- Open Access
Enhanced sensitivity of celecoxib in human glioblastoma cells: Induction of DNA damage leading to p53-dependent G1 cell cycle arrest and autophagy
Molecular Cancer volume 8, Article number: 66 (2009)
Selective cyclooxygenase (COX)-2 inhibitors elicit anti-proliferative responses in various tumours, however the underlying anti-tumour mechanisms are unclear. Mutational inactivation of the tumour suppressor p53 gene is frequent in malignant gliomas. The role of p53 mutation in the anti-tumour responses of the selective COX-2 inhibitor celecoxib in human glioblastoma cells is unknown. In this study, we used human glioblastoma cells with various p53 status; U87MG (with high and low p53 functional levels), LN229 (functional p53) and U373MG (mutant p53) cells. Inhibition of p53 was achieved in U87MG cells transfected with E6 oncoprotein (U87MG-E6) and treated with pifithrin-α, a reversible inhibitor of p53 (U87MG-PFT). We investigated whether the anti-glioblastoma responses of celecoxib were p53-dependent, and whether celecoxib induced DNA damage leading to p53-dependent G1 cell cycle arrest, followed by autophagy or apoptosis.
Our findings demonstrated that celecoxib concentration-dependently reduced glioblastoma cell viability, following 24 and 72 hours of treatment. Inhibition of functional p53 in glioblastoma cells significantly reduced the anti-proliferative effect of celecoxib. In U87MG cells, celecoxib (8 and 30 μM) significantly induced DNA damage and inhibited DNA synthesis, corresponding with p53 activation. Celecoxib induced G1-phase cell cycle arrest, accompanied with p21 activation in U87MG cells. Cell cycle progression of U87MG-E6 and U87MG-PFT cells was not affected by celecoxib. In parallel, celecoxib induced G1 cell cycle arrest in LN229 cells, but not in U373MG cells. Autophagy was induced by celecoxib in U87MG and LN229 cells, as shown by the significantly greater population of acridine orange-stained cells and increased levels of LC3-II protein (in comparison with non-treated controls). Celecoxib did not induce significant autophagy in U87MG-PFT, U87MG-E6 and U373MG cells, which lack functional p53. Regardless of p53 status, celecoxib caused no significant difference in apoptosis level of U87MG, U87MG-PFT, U87MG-E6 and U373MG cells.
Our findings reveal that p53 increases human glioblastoma sensitivity to celecoxib. Celecoxib inhibits glioblastoma cell viability by induction of DNA damage, leading to p53-dependent G1 cell cycle arrest and p53-dependent autophagy, but not apoptosis.
Despite conventional therapy of surgical resection, radiotherapy and chemotherapy, the median survival of malignant glioma patients remain poor. Most patients with glioblastoma multiforme survive less than 2 years after diagnosis . Therapeutic improvements are needed to extend the survival of malignant glioma patients. Cyclooxygenase (COX)-2, an isoform of COX which is the rate-limiting enzyme in conversion of arachidonic acid into prostaglandins, is inducible in the presence of cytokines and growth factors during inflammation . The importance of COX-2 in carcinogenesis and brain tumour progression is highlighted by the detection of COX-2 in brain tumours [3, 4] and COX-2 overexpression in gliomas associated with poor prognosis . Targeting COX-2 with selective COX-2 inhibitors (NS-398, SC-236 and celecoxib) has proven effective to reduce human glioblastoma cell viability in vitro [4, 6–9] and in rodent models [6, 9–11]. Celecoxib is the only selective COX-2 inhibitor approved by the FDA for adjuvant treatment of patients with familial adenomatous polyposis.
