, cells were treated in 35 mm dishes with 30–80 Gy x-ray irradiation in a CellRad Faxitron (130–150 kV, 5 mA), before seeding into a 96 well culture plates. Etoposide treatment was conducted directly in pre-seeded 96 well plates, with treatment of 20 μM–100 μM etoposide. Cisplatin was also added directly to cells plated in 96 well plates at concentrations ranging from 1 to 5 μg/μl, doses which are comparable to plasma levels obtained 1 h after IV injection in clinic . CellTiter 96®Aqueous One Solution (Promega) was added to wells and incubated for 2–4 h at 37 °C at the end of each treatment time point. Measurements were obtained with a plate reader at 492 nm (Multiskan, Thermo Scientific).
D283-MED cells were cultured on 6 well plates, 24 h prior drug treatments. The cells were treated with etoposide (20 μM) or left untreated (control). At the end each time point, cells were prepared according manufacturer protocols for FACS analysis. Samples were ran using a ViaCount analysis on a GUAVA flow cytometry (Guava EasyCyte Plus). Percentages of viable cells were measured using the Guava ViaCount software.
Cell cycle analysis
D283-MED cells were cultured on 6 well plates in either normoxia or hypoxia, with or without etoposide treatment. The preconditioned cells were centrifuged and resuspended in HBSS (200 μl) and stained with 25 μl of propidium iodide [10 μg/ml]. FACS analysis was performed using GUAVA flowcytometry (Guava EasyCyte Plus). Percentage of cells in each cell cycle phase was calculated using Guaava Express Pro software.
D283-MED were plated on polyornithine [100 μg/ml] pre-treated coverslips 16 h prior to treatment. Cells were fixed with paraformaldehyde (4%), and washed in PBS. PBS containing 1% BSA and 0.1% Triton-X was used for blocking and permeabilisation of cells, followed by primary antibody incubation with γH2AX for 16 h, and secondary antibody incubation for 30 min. Cells were then stained with DAPI (Hoechst, 1 μl/ml in PBS) for 5 min. Coverslips were mounted onto glass slides using Dako mounting medium. Images were obtained using Leica DM2500 microscope (Leica) and quantified using AQM Advance 6 software (Kinetic Imaging Ltd., UK).
Conducted as described in . In brief, 20–40 μg of protein was resolved on a 10% SDS-PAGE gel and transferred to nitrocelloulose membrane (0.2 μM) before incubation in primary and secondary antibody. Amersham ECL Prime Western Blotting Detection Reagent (GE Healthcare) was used for development of signal, and a G:BOX gel imaging system (Syngene, UK) used for detection. Western blot quantification was conducted with ImageJ 1.45 s open source software (National Institutes of Health, USA).
D283-MED cells were cultured in a 12 well plate directly before drug treatments. Cells were collected by centrifugation and re-suspended in 1 ml ice-cold PBS. The samples were diluted with pre-warmed agarose and loaded on the slide provided by the OxiSelectTM comet assay kit. Subsequently, the Comet assay procedures were performed as per manufacturer’s protocol, followed by alkaline electrophoresis. Vista dye was added immediately after electrophoresis for DNA staining. Slides were then imaged using Leica DM2500 microscope. Images were analysed and quantified using the ImageJ 1.45 s open source software (National Institutes of Health, USA).
Statistical significance t-test was performed using OriginPro 8.6.0 (OriginLab Corporation, USA) for mean comparisons.
Long term hypoxia induces etoposide and X-ray irradiation resistance in MB and glioblastoma cells
Tumour hypoxia is usually associated with poor patient survival. In medulloblastoma, tumours with increased expression of VEGF, GLUT1 or CA9, markers indicative of tumour hypoxia, result in reduced overall patient survival (Fig. 1). Such reduced survival rate for hypoxic tumours can be attributed, in part, to hypoxia-induced chemo- and radioresistance. Indeed, hypoxia has previously been associated with increased drug resistance in a number of tumours including glioblastoma, hepatocellular carcinoma and breast tumours [18, 33, 34]. Medulloblastoma exhibit poor response to chemo- and radiotherapeutic interventions [35, 36], yet the possibility that this could be explained by tumour hypoxia is unexplored. We used two MB cell lines: D283-MED (representative of Group3/4) [37, 38], and MEB-Med8A (representative of Group 3) [39, 40], to assess the effects of hypoxia pre-conditioning on cell sensitivity to chemotherapeutic treatment and X-ray irradiation. The results were compared with the classic glioblastoma cell line U87MG. Glioblastomas have been extensively described to be hypoxic, with oxygen concentration measured around 1% O2 or below [41, 42], with a strong correlation between regional hypoxia and poor patient survival . Here we used 1% O2 for hypoxic conditions as this level can induce a hypoxic response (increased levels of HIF-1α) without affecting cell proliferation or survival in a range of brain tumour cell lines .
The D283-MED and MEB-Med8A cell lines display differential sensitivity to etoposide and cisplatin [14, 44], hence a range of doses have been used for both drugs. The cells were exposed to 1% O2 for 1 day (acute hypoxia) or for 5 days (chronic hypoxia) prior to drug treatment. The cells subsequently remained under hypoxic conditions during treatment. Control samples were cultured and treated at atmospheric O2 levels (normoxia, 21% O2). For D283-MED cells, MTS survival assays showed that 5 days of hypoxic preconditioning triggered significant resistance to etoposide, with a cell viability of ~ 74% in hypoxic cells treated with etoposide compared to ~ 14% in normoxic conditions (Fig. 2a). In contrast, 1 day of hypoxic preconditioning did not induce any significant resistance, suggesting that the duration of hypoxic exposure is critical to alter the cell response to drugs. The hypoxia-induced resistance to etoposide was also observed in MEB-Med8A cells, although to a lesser extent and with high variability thereby without reaching statistical significance (Fig. 2b; p = 0.57). The U87MG glioblastoma cells displayed similar results to the D283-MED cell line (Fig. 2c), with 5 day preconditioning resulting in significantly higher cell viability compared to the normoxic controls. Results for the D283-MED cell line were reproduced with the cell viability assay ViaCount™, to ensure that the MTS results were not biased by altered mitochondrial activity in hypoxia, and similar data were obtained (Additional file 1: Figure S1A). Additionally, we investigated the effects of hypoxia on cell death induced by cisplatin, an interstrand crosslinking agent triggering double strand breaks. In all three cell lines, we observed resistance to cisplatin in hypoxia (Fig. 2d-f), with statistical significance in the MEB-Med8A and U87MG cells ((p < 0.05); Fig. 2d-f). Acquired resistance was also investigated upon X-ray irradiation. In this case, the cells were pre-incubated in 1% or 21% O2 for 5 days and the cells were irradiated in normoxic conditions to prevent loss of the oxygen enhancement effect during irradiation treatment . With this protocol we ensured that only the effects of hypoxia preconditioning were assessed. Similarly to etoposide treatment, yet to a lesser extent, resistance to X-ray irradiation upon hypoxic preconditioning was observed for the D283-MED and the U87MG cell lines (Fig. 2g). The MEB-Med8A cells showed an inverse trend (Fig. 2g). This counterintuitive result may be due to the fact that this cell line appeared stressed by the cooling procedure prior to irradiation, hence generating variable results.
We further assessed the ability of etoposide to induce cell cycle arrest in D283-MED cells preconditioned or not in 1% O2. Hypoxia preconditioning on its own did not induce any cell cycle alteration (Additional files 1 Figure S1B and C). This important control indicates that the reduced effect of etoposide in hypoxic preconditioned cells is not due to changes in cell proliferation agreeing with previous observations in glioblastoma . Etoposide induced a clear G2/M arrest in normoxic cells (63% of cells in G2/M when treated with etoposide, compared to 30% for untreated cells). This arrest was largely diminished in hypoxic cells with only 40% in G2/M upon etoposide treatment (Additional files 1: Figure S1B), in line with the effects of hypoxia on etoposide-induced cell death. Taken together, chronic hypoxia exposure results in resistance to the chemotherapeutic agent etoposide induced cell death and cell cycle arrest, and it also affects the sensitivity to cisplatin and X-ray irradiation. This resistance is not due to alteration of the cell cycle by hypoxia (Additional file 1: Figure S1) or to the absence of oxygen during the irradiation process, as irradiation was performed in atmospheric conditions. It, therefore, points to global changes in cell signalling, resulting in lack of sensitivity to the DNA damaging protocols used.
Chronic hypoxic exposure induces large transcriptional remodelling
To investigate the molecular mechanisms driving the observed hypoxia-induced cell death resistance in D283-MED, we used micro-array gene expression analysis to assess the global transcriptomic modifications triggered by long-term hypoxia. Hypoxia-inducible factors (HIF) are the main transcription factor family directly regulating gene expression in hypoxia. HIF-1 alpha (HIF-1α) is the primary isoform governing the expression of genes whose levels are directly dependent on oxygen availability. The levels of HIF-1α can oscillate over-time due to the prolyl-hydroxylase negative feedback loop [46, 47]. Hence, hypoxia-induced gene expression was measured at a time point that correlates with the first peak in HIF-1α stabilisation, and at two later time points subsequent to additional peaks of HIF accumulation (Fig. 3a). Considering all three time points together, we found that 6124 transcripts were significantly up- or down-regulated in hypoxia (Fig. 3b). This corresponds to 4303 significantly regulated genes (and 23,611 non-regulated genes). Significantly regulated transcripts were further analysed globally by clustergram (Fig. 3c), which showed a large number of genes regulated at late time points (64 h and 96 h), but less in acute conditions (6 h) (Fig. 3d, e). The genes regulated at the short 6 h time-point were associated with the hypoxic response (Additional file 2: Figure S2A). Conversely, at late time-points, we found genes involved in apoptosis and the cell cycle (Additional file 2: Figure S2B, C). Most transcriptional analyses upon hypoxic exposure have previously been performed after 24–48 h of hypoxia, corresponding to more acute conditions. Given the high number of transcripts regulated only at 64 h and 96 h, it is likely that many regulatory mechanisms in cellular adaptation to long term hypoxia have been missed thus far.
We initially performed a biased analysis and specifically examined the expression of several multi-drug resistance genes. These genes were the obvious candidates potentially responsible for hypoxia-induced treatment resistance and had previously been described to have a role in hypoxia-induced drug resistance in other cellular models including glioblastoma . However, none of the well described multi-drug resistance (MDR) genes, abcb1 (mdr1), abcc1 (mrp1) and abcg1, were up-regulated in hypoxia (Fig. 4a).
For a non-biased analysis using the k-means clustering method, the large number of regulated transcripts were further grouped into 16 smaller clusters based on their expression profile pattern, to find potential correlation between groups of genes with similar expression dynamics (Additional file 3: Figure S3A). From this we identified that genes involved in the response to double strand breaks were strongly regulated at later hypoxic time points. The effectiveness of DNA damage response mechanisms can play a key role in response to chemo- and radiotherapy. Therefore, we generated heat map clustergrams of the HRR and NHEJ pathways, which are primarily responsible for the repair of DSB, the most lethal form of DNA damage (Fig. 4b and c). Strong regulation was observed for a number of genes involved in both NHEJ (Fig. 4b) and HRR (Fig. 4c). We further focused on HRR pathways as key genes involved in signal transduction for HRR were down-regulated strongly by hypoxia. Down-regulated transcripts include brca2 and two members of the MRN complex, mre11A (MRE11) and Nibrin (NBN). NBN plays a key role in ATM activation and signal amplification of the DNA damage response . Therefore, the hypoxia mediated down-regulation of key components of the HRR pathway could be responsible of the altered cellular response to etoposide.