The molecular events underlying the anti-tumour properties of COX-2 inhibitors are not fully understood. Several mechanisms have been proposed in various tumour models. COX-2 inhibition by celecoxib induces G1 cell cycle arrest, corresponding with activation of G1-phase cyclin-CDK inhibitors, p21 and p27 [12–14]. Celecoxib activates apoptotic proteins BAD, caspases and PARP, followed by cell apoptosis and reduced tumour cell proliferation [9, 13–17]. Anti-tumour mechanisms of COX-2 inhibitors also include inhibition of tumour angiogenesis , inhibition of prostaglandin-induced immunosuppressive activity  and increased DNA damage/reduced DNA repair capacity . Peroxidation of arachidonic acid into prostaglandins by COX generates reactive oxygen species and free radicals, which induce DNA damage and tumourigenicity . Inhibition of COX by COX inhibitors aspirin , nimesulide , rofecoxib and celecoxib  protects DNA from oxidative damage by scavenging hydroxyl radicals and superoxide in vitro in non-tumour models. However, prevention of DNA damage by COX inhibitors has not been reported in tumour cells. In contrast, aspirin significantly induces DNA damage of HT-29 human colon carcinoma , whereas celecoxib causes DNA damage in MCa-35 murine mammary and A549 human lung cancer cells . Whether COX-2 inhibitors induce DNA damage in glioblastoma cells is unclear.
Mutational inactivation of the tumour suppressor gene p53 (a regulator of cell growth and death) is frequently found in human tumours, with p53 mutation/inactivation reported in 63–65% of high-grade gliomas . Induction of DNA damage initiates a cascade of signalling with p53 activation (phosphorylation at Ser 15 and Ser 20) and subsequent transcriptional activation of p53 response genes (including p21, GADD45, BAX, PUMA, Bcl2 and NOXA), thus provoking cell cycle arrest and/or apoptosis . Genotoxic stress caused by DNA-damaging agents also induce p53-dependent autophagy [29, 30], the type II programmed cell death characterised by the formation of cytosolic double-membrane vesicles (autophagosomes) that engulf cellular content by digestion, when fused with lysosomes . The mechanisms of p53-dependent induction of autophagy are not fully understood, but are thought to involve both the transcription-independent functions (e.g. activation of the nutrient energy sensor AMP kinase) and transcription-dependent functions (e.g. upregulation of mTOR inhibitors PTEN and TSC1, or p53-regulated autophagy and cell death gene DRAM) [30, 32]. Anti-tumour mechanisms by COX inhibition have been shown to be either p53-dependent [33, 34] or p53-independent in various cancer and non-cancer cells. The anti-proliferative mechanism of COX-2 inhibitors underpin by autophagy induction in tumours is unclear. To date, only one recent report suggests that celecoxib induces both autophagy and apoptosis, mediated by P-glycoprotein independent of p53 mechanisms, in hepatocellular carcinoma cells . The role of p53 in celecoxib-induced autophagy and celecoxib-induced anti-proliferative responses clearly needs to be verified.
In this study, we investigated (a) whether the anti-proliferative response induced by celecoxib was dependent on the presence of functional p53 and b) whether celecoxib-induced DNA damage resulted in p53-dependent G1 cell cycle arrest, followed by apoptosis or autophagy. We studied the effect of celecoxib in human glioblastoma cells with various p53 status; U87MG cells with high and low levels of p53 [by both genetic (oncoprotein E6) and pharmaceutical intervention (pifithrin-α)], LN229 (with wild type p53 function despite a p53 mutation in the coding sequence ) and U373MG (with mutant p53) cells. Our findings show that the anti-proliferative sensitivity of celecoxib is dependent on p53 in human glioblastoma cells. We further demonstrate that celecoxib enhances glioma cytotoxicity by induction of DNA damage and p53-dependent G1 cell cycle arrest, followed by p53-dependent autophagy but not apoptosis.
Celecoxib concentration-dependently inhibited human glioblastoma cell viability, with enhanced anti-proliferative response by the presence of functional p53
Celecoxib concentration-dependently reduced the viability of human glioblastoma cells U87MG, which contains wild-type p53 (Figure 1A–D). To determine whether the anti-proliferative response to celecoxib was dependent on p53, we first compared the effect of celecoxib on viability of U87MG-E6 and U87MG cells. Viral oncoprotein E6 inhibits p53 function by abrogating specific DNA binding and transactivation of p53, sequestering p53 into the cytoplasm and accelerating its degradation . Inhibition of p53 by oncoprotein E6 reduced the sensitivity of U87MG cells to celecoxib, as shown by the enhanced U87MG-E6 cell viability following celecoxib treatment, compared with non-transfected U87MG cells (Figure 1A–B). Following 72 hours of celecoxib treatment, U87MG-E6 cells were significantly more viable than U87MG cells (P < 0.05, Figure 1B). The prerequisite of p53 to protect U87MG cells from the anti-proliferative effect of celecoxib was confirmed with U87MG cells treated with PFT (U87MG-PFT). PFT-α inhibits p53 by reversibly blocking p53-transcriptional activation . Inhibition of p53 by PFT significantly reduced sensitivity of U87MG cells to celecoxib, with enhanced U87MG-PFT cell viability at 24 and 72 hours following celecoxib treatment, compared with untreated U87MG cells (P < 0.05, Figure 1C–D).