DNA damage recognition and signal transduction is dampened in chronic hypoxia
Sensing of DNA damage is a crucial step in the initiation of double strand break (DSB) repair by the HRR machinery, and its alterations is likely to impact further downstream signalling of the repair pathway. The strong reduction in NBN transcription (70% decrease) (Fig. 5a) observed in the micro-array was confirmed using qPCR, which equally showed a decrease of NBN mRNA by 70% at 96 h (Fig. 5b). Similarly, NBN protein levels were reduced by ~ 50% after 96 h of hypoxic exposure (Fig. 5c). To further understand the effect of chronic hypoxia on each member of the MRN complex, mRNA levels of NBN, MRE11 and RAD50 were determined by qPCR upon 5 days of hypoxic incubation. Hypoxia had little effect on RAD50 mRNA levels, yet there was significant down-regulation of MRE11 (~ 53%) comparable to NBN (Fig. 5d), which was further confirmed at the protein level (Fig. 5e). Surprisingly, such decreases in NBN and MRE11 expression was not observed in the U87MG cells (Additional file 4: Figure S4A).
NBN is responsible for the recruitment and activation of ATM, which then gets activated through auto-phosphorylation at the DNA breakage site [50, 51]. Active ATM phosphorylates downstream targets including the histone variant H2AX and Chk2, ultimately resulting in repair of the break or activation of pro-apoptotic pathways via p53 stabilisation (reviewed by ). To understand whether the hypoxia-induced down-regulation of NBN and MRE11 influences ATM activation, we assessed the level of ATM and ATM serine 1981 in hypoxic and normoxic D283-MED cells. Etoposide has the ability to induce replication associated DSB thus triggering ATM activation, measured by an increase in ATM serine 1981 (Fig. 6). For cells pre-incubated in 1% O2 for 5 days we observed a ~ 70% reduction in ATM levels compared to the normoxic control. Upon etoposide treatment ATM serine 1981 was ~ 85% lower in hypoxic cells. This effect of hypoxia on ATM levels was even stronger when cells were exposed to more severe hypoxic conditions (0.1% O2) (Fig. 6). In contrast, in MEB-Med8A and U87MG, hypoxia had little effect on both ATM and phospho-ATM serine 1981 levels (Additional file 4: Figure S4 B and Additional file 5: Figure S5), in line with the previous observation of NBN/MRE11 levels being unaffected by hypoxia in the U87MG cells.
To ensure that the reduced ATM activation was not a result of decreased etoposide efficacy in hypoxia, we measured the levels of phosphorylated γH2AX, a marker of double strand breaks. In control non-treated cells, there was little γH2AX staining in normoxic and hypoxic cells (Fig. 7a), indicating that, as expected, 1% O2 is not sufficient to create DSBs in cells. After 15 min of etoposide treatment a similar level of γH2AX levels were observed in normoxia and hypoxia (3.7-fold and 2.9-fold increase, respectively; non-significant difference), demonstrating that the efficacy of etoposide in generating DSBs is not affected by the hypoxic conditions alone. This was further confirmed using an alkaline comet assay, which showed that hypoxia had no direct effect on the ability of etoposide to induce DNA strand breaks. Indeed, etoposide induced a clear comet tail in D283-MED cells, and no difference of olive tail moments could be observed between the normoxic and hypoxic cells at any time point (Fig. 7b). Together, these experiments demonstrate that etoposide remains fully functional in a low oxygen environment (1% O2). These data suggest that as a result of decreased NBN and MRE11 expression in hypoxic conditions there is a clear dampening of further down-stream signalling in the HRR pathway in D283-MED cells.
p53 activation is reduced in chronic hypoxia
An obvious candidate involved in both cell cycle arrest and apoptosis is p53, a central transcription factor critical for the effectiveness of DNA damaging agents. We have previously shown, the essential role of p53 in etoposide-induced cell death in MB cells [13, 53]. ATM is directly responsible for p53 stabilisation through phosphorylation . Initially we assessed p53 transcriptional activity in D283-MED by measuring the mRNA levels of three well described p53 target genes: mdm2 (murine double minute 2), puma (p53 upregulated modulator of apoptosis) and p21. Hypoxia (5 days at 1% O2) did not alter the p53 basal activity, as shown by the similar levels of expression of the target mRNA in all conditions (Fig. 8a). As expected, etoposide treatment strongly induced the transcription of mdm2, puma and p21 (~ 32-, ~ 5- and ~ 26-fold, respectively; Fig. 8b). However, in cells preconditioned in hypoxia, no increase in puma mRNA could be detected and only ~ 3- and ~ 2.5-fold increases of mdm2 and p21 were observed, which is approximatively 10 times lower than in normoxic cells (Fig. 8b). The impairment of etoposide-induced p53 transcriptional activity in hypoxic cells was further confirmed by lower levels of p53 phosphorylation on serine 15 (Fig. 8c, d), a marker of p53 activation . Again, basal p53 and p53 serine 15 protein levels were similar in both normoxic and hypoxic cells, yet in hypoxic cells, etoposide failed to fully induce p53 stabilisation with three times lower levels of phosphorylation observed when normalised to the total amount of p53 (Fig. 8d). Similar results were obtained for the U87MG glioblastoma cell line (Additional file 6: Figure S6A, B), suggesting that, whilst recruiting different mechanisms of resistance, there is a convergence on the activation of p53 protein.
Tumour hypoxia has been extensively correlated with acquired resistance to cytotoxic drugs and irradiation, yet the underlying mechanisms are variable between tumour types. The impact of oxygen deprivation during treatment as opposed to the cellular experience prior to treatment has not been untangled so far. Whilst the oxygen enhancement effect, whereby oxygen directly reacts with broken end of DNA preventing their repair, has been implicated in reduced effectiveness of radiotherapy in hypoxia [45, 55], we here demonstrate that the cellular oxygenation history has a broad impact on cell adaptation and sensitivity to DNA damaging agents. To observe resistance to drug and irradiation a chronic hypoxic preconditioning of several days is necessary, in both medulloblastoma and glioblastoma cells. Although, the prolonged hypoxia exposure triggers different adaptive mechanisms between cell lines, they ultimately converge on the inability to activate the pro-apoptotic p53 protein, thereby mediating cell death and cell-cycle arrest resistance.
Timing and severity of hypoxic exposure impacts how DNA repair mechanisms are altered
Low oxygen environments such as those experienced within tumours have previously been reported to influence the response to DNA damage and its repair (reviewed in [56, 57]). Hypoxia alone has been reported to activate ATM, yH2AX and p53 [58,59,60], however, this was not the case in our hypoxic conditions (1% O2), which were much milder than those used in these previous studies (0–0.2% O2). Additionally, severe hypoxia has been reported to reduce HRR capacity by the down-regulation of key repair proteins such as RAD51 and BRCA1 [61,62,63]. Work by To et al. identified that moderate hypoxia (1% O2) resulted in transcriptional downregulation of NBN through HIF-1α binding to the NBN promoter thereby displacing Myc , supporting our own findings (Fig. 5). Such impact of chronic hypoxia on HRR was reported to result in increased sensitivity to DNA damaging substances such as crosslinking agents (Cisplatin, Mytomycin C) and irradiation [63, 65]. Our data suggest that hypoxia-induced downregulation of the MRN complex, in D283-MED cells, results in resistance to DSB inducing agents by impairing signalling events downstream of the MRN recruitment hence resulting in reduced p53 activity and apoptosis.
This observed requirement of functional Nibrin and MRN complex for triggering cell death is supported by clinical studies, which demonstrated that expression of Nibrin or an intact MRE11 complex was essential for good treatment outcome [66,67,68]. Moreover, Cerosaletti et al. have demonstrated the active role of NBN in ATM activation, beyond its role in recruiting MRE11/Rad50 . This mechanism fully support our observations, where decrease of nibrin expression is associated with a lack of ATM activation and subsequent absence of p53 stabilisation and activity.
The differing O2 levels experienced by cells, are varied in terms of localisation within the solid tumour and duration of the hypoxic episodes , including cycling hypoxia . In vitro experiments, trying to recreate such variety of hypoxic severity and duration have led to conflicting results rendering studies hard to compare . We identified that hypoxia-induced resistance to etoposide required chronic (5 day), rather than acute (24 h), hypoxia. Previous studies investigating hypoxia and drug resistance primarily utilised acute (6–48 h) time points. For example, resistance to cisplatin and doxorubicin induced by hypoxia in non-small cell lung cancer was due to incubation in 0.5% O2 for only 16 h . Our work highlights the necessity to explore both chronic and acute exposure times to ensure adequate observation of any potential hypoxia induced resistance in cancer models. When considering the impact of hypoxia duration on DNA repair mechanisms, short exposures (minutes to hours) are thought to regulate repair proteins through post-translational modifications and changes to translation efficiency, whereas longer exposure (days-weeks) results in alteration to transcription, as well as epigenetic modifications . The reported activation of numerous DNA repair proteins by hypoxia, such as ATM and p53, as well as the reduced capacity of HRR was primarily observed after acute and severe hypoxic exposure (16–72 h) [58, 59, 61,62,63, 65]. Our gene expression analysis identified a significant proportion of genes involved in DNA DSB repair that were only regulated at later hypoxic time points (64–96 h). This highlights the need to extend hypoxia incubation periods for DNA repair related studies. Thus far the impact of more chronic moderate hypoxia on DNA repair mechanisms and the biological and clinical implications may have been missed.
Heterogeneity of the cellular response to hypoxia between cell types
We observed a strong hypoxia-induced chemo- and radio-resistance in the D283-MED cell line (Fig. 2), however the MEB-Med8A cells did not show the same extent of resistance. This differing response might be due to the differences in the molecular signature of these two cell lines. MEB-Med8A is a Group 3 medulloblastoma cell line, with strong associations with classical Group 3 characteristics, such as myc amplification and pvt1-myc fusion [39, 40], whereas the grouping affiliation of D283-MED is more controversial, with a lack of myc amplification pointing towards Group 4 [37, 38]. It was previously demonstrated that the p53 and NF-kappaB function is key in MB cells for an effective response to DNA damaging agents [13, 14]. For example, MEB-Med8A has a truncated form of p53, which directly impacts on the sensitivity to chemotherapeutic drugs [13, 14]. Such distinct genetic backgrounds are likely to also explain their differing response to hypoxia, reinforcing the view that the genetic make-up of a tumour is a key factor to consider when selecting therapeutic regimens. In addition to the resistance observed in D283-MED cells, similar effects of hypoxic preconditioning were observed in U87MG cells, a classic glioblastoma cell line, in agreement with previous reports [8, 73]. However, in the U87MG cells, hypoxia did not influence the level of the MRN complex or ATM activation (Additional file 4: Figure S4) as it did in the D283-MED cells, demonstrating again the heterogeneity in the cellular response to hypoxia, beyond HIF activation. Additionally, we did not observe other reported mechanisms of hypoxia-induced resistance such as the induction of MDR genes  in the D283-MED cells.
The complex and varied response to hypoxia is also apparent when comparing in vitro cell line models to in vivo organisms and pre-clinical models. In this case, our results obtained in vitro mimicked the observations made in hypoxic tumours in vivo, in terms of resistance to cancer treatments. Moreover, hypoxia related changes to DNA repair proteins have been translated to an in vivo setting. For example, active phospho-ATM is co-localised with the hypoxic marker CAIX in tumour xenografts  and RAD51 down-regulation was observed in cervical and prostate cancer xenografts  as well as in a glioma model .
In conclusion, we have shown that the chemo- and radio-resistance triggered by a chronic hypoxic exposure can be explained by a broad gene expression remodelling of components of the DNA DSB sensing machinery, subsequently affecting the activation of DNA repair and pro-apoptotic mechanisms. This suggests that reactivation of the signalling pathway could re-sensitise cells to treatment. However, the way cells adapt to the low oxygen levels is diverse with individual cell line or cell-type specific responses. In this study for example, whilst the U87MG cells exposed to chronic hypoxia, showed a similar resistance to treatment and a similar dampened p53 activation to the D283-MED cells, the mechanism of alteration of the DNA DSB sensing and repair pathways were different. Such diversity in the cellular adaptation, makes it difficult to define global clinical strategies for hypoxic cell sensitisation. From a clinical perspective, the development of HIF inhibitors targeting either HIF mRNA transcription, translation, or HIF stabilisation  might help tackling the treatment resistance problem by re-sensitising hypoxic tumours. In the U251 glioblastoma cells, campothecins (CPTs) analogues can inhibit the accumulation of HIF1α protein . However, individual tumours react differently to hypoxic episodes, as highlighted by our own data, which exemplifies the need to understand how hypoxia impacts tumour cell biology on an individual tumour basis leading to a more personalised clinical approach.