The p53-dependent anti-proliferative response induced by celecoxib was also shown in LN229 and U373MG glioblastoma cells. Celecoxib (24 and 72 hours treatment) inhibited viability of LN229 and U373MG cells in a concentration-dependent manner (Figure 1E–F). At 72 hours of celecoxib treatment, U373MG cells (with mutant p53) were significantly more viable than LN229 cells (with functional p53; P < 0.05, Figure 1F). These results parallel the enhanced anti-proliferative responses of celecoxib in U87MG cells (high level of functional p53), compared with U87MG-E6 and U87MG-PFT (low functional level of p53), thus verifying a p53-dependent anti-proliferative response induced by celecoxib. In subsequent experiments, we tested the effect of celecoxib at 8 μM, a concentration equivalent to human plasma concentration following consumption of 800 mg/kg celecoxib daily (the FDA approved dosage for familial adenomatous polyposis ), as well as at 30 μM, a lower than EC50 concentration.
Celecoxib activated p53
We verified that stable transfection of U87MG cells with oncoprotein E6 inhibited p53 protein expression (Figure 2A). In U87MG and LN229 cells (both with functional p53), we analysed whether celecoxib activated p53 with resultant p53-dependent anti-proliferative effects. Western blot analysis showed that celecoxib enhanced total p53 protein expression in a concentration-dependent manner in U87MG and LN229 cells (Figure 2B). Activation of p53 by celecoxib was verified by translocation of p53 from cytoplasm into nucleus when U87MG cells were treated with celecoxib (8 and 30 μM, 18 hours treatment) compared with untreated controls (Figure 2C).
Celecoxib caused p53-dependent G1 cell cycle arrest, accompanied with p21 activation
We analysed the human glioblastoma cells to determine whether activation of p53 by celecoxib led to cell cycle arrest. We synchronised glioblastoma cells in serum-free media for 48 hours, with resultant 75.7 ± 1.6% of U87MG cells and 82.3 ± 1.7% of U87MG-E6 cells, being arrested at G0 phase. Thereafter, starved cells were released from serum-free condition and treated with celecoxib for 18 hours in medium containing 10% FBS. Following release from starvation, celecoxib activated p53, as shown by the enhanced total p53 expression in U87MG cells. Addition of PFT inhibited celecoxib-induced p53 expression (Figure 3A). At 18 hours following release from starvation, cell cycle analysis showed that 47.8 ± 2.7% of untreated U87MG cells remained in G1 phase. Celecoxib (in a concentration-dependent manner) prevented U87MG cells from entering S-phase, resulting in a significantly greater population of cells at G1-phase, compared to untreated controls (P < 0.05, Figure 3B, 3D). There was reciprocal reduction of celecoxib-treated U87MG cells in S- and G2M-phases, compared to untreated controls.