Ataxia Telangiectasia Mutated
Carbonic anhydrase IX
Central nervous system
Double strand break
Hypoxia indcuble factor 1
Homologous recombination repair
Murine double minute 2
Modified Eagle’s medium
Non-homologous end joining
p53 upregulated modulator of apoptosis
Quantitative polymerase chain reaction
Marino S. Medulloblastoma: developmental mechanisms out of control. Trends Mol Med. 2005;11(1):17–22.
Taylor MD, Northcott PA, Korshunov A, Remke M, Cho YJ, Clifford SC, Eberhart CG, Parsons DW, Rutkowski S, Gajjar A, et al. Molecular subgroups of medulloblastoma: the current consensus. Acta Neuropathol. 2012;123(4):465–72.
Kool M, Korshunov A, Pfister SM. Update on molecular and genetic alterations in adult medulloblastoma. Memo. 2012;5(3):228–32.
Skowron P, Ramaswamy V, Taylor MD. Genetic and molecular alterations across medulloblastoma subgroups. J Mol Med (Berl). 2015;93(10):1075–84.
Cavalli FMG, Remke M, Rampasek L, Peacock J, Shih DJH, Luu B, Garzia L, Torchia J, Nor C, Morrissy AS, et al. Intertumoral heterogeneity within Medulloblastoma subgroups. Cancer Cell. 2017;31(6):737–54 e736.
Pizer B, Clifford S. Medulloblastoma: new insights into biology and treatment. Archives of Disease in Childhood-Education and Practice Edition. 2008;93(5):137–44.
Yock TI, Tarbell NJ, Yeap BY, Ebb DH, Weyman E, Eaton BR, Sherry NA, Jones RM, MacDonald SM, Pulsifer MB, et al. Proton beam therapy for medulloblastoma - Author's reply. Lancet Oncol. 2016;17(5):e174–5.
Cho YJ, Tsherniak A, Tamayo P, Santagata S, Ligon A, Greulich H, Berhoukim R, Amani V, Goumnerova L, Eberhart CG, et al. Integrative genomic analysis of Medulloblastoma identifies a molecular subgroup that drives poor clinical outcome. J Clin Oncol. 2011;29(11):1424–30.
Northcott PA, Korshunov A, Witt H, Hielscher T, Eberhart CG, Mack S, Bouffet E, Clifford SC, Hawkins CE, French P, et al. Medulloblastoma comprises four distinct molecular variants. J Clin Oncol. 2011;29(11):1408–14.
Metcalfe C, de Sauvage FJ. Hedgehog fights back: mechanisms of acquired resistance against smoothened antagonists. Cancer Res. 2011;71(15):5057–61.
Dee S, Haas-Kogan DA, Israel MA. Inactivation of p53 is associated with decreased levels of radiation-induced apoptosis in medulloblastoma cell lines. Cell Death Differ. 1995;2(4):267–75.
Tabori U, Baskin B, Shago M, Alon N, Taylor MD, Ray PN, Bouffet E, Malkin D, Hawkins C. Universal poor survival in children with medulloblastoma harboring somatic TP53 mutations. J Clin Oncol. 2010;28(8):1345–50.
Meley D, Spiller DG, White MRH, McDowell H, Pizer B, Sée V. p53-mediated delayed NF-κB activity enhances etoposide-induced cell death in medulloblastoma. Cell Death and Disease. 2010; in press(in press).
Fan YN, Meley D, Pizer B, See V. Mir-34a mimics are potential therapeutic agents for p53-mutated and chemo-resistant brain tumour cells. PLoS One. 2014;9(9):e108514.
Hill RM, Kuijper S, Lindsey JC, Petrie K, Schwalbe EC, Barker K, Boult JK, Williamson D, Ahmad Z, Hallsworth A, et al. Combined MYC and P53 defects emerge at medulloblastoma relapse and define rapidly progressive, therapeutically targetable disease. Cancer Cell. 2015;27(1):72–84.
Zhukova N, Ramaswamy V, Remke M, Pfaff E, Shih DJ, Martin DC, Castelo-Branco P, Baskin B, Ray PN, Bouffet E, et al. Subgroup-specific prognostic implications of TP53 mutation in medulloblastoma. J Clin Oncol. 2013;31(23):2927–35.
Brown JM. The hypoxic cell: a target for selective cancer therapy--eighteenth Bruce F. Cain Memorial Award lecture. Cancer Res. 1999;59(23):5863–70.
Sullivan R, Graham CH. Hypoxia prevents etoposide-induced DNA damage in cancer cells through a mechanism involving hypoxia-inducible factor 1. Mol Cancer Ther. 2009;8(6):1702–13.
Piret JP, Cosse JP, Ninane N, Raes M, Michiels C. Hypoxia protects HepG2 cells against etoposide-induced apoptosis via a HIF-1-independent pathway. Exp Cell Res. 2006;312(15):2908–20.
Hussein D, Estlin EJ, Dive C, Makin GW. Chronic hypoxia promotes hypoxia-inducible factor-1alpha-dependent resistance to etoposide and vincristine in neuroblastoma cells. Mol Cancer Ther. 2006;5(9):2241–50.
Harris AL. Hypoxia--a key regulatory factor in tumour growth. Nat Rev Cancer. 2002;2(1):38–47.
Herrmann A, Rice M, Levy R, Pizer BL, Losty PD, Moss D, See V. Cellular memory of hypoxia elicits neuroblastoma metastasis and enables invasion by non-aggressive neighbouring cells. Oncogenesis. 2015;4:e138.
Sermeus A, Cosse JP, Crespin M, Mainfroid V, de Longueville F, Ninane N, Raes M, Remacle J, Michiels C. Hypoxia induces protection against etoposide-induced apoptosis: molecular profiling of changes in gene expression and transcription factor activity. Mol Cancer. 2008;7.
Kaynar MY, Sanus GZ, Hnimoglu H, Kacira T, Kemerdere R, Atukeren P, Gumustas K, Canbaz B, Tanriverdi T. Expression of hypoxia inducible factor-1alpha in tumors of patients with glioblastoma multiforme and transitional meningioma. J Clin Neurosci. 2008;15(9):1036–42.