To establish whether the celecoxib-induced G1 cell cycle arrest in U87MG cell was dependent on p53, we analysed the effect of celecoxib (8 and 30 μM) on cell cycle progression of U87MG-PFT and U87MG-E6 cells. PFT by itself, prevented U87MG cells from entering S-phase, as demonstrated by the greater population of cells at G1-phase (58.7 ± 2.3%) compared to the population of untreated U87MG cells at G1 phase (47.8 ± 2.7%; Figure 3D). PFT (25 μM), being a transient and reversible inhibitor of p53, is less efficient in blocking elevated amount of p53 (such as when p53 expression was increased during serum starvation, data not shown), resulting in a greater population of U87MG-PFT cells at G1phase compared to the population of U87MG cells at G1 phase. In parallel, Xu et al. (2005) demonstrated that PFT (20 μM) had no effect on cell cycle progression of U87MG cells . Addition of celecoxib to PFT-treated U87MG cells did not affect the cell cycle progression when p53 was inhibited (P > 0.05, Figure 3B, 3D), suggesting a p53-dependent celecoxib-induced G1 cell cycle arrest in U87MG cells. Continuous inactivation of p53 by E6 in U87MG-E6 cells reduced the proportion of cells at G1 phase (29.5 ± 3.3%), compared with the population of U87MG cells at G1 phase (47.8 ± 2.7%). This is in accord with the functional role of p53 in arresting cells at G1 phase, as was previously shown . Similar to U87MG-PFT cells, celecoxib had no significant effect on U87MG-E6 cell cycle progression (P > 0.05, Figure 3B, 3D), thus confirming a p53-mediated G1 cell cycle arrest by celecoxib in U87MG glioblastoma cells.
82.4 ± 0.9% of LN229 and 51.0 ± 3.7% of U373MG cells were arrested at G0/1 phase, following 48 hours of starvation in serum-free media. At 18 hours following treatment (in media containing 10% FBS), celecoxib prevented LN229 cells from entering S-phase and concentration-dependently increased the percentage population of LN229 cells in G1 phase, compared with untreated controls (P < 0.05, Figure 3C, 3E). Celecoxib had no significant effect on cell cycle progression of U373MG cells (P > 0.05, Figure 3C, 3E). These findings parallel the effect of celecoxib that induces G1 cell cycle arrest in U87MG cells, but not U87MG-E6 or U87MG-PFT cells, thus verifying an induction of p53-dependent G1 cell cycle arrest by celecoxib in human glioblastoma cells.
Induction of G1 cell cycle arrest following DNA damage is dependent on up-regulation of CDK inhibitors such as p21, a direct transcriptional target of p53 that is strongly induced by DNA damage in cells expressing wild-type p53 . We analysed whether p53-dependent G1 cell cycle arrest caused by celecoxib was mediated via p21 activation. Under the same synchronised cell condition where celecoxib induced p53-dependent G1 cell cycle arrest, our data showed that celecoxib caused a concentration-dependent increased in p21 mRNA expression in U87MG cells, but not in U87MG-E6 cells where p53 expression was depleted (Figure 4A). We verified these findings by immunocytochemistry, which demonstrated nuclear induction of p21 when U87MG cells were treated with celecoxib (8 and 30 μM; Figure 4B). In U87MG-E6 cells, celecoxib (8 and 30 μM) caused no significant changes in p21 mRNA expression (Figure 4A) and nuclear p21 protein level (Figure 4B). These data suggest that celecoxib-induced p53-dependent G1 cell cycle arrest is mediated by p21 activation in U87MG cells.
Celecoxib induced p53-dependent cell autophagy but not apoptosis
We investigated the functional consequences of celecoxib on programmed cell death type I (apoptosis) and type II (autophagy), whether celecoxib inhibited glioma proliferation by p53-dependent induction of apoptosis or autophagy. In addition to inducing apoptosis, p53 is also known to protect cells from apoptosis and necrotic cell death . As such, inhibition of p53 by PFT and E6 significantly increased the apoptosis level of U87MG-PFT and U87MG-E6 cells, respectively, compared to the basal apoptosis level of U87MG cells (P < 0.05, Figure 5B). Similarly, the basal apoptosis level of U373MG cells (with mutant p53) was greater than LN229 and U87MG cells (both with functional p53; Figure 5B), as was also shown by others . Regardless of p53 status in the glioma cells, celecoxib (8 and 30 μM, 72 hours treatment) did not cause any significant change in apoptosis population of U87MG, U87MG-PFT, U87MG-E6 and U373MG cells (P > 0.05, Figure 5). Celecoxib concentration-dependently increased apoptosis population of LN229 cells, from 2.4 ± 0.4% (controls) to 3.2 ± 0.5% (8 μM, P > 0.05) and 4.0 ± 0.5% (30 μM; P < 0.05, Figure 5C) of total cell population. At 72 hours treatment, celecoxib (30 μM) significantly inhibited the survival of LN229 cells to a remaining viable population of 38.9 ± 7.4% (see Figure 1F; P < 0.05, Student's t-test). The small 1.6% increment in apoptosis level of LN229 cells following 72 hours celecoxib treatment (30 μM) suggests apoptosis as a minor mechanism to mediate the anti-proliferative response induced by celecoxib in LN229 cells. The non-significant change in apoptosis level following celecoxib treatment in U87MG, U87MG-PFT, U87MG-E6 and U373MG cells further demonstrates that an alternative major cell death mechanism (such as autophagy) is involved in the anti-proliferative response induced by celecoxib in human glioblastoma cells.