Fardin P, Barla A, Mosci S, Rosasco L, Verri A, Versteeg R, Caron HN, Molenaar JJ, Ora I, Eva A, et al. A biology-driven approach identifies the hypoxia gene signature as a predictor of the outcome of neuroblastoma patients. Mol Cancer. 2010;9:185.
Vaupel P: Tumor oxygenation: an appraisal of past and present concepts and a look into the future : Arisztid G. B Kovach Lecture Advances in experimental medicine and biology 2013, 789:229–236.
Chia SK, Wykoff CC, Watson PH, Han C, Leek RD, Pastorek J, Gatter KC, Ratcliffe P, Harris AL. Prognostic significance of a novel hypoxia-regulated marker, carbonic anhydrase IX, in invasive breast carcinoma. J Clin Oncol. 2001;19(16):3660–8.
Nordfors K, Haapasalo J, Korja M, Niemela A, Laine J, Parkkila AK, Pastorekova S, Pastorek J, Waheed A, Sly WS, et al. The tumour-associated carbonic anhydrases CA II, CA IX and CA XII in a group of medulloblastomas and supratentorial primitive neuroectodermal tumours: an association of CA IX with poor prognosis. BMC Cancer. 2010;10:148.
Cruzeiro GA, Dos Reis MB, Silveira VS, Lira RC, Carlotti CG, Neder L, Oliveira RS, Yunes JA, Brandalise SR, Aguiar S, et al. HIF1A is overexpressed in medulloblastoma and its inhibition reduces proliferation and increases EPAS1 and ATG16L1 methylation. Curr Cancer Drug Targets. 2017.
Richards R, Jenkinson MD, Haylock BJ, See V. Cell cycle progression in glioblastoma cells is unaffected by pathophysiological levels of hypoxia. Peerj. 2016;4.
Pfaffl MW, Horgan GW, Dempfle L. Relative expression software tool (REST (c)) for group-wise comparison and statistical analysis of relative expression results in real-time PCR. Nucleic Acids Res. 2002;30(9):1-10.
Rajkumar P, Mathew BS, Das S, Isaiah R, John S, Prabha R, Fleming DH. Cisplatin concentrations in Long and short duration infusion: implications for the optimal time of radiation delivery. J Clin Diagn Res. 2016;10(7):XC01–4.
Amberger-Murphy V. Hypoxia helps glioma to fight therapy. Curr Cancer Drug Targets. 2009;9(3):381–90.
Cosse JP, Sermeus A, Vannuvel K, Ninane N, Raes M, Michiels C. Differential effects of hypoxia on etoposide-induced apoptosis according to the cancer cell lines. Mol Cancer. 2007;6:61.
Finlay JL. The role of high-dose chemotherapy and stem cell rescue in the treatment of malignant brain tumors: a reappraisal. Pediatr Transplant. 1999;3(Suppl 1):87–95.
Skowronska-Gardas A, Chojnacka M, Morawska-Kaczynska M, Perek D, Perek-Polnik M. Patterns of failure in children with medulloblastoma treated with 3D conformal radiotherapy. Radiotherapy and oncology. journal of the European Society for Therapeutic Radiology and Oncology. 2007;84(1):26–33.
Bigner SH, Friedman HS, Vogelstein B, Oakes WJ, Bigner DD. Amplification of the c-myc gene in human medulloblastoma cell lines and xenografts. Cancer Res. 1990;50(8):2347–50.
Sengupta S, Weeraratne SD, Sun HY, Phallen J, Rallapalli SK, Teider N, Kosaras B, Amani V, Pierre-Francois J, Tang YJ, et al. alpha 5-GABAA receptors negatively regulate MYC-amplified medulloblastoma growth. Acta Neuropathol. 2014;127(4):593–603.
Langdon JA, Lamont JM, Scott DK, Dyer S, Prebble E, Bown N, Grundy RG, Ellison DW, Clifford SC. Combined genome-wide allelotyping and copy number analysis identify frequent genetic losses without copy number reduction in medulloblastoma. Genes Chromosomes & Cancer. 2006;45(1):47–60.
Northcott PA, Shih DJH, Peacock J, Garzia L, Morrissy AS, Zichner T, Stutz AM, Korshunov A, Reimand J, Schumacher SE, et al. Subgroup-specific structural variation across 1,000 medulloblastoma genomes. Nature. 2012;488(7409):49–56.
Whittle IR, Stavrinos N, Akil H, Yau Y, Lewis SC. Assessment of physiological parameters within glioblastomas in awake patients: a prospective clinical study. Br J Neurosurg. 2010;24(4):447–53.
Collingridge DR, Piepmeier JM, Rockwell S, Knisely JPS. Polarographic measurements of oxygen tension in human glioma and surrounding peritumoural brain tissue. Radiother Oncol. 1999;53(2):127–31.
Spence AM, Muzi M, Swanson KR, O'Sullivan F, Rockhill JK, Rajendran JG, Adamsen TC, Link JM, Swanson PE, Yagle KJ, et al. Regional hypoxia in glioblastoma multiforme quantified with [18F]fluoromisonidazole positron emission tomography before radiotherapy: correlation with time to progression and survival. Clinical cancer research : an official journal of the American Association for Cancer Research. 2008;14(9):2623–30.
Nor C, Sassi FA, de Farias CB, Schwartsmann G, Abujamra AL, Lenz G, Brunetto AL, Roesler R. The histone deacetylase inhibitor sodium butyrate promotes cell death and differentiation and reduces neurosphere formation in human medulloblastoma cells. Mol Neurobiol. 2013;48(3):533–43.
Chapman JD, Reuvers AP, Borsa J, Greenstock CL. Chemical radioprotection and Radiosensitization of mammalian-cells growing in-vitro. Radiat Res. 1973;56(2):291–306.
Stiehl DP, Wirthner R, Koditz J, Spielmann P, Camenisch G, Wenger RH. Increased prolyl 4-hydroxylase domain proteins compensate for decreased oxygen levels. Evidence for an autoregulatory oxygen-sensing system. J Biol Chem. 2006;281(33):23482–91.