To analyse autophagy, we used acridine orange to stain acidic vesicular organelles (AVOs) that include autophagic vacuoles . In untreated U87MG cells, the cytoplasm and nucleolus fluoresced bright green and dim red. Celecoxib treatment induced the development of AVOs in U87MG cells, as shown by the concentrated fluorescence bright red acidic compartments (Figure 6A). The intensity of red fluorescence is proportional to the degree of acidity and/or volume of the cellular acidic compartment . An increase in the intensity of red fluorescence was observed in U87MG cells treated with increasing concentrations of celecoxib (from 8 to 30 μM, Figure 6A–B). When the AVO staining of celecoxib-treated U87MG cells was quantified, we demonstrated that 14.0 ± 3.9% and 18.4 ± 5.7% of total cells were significantly stained with acridine orange following celecoxib treatment (8 and 30 μM, respectively), compared with untreated controls (3.8 ± 0.0%; P < 0.05, Figure 6C). Inhibition of p53 by PFT significantly induced autophagy of U87MG cells (P < 0.05, Figure 6C; ). Addition of celecoxib had no significant effect on the acridine orange staining of U87MG-PFT cells (P > 0.05, Figure 6C). In U87MG-E6 cells with reduced level of p53, development of AVOs following celecoxib treatment was not obvious (by microscopic observation, Figure 6A) and statistically non-significant (by FACS analysis; P > 0.05, Figure 6B, 6C). We verified the celecoxib-induced p53-dependent autophagy in U87MG cells by the changes in expression of light chain 3 (LC3)-II, an autophagosome-specific protein that is recruited to the autophagosome membrane during autophagy . Celecoxib (8 and 30 μM) further induced cleavage of LC3 (conversion from LC3-I to LC3-II) in U87MG cells, in parallel with the development of AVOs following celecoxib treatment. Celecoxib (8 and 30 μM) had no effect on the level of LC3-II expression in U87MG-PFT and U87MG-E6 cells (Figure 6E).
In LN229 cells (with functional p53), celecoxib (8 and 30 μM, 72 hours treatment) significantly induced the development of AVOs (P < 0.05, Figure 6D), as shown by the significant increased of celecoxib-treated acridine orange-stained cells (14.8 ± 8.7% [8 μM] and 19.7 ± 7.4% [30 μM]), compared with controls (2.9 ± 1.8%). The level of autophagy induction by celecoxib in LN229 cells (4.0–5.8 fold of controls) was similar to the extent of autophagy induction in celecoxib-treated U87MG cells, which express functional p53. Celecoxib-induced autophagy response in LN229 cells was supported by the increased expression of LC3-II (Figure 6F). Celecoxib had no significant effect on the development of AVOs, or the level of LC3-II expression in U373MG cells, which contain mutant p53 (Figure 6D, 6F). These findings suggest that celecoxib induced p53-dependent autophagy rather than apoptosis in glioblastoma cells.
Celecoxib induced DNA damage and inhibited DNA synthesis
To investigate the upstream events preceding p53 activation following celecoxib treatment, we analysed the effect of celecoxib on DNA damage by Comet assays under non-denaturing condition, where induction of comet tails suggests DNA double-strand breaks. Following 5 and 18 hours of treatment, celecoxib (8 and 30 μM) significantly increased comet tail moments of U87MG cells (P < 0.05, Figure 7A). Normalised mean tail moments by celecoxib (30 μM) at 5 and 18 hours were 259 ± 37% and 372 ± 67%, respectively, of untreated controls (Figure 7A). The effect of celecoxib on DNA synthesis was assessed by incorporation of 3H-thymidine into DNA during cellular S-phase. Celecoxib (8 and 30 μM, 5 hours treatment) concentration-dependently inhibited DNA synthesis of U87MG cells (by 25–36% vs. controls, P < 0.05, Figure 7B), corresponding with celecoxib-induced DNA damage.
Therapeutic targeting of glioblastoma cells with selective COX-2 inhibitors such as celecoxib has demonstrated potential [4, 6–11]. However the underlying anti-proliferative mechanisms of COX-2 inhibitors remain unclear. Understanding the mechanisms underlying the anti-tumour properties of COX-2 inhibitors is needed for optimisation of therapeutic targeting by COX-2 inhibitors. In this study, we analysed the p53-dependent anti-proliferative effect induced by a selective COX-2 inhibitor, celecoxib in human glioblastoma cells. Our findings demonstrate that celecoxib induced p53-dependent G1 cell cycle arrest followed by autophagy, which are critical for inhibiting growth and proliferation of glioblastoma cells containing functional p53. We demonstrate insensitivity/resistance of glioblastoma cells to the anti-proliferative effect of celecoxib when p53 expression is inhibited/mutated, but enhanced cytotoxic response of celecoxib when glioblastoma cells express functional p53. Growth inhibition mediated via p53-dependent [33, 34, 48] and p53-independent [16, 49, 50] mechanisms have been reported with non-selective and selective COX-2 inhibitors in studies of tumour and non-tumour cells. In brain tumours, this finding is the first to report a p53-dependent anti-glioblastoma effect of a selective COX-2 inhibitor, which supports selective usage of celecoxib in human glioblastomas with functional p53 for enhanced anti-tumour responses.
p53 is a key molecule in DNA damage response, causing inhibition of cell proliferation by induction of cell cycle arrest, apoptosis/autophagy or senescence. The inhibitory effect of p53 on cell proliferation is due to transcriptional activation of target genes such as p21, GADD45, Bax, DR5 and PUMA . In this study, inhibition of COX-2 by celecoxib  activated p53 in human glioblastoma U87MG cells, as demonstrated by translocation of p53 from cytoplasm to nucleus accompanied with accumulation of total p53 expression. In line with our study, activation of p53 by COX inhibitors has also been demonstrated in colon and oral cancer cells [33, 34, 52]. We investigated whether celecoxib-induced p53 activation is followed by cell cycle arrest, apoptosis or autophagy in human glioblastoma cells. One study demonstrated a tumour cell-type dependent effect of cell cycle arrest and apoptosis following celecoxib treatment. Liu and colleagues (2003) reported that celecoxib-induced DNA damage led to G2M cell cycle arrest in mammary (and not lung) cancer, but apoptosis in lung (and not mammary) cancer cells . The underlying mechanisms for these differential celecoxib-induced functional responses were not addressed. Our study in human glioblastoma cells reveal that celecoxib-induced p53 activation is followed by p53-dependent G1 cell cycle arrest and p21 activation. Celecoxib-induced G1 cell cycle arrest accompanied by increased p21 protein expression has been reported in human cholangiocarcinoma , colorectal [13, 17], hepatocellular  and prostate cancer cells .