Bagnall J, Leedale J, Taylor S, Spiller DG, White MRH, Sharkey KJ, Bearon RN, See V. Tight control of hypoxia inducible factor (HIF)-alpha transient dynamics is essential for cell survival in hypoxia. J Biol Chem. 2013.
Chen L, Feng P, Li S, Long D, Cheng J, Lu Y, Zhou D. Effect of hypoxia-inducible factor-1alpha silencing on the sensitivity of human brain glioma cells to doxorubicin and etoposide. Neurochem Res. 2009;34(5):984–90.
Cerosaletti K, Concannon P. Independent roles for nibrin and Mre11-Rad50 in the activation and function of Atm. J Biol Chem. 2004;279(37):38813–9.
Falck J, Coates J, Jackson SP. Conserved modes of recruitment of ATM, ATR and DNA-PKcs to sites of DNA damage. Nature. 2005;434(7033):605–11.
You ZS, Chahwan C, Bailis J, Hunter T, Russell P. ATM activation and its recruitment to damaged DNA require binding to the C terminus of Nbs1. Mol Cell Biol. 2005;25(13):5363–79.
Shiloh Y, Ziv Y. The ATM protein kinase: regulating the cellular response to genotoxic stress, and more. Nat Rev Mol Cell Biol. 2013;14(4):197–210.
Sakaguchi K, Herrera JE, Saito S, Miki T, Bustin M, Vassilev A, Anderson CW, Appella E. DNA damage activates p53 through a phosphorylation-acetylation cascade. Genes Dev. 1998;12(18):2831–41.
Saito S, Goodarzi AA, Higashimoto Y, Noda Y, Lees-Miller SP, Appella E, Anderson CW. ATM mediates phosphorylation at multiple p53 sites, including Ser(46), in response to ionizing radiation. J Biol Chem. 2002;277(15):12491–4.
Deschner EE, Gray LH. Influence of oxygen tension on X-Ray-induced chromosomal damage in Ehrlich ascites tumor cells irradiated Invitro and Invivo. Radiat Res. 1959;11(1):115–46.
Bristow RG, Hill RP. Hypoxia, DNA repair and genetic instability. Nat Rev Cancer. 2008;8(3):180–92.
Scanlon SE, Glazer PM. Multifaceted control of DNA repair pathways by the hypoxic tumor microenvironment. DNA Repair (Amst). 2015;32:180–9.
Bencokova Z, Kaufmann MR, Pires IM, Lecane PS, Giaccia AJ, Hammond EM. ATM activation and signaling under hypoxic conditions. Mol Cell Biol. 2009;29(2):526–37.
Hammond EM, Dorie MJ, Giaccia AJ. ATR/ATM targets are phosphorylated by ATR in response to hypoxia and ATM in response to reoxygenation. J Biol Chem. 2003;278(14):12207–13.
Wrann S, Kaufmann MR, Wirthner R, Stiehl DP, Wenger RH. HIF mediated and DNA damage independent histone H2AX phosphorylation in chronic hypoxia. Biol Chem. 2013;394(4):519–28.
Bindra RS, Schaffer PJ, Meng A, Woo J, Maseide K, Roth ME, Lizardi P, Hedley DW, Bristow RG, Glazer PM. Down-regulation of Rad51 and decreased homologous recombination in hypoxic cancer cells. Mol Cell Biol. 2004;24(19):8504–18.
Bindra RS, Schaffer PJ, Meng A, Woo J, Maseide K, Roth ME, Lizardi P, Hedley DW, Bristow RG, Glazer PM. Alterations in DNA repair gene expression under hypoxia: elucidating the mechanisms of hypoxia-induced genetic instability. Ann N Y Acad Sci. 2005;1059:184–95.
Chan N, Koritzinsky M, Zhao H, Bindra R, Glazer PM, Powell S, Belmaaza A, Wouters B, Bristow RG. Chronic hypoxia decreases synthesis of homologous recombination proteins to offset chemoresistance and radioresistance. Cancer Res. 2008;68(2):605–14.
To Kkw, Sedelnikova OA, Samons M, Bonner WM, Huang LE. The phosphorylation status of PAS-B distinguishes HIF-1 alpha from HIF-2 alpha in NBS1 repression. Embo J. 2006;25(20):4784–94.
Kumareswaran R, Ludkovski O, Meng A, Sykes J, Pintilie M, Bristow RG. Chronic hypoxia compromises repair of DNA double-strand breaks to drive genetic instability. J Cell Sci. 2012;125(Pt 1):189–99.
Kuo KT, Chou TY, Hsu HS, Chen WL, Wang LS. Prognostic significance of NBS1 and snail expression in esophageal squamous cell carcinoma. Ann Surg Oncol. 2012;19:S549–57.
Soderlund K, Stal O, Skoog L, Rutqvist LE, Nordenskjold B, Askmalm MS. Intact Mre11/Rad50/Nbs1 complex predicts good response to radiotherapy in early breast cancer. International Journal of Radiation Oncology Biology Physics. 2007;68(1):50–8.
Gao JF, Zhang H, Arbman G, Sun XF. RAD50/MRE11/NBS1 proteins in relation to tumour development and prognosis in patients with microsatellite stable colorectal cancer. Histol Histopathol. 2008;23(12):1495–502.
Cerosaletti K, Wright J, Concannon P. Active role for nibrin in the kinetics of atm activation. Mol Cell Biol. 2006;26(5):1691–9.
Dewhirst MW, Braun RD, Lanzen JL. Temporal changes in PO2 of R3230AC tumors in Fischer-344 rats. Int J Radiat Oncol Biol Phys. 1998;42(4):723–6.
Bayer C, Vaupel P, [et al] Acute versus chronic hypoxia in tumors: controversial data concerning time frames and biological consequences. Strahlentherapie und Onkologie : Organ der Deutschen Rontgengesellschaft 2012, 188(7):616–627.
Song XR, Liu XX, Chi WL, Liu YL, Wei L, Wang XW, Yu JM. Hypoxia-induced resistance to cisplatin and doxorubicin in non-small cell lung cancer is inhibited by silencing of HIF-1 alpha gene. Cancer Chemother Pharmacol. 2006;58(6):776–84.