While apoptosis is considered a major anti-proliferative mechanism of celecoxib [9, 13–15, 17, 26], our findings show that induction of p53-dependent G1 cell cycle arrest by celecoxib is followed by p53-dependent cell autophagy and not apoptosis. It should be noted that higher concentrations of celecoxib (40–100 μM) induce apoptosis [9, 13–15, 17, 26]. The celecoxib concentrations (40–100 μM) are 4 to 11-fold greater than 8 μM, the human plasma concentration of celecoxib after consumption of 800 mg/kg per day  and the concentration that is presently used in this study. Mazzanti et al. (2009) recently showed that celecoxib (10 and 20 μM) induces apoptosis, but lower concentrations of celecoxib (at 2.5 and 5 μM) induce autophagy in hepatocellular carcinoma cells that are cultured in serum-free medium . The sensitivity of tumour cells to celecoxib-induced cellular apoptosis or autophagy is likely to be concentration- or tumour type-dependent. The role of p53 in autophagy remains controversial with studies suggesting activation of p53, as well as inhibition of p53, as inductive of autophagy . In our study, induction of autophagy by celecoxib in glioblastoma cells is p53-dependent, as shown by the autophagy induction only in celecoxib-treated glioblastoma cells with high (and not low) functional level of p53. In contrast, Mazzanti et al. (2009) reported that induction of autophagy by celecoxib (2.5 and 5 μM) is mediated by P-glycoprotein and Bcl2 via a p53-independent mechanism. The role of autophagy in cancer development is complex, as it has been implicated in both tumour survival and tumour cell death . Induction of cell cycle arrest preceding autophagy induction inhibits tumor growth . Our results support the induction of p53-dependent G1 cell cycle arrest, followed by autophagy as a mechanism for celecoxib to prevent glioma cell survival. Induction of p53-dependent autophagy independent of apoptosis should be considered as one of the underlying anti-proliferative mechanisms of COX-2 inhibitors, celecoxib in particular, in various tumours.
We investigated the 'up-stream' mechanisms preceding p53 activation in U87MG cells treated with celecoxib. We found that celecoxib (8 and 30 μM) induced DNA damage, accompanied with inhibition of DNA synthesis in U87MG cells, which led to p53-induced G1 cell cycle arrest and autophagy events. These findings of celecoxib-induced DNA damage followed by p53-dependent G1 cell cycle arrest and autophagy are clinically relevant since low concentration of celecoxib (8 μM) are attainable in human serum . In cancer cells, DNA damage was induced following celecoxib treatment (at high concentrations of 50 and 100 μM) in murine lung (A549) and mammary (MCa-35) cancer cells , and by the non-selective COX inhibitor aspirin in HT-29 human colon carcinoma . Activation of DNA damage-p53 signalling by COX-2 inhibitors has not been reported. One study proposes induction of DNA damage by the COX inhibitor R-flurbiprofen following the observation that R-flurbiprofen increases p53 (Ser 15) phosphorylation in colon cancer cells, but this has yet to be verified . Our study demonstrates that selective COX-2 inhibition by celecoxib induces DNA damage and inhibits DNA synthesis, resulting in p53 activation and subsequent anti-proliferative effects in glioblastoma cells. The mechanisms underlying celecoxib-induced DNA damage remain unclear and are beyond the scope of this study. Whilst inhibition of COX-2 expression is reported to reduce generation of reactive oxygen species and prevent DNA damage, recent studies show that COX-2 inhibitors celecoxib  and sulindac , induce reactive oxygen species to mediate anti-tumour responses. Seo et al. (2007) also showed that induction of reactive oxygen species by sulindac was accompanied by phosphorylation of p53 (Ser 15) and accumulation of p53 in human multiple myeloma cells . It is possible that celecoxib induces reactive oxygen species, followed by activation of DNA damage-p53 signalling to mediate anti-glioblastoma effects, but this requires further investigation.
Our study reveals an important underlying mechanism of celecoxib-mediated inhibition of glioblastoma cell growth, by induction of DNA damage leading to p53-dependent G1 cell cycle arrest and autophagy, but not apoptosis. These results highlight the importance of p53 for enhanced anti-glioblastoma response by celecoxib. With the clinical relevant concentration of celecoxib used in this study, the present findings support potential clinical application of celecoxib to improve therapy of glioblastoma multiforme patients.
Cell culture and drug treatment
Human glioblastoma cells U87MG, U373MG, LN229 (American Type Culture Collection, Rockville, MD) and U87MG-E6 (U87MG cells transfected with human papillomavirus E6 oncoprotein, kindly provided by Russell O. Pieper, UCSF Comprehensive Cancer Centre, San Francisco, CA) were grown in Dulbecco's modified Eagle's medium (DMEM) supplemented with fetal bovine serum (FBS, 10%), nonessential amino acids (100 μM), sodium pyruvate (1 mM), streptomycin (100 μg/ml) and penicillin (100 U/ml, Gibco BRL, Grand Island, NY) at 37°C in an atmosphere containing 5% CO2.