Hsieh CH, Lee CH, Liang JA, Yu CY, Shyu WC. Cycling hypoxia increases U87 glioma cell radioresistance via ROS induced higher and long-term HIF-1 signal transduction activity. Oncol Rep. 2010;24(6):1629–36.
Olcina MM, Foskolou IP, Anbalagan S, Senra JM, Pires IM, Jiang YY, Ryan AJ, Hammond EM. Replication stress and chromatin context Link ATM activation to a role in DNA replication. Mol Cell. 2013;52(5):758–66.
Marotta D, Karar J, Jenkins WT, Kumanova M, Jenkins KW, Tobias JW, Baldwin D, Hatzigeorgiou A, Alexiou P, Evans SM, et al. In vivo profiling of hypoxic gene expression in gliomas using the hypoxia marker EF5 and laser-capture microdissection. Cancer Res. 2011;71(3):779–89.
Masoud GN, Li W. HIF-1alpha pathway: role, regulation and intervention for cancer therapy. Acta Pharm Sin B. 2015;5(5):378–89.
Rapisarda A, Uranchimeg B, Sordet O, Pommier Y, Shoemaker RH, Melillo G. Topoisomerase I-mediated inhibition of hypoxia-inducible factor 1: mechanism and therapeutic implications. Cancer Res. 2004;64(4):1475–82.
We thank Dr. Nigel Jones and Prof Dave Fernig (University of Liverpool) for critical reading of the manuscript. We thank Dr. Jason Parson (University of Liverpool) for access to the CellRad Faxitron irradiator and Dr. Helen Wright (University of Liverpool) for her support with cell cycle analysis. We thank Damon Daniels (University of Manchester) for his help with micro-array analysis and Matlab coding.
C.F. and S.C. were funded by Alder Hey Children Hospital charitable funds. Immunostaining imaging was performed in the Liverpool Centre for Cell Imaging using equipment funded by the MRC (MR/K015931/1).
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All microarray raw and normalised data are available on NCBI: http://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE106959). All the data mentioned are included in the manuscript either as a main or supplemental figures.
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Figure S1. Hypoxia alone does not affect the cell cycle of D283-MED cells. D283-MED cells were pre-incubated in 1% O2 for 5 days or left in normoxia 21% O2. Cells were treated with etoposide (20 μM) for the indicated time. Cell survival was assessed using ViaCount assay. (B) Cells were incubated in 21% O2 or 5 days in 1% O2 and treated with etoposide (1 μM) for 30 h. Cell cycle profile obtained from the Guava software. Quantitative data showing the percentage of cells in each phase, value is calculated by dividing the number of cells in each phase by the total number of cells for that sample. (C) Cell cycle profiles obtained from flow cytometry. D283-MED cells were cultured in normoxia or hypoxia (1% O2) for indicated times. Cell cycle profile quantification showing percentage of cells in each cell cycle phase. (JPG 3287 kb)
Figure S2. Expression profile analysis (A) Network connection of upregulated genes in acute (6 h) hypoxia. IPA network analysis linking the genes interaction in the 6 h hypoxia expression data. The connections with HIF-1α are highlighted in light blue demonstrating a direct connection with two of its target genes, EGLN3 and PFKFB3. Genes highlighted in red are upregulated in our data at 6 h hypoxia. Altogether, ~ 30% of the upregulated genes in acute hypoxia have an interconnection with HIF-1, demonstrating a clear hypoxic response. (B, C) Clustergram analysis for apoptosis and cell signalling. An expression profile was produced for genes involved in (B) apoptosis and (C) cell signalling for D283-MED cells incubated in 1% O2 for 0–96 h. (JPG 3108 kb)
Figure S3. k-means clustering of regulated transcripts. Significantly regulated transcripts from microarray data clustered into one of 16 groups using k-means. Transcripts with similar expression level are grouped together in the same cluster. (JPG 3008 kb)
Figure S4. Expression of the MRN complex and ATM activation are not affected by chronic hypoxia in U87MG cells. U87MG cells were pre-incubated in 21% O2, 1% O2 or 0.1% O2 for 5 days prior to 4 h 100 μM etoposide treatment where indicated. (A) mRNA levels of NBN, MRE11, RAD50 were determined by qPCR, normalised to the housekeeping gene cyclophillin A and shown as fold change relative to normoxic control. (B) Levels of ATM and ATM serine 1981 determined using western blotting and densitometry of a representative western blot measured using ImageJ. (JPG 2679 kb)
Figure S5. ATM levels and ATM activation in hypoxic MEB-Med8A cells. MEB-Med8A cells were pre-incubated in 21% O2, 1% O2 or 0.1% O2 for 5 days prior to 4 h 50 μM etoposide treatment where indicated. Levels of ATM and ATM serine 1981 determined using western blotting and densitometry of a representative western blot measured using ImageJ. (JPG 2299 kb)
Figure S6. Etoposide induced p53 activity is dampened by chronic hypoxia in U87MG cells. U87MG cells were incubated in 1% O2 or 21% O2 for 5 days, prior to etoposide treatment where indicated. Three p53 target genes, MDM2, PUMA and p21 were assessed by qPCR. (A) Levels of MDM2, p21 and PUMA mRNA with or without etoposide treatment. Data represented as normalised to housekeeping gene (cyclophilin A) and fold change with respect to the untreated control. Data are representative of a single experiment. (B) Total p53 and phosphorylated p53 serine 15 levels assessed by western blot. Densitometry quantification of the band intensity was analysed by ImageJ of a single experiment. Plot represents p53 serine 15 normalised over the p53 total. (JPG 2722 kb)
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Cowman, S., Fan, Y.N., Pizer, B. et al. Decrease of Nibrin expression in chronic hypoxia is associated with hypoxia-induced chemoresistance in some brain tumour cells. BMC Cancer 19, 300 (2019). https://doi.org/10.1186/s12885-019-5476-9
- NBS-1 p53
- MRN complex
- Drug resistance
- DNA damaging agents
- Homologous recombination repair