Celecoxib (Pfizer Pharmacia, New York, NY) and pifithrin-α (PFT, Sigma, St. Louis, MO) was prepared as 100 mg/ml and 10 mg/ml stock in dimethyl sulfoxide (DMSO; Sigma), respectively. Stock solutions were diluted to required concentrations with culture medium on the day of treatment. U87MG cells were treated with PFT (U87MG-PFT) for 30 minutes prior to celecoxib treatment. Vehicle DMSO was used as drug replacement in experimental controls. The final DMSO concentration did not exceed 0.15% (v/v). All experiments were performed in accordance with guidelines approved by the Institutional Review Board of National Cancer Centre, Singapore.
Cell viability assay
In 96-well plates, cells were treated with increasing concentrations of celecoxib to identify dose-dependent viability of U87MG, U87MG-E6, U87MG-PFT, LN229 and U373MG cells. In some cases, U87MG cells were pre-treated with PFT (25 μM) for 30 minutes prior to celecoxib treatment. After 24 and 72 hours, cells were stained with 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT, 1 mg/ml), incubated for 4 hours at 37°C, lysed with lysis buffer (N, N-dimethyl formamide, 50%; sodium dodecyl sulphate, 20%) and absorbance measured at 570 nm. Readings of celecoxib-treated cells were normalised against DMSO-treated controls.
Western blot analysis
Cells treated with DMSO or celecoxib (8 and 30 μM) were lysed and protein quantitated by Bradford assays (Bio-Rad Laboratories, Hercules, CA). Equal amounts of protein were separated in SDS-polyacrylamide gels and transferred onto nitrocellulose membranes (Amersham Biosciences). Membranes were blocked with 5% skim milk, incubated overnight (4°C) with monoclonal anti-p53 (DO-1, 1:500, Santa Cruz Biotechnology, Santa Cruz, CA) or rabbit polyclonal anti-LC3 (1:500, Santa Cruz Biotechnology), followed by horseradish peroxidase-conjugated secondary antibodies (Amersham Biosciences). Protein bands were visualised with ECL plus chemiluminescence kit (Amersham Biosciences). For loading controls, membranes were stripped and re-probed with horseradish peroxidase-conjugated anti-β-actin (Santa Cruz Biotechnology).
Celecoxib-treated (0, 8 and 30 μM) cells (grown on cover slips) were fixed and permeabilised in 0.2% Triton X-100. After wash, cells were blocked with 5% BSA, incubated with specific antibodies against p53 (1:50, Neomarkers, Fremont, CA) or p21 (1:100, Santa Cruz Biotechnology) for 1 hour at room temperature, followed by incubation with anti-mouse FITC-conjugated secondary antibodies (1:200, Molecular Probes). Cover slips were mounted with VectaShield Mounting Medium containing DAPI (Vecta Laboratories, Burlingame, CA). Images were viewed under a Laser Scanning Microscope and images captured using software LSM510 (Zeiss, Germany).
Cell cycle analysis and p21 mRNA expression
Cells were synchronised at Go phase in serum-free medium for 48 hours, followed by celecoxib treatment (0, 8 and 30 μM) in medium containing 10% FBS for 18 hours. In some cases, U87MG cells were pre-treated with PFT (25 μM) for 30 minutes prior to celecoxib treatment. For cell cycle analysis, collected cells were fixed overnight with ice-cold ethanol (75%), stained with propidium iodide (5 μg/ml, Sigma) supplemented with 100 μg/ml RNase (Sigma), and then analysed with flow cytometry using CellQuest Pro (BD Biosciences, San Jose, CA) for 10,000 events. For p21 mRNA analysis, total RNA was extracted from celecoxib-treated cells with Tri-Reagent (Molecular Research Centre, Cincinnati, OH). 1 μg total RNA was reverse transcribed using the ImProm-II Reverse Transcription system (Promega Corporation, Madison, WI). PCR was performed with specific primers for p21 (forward: 5'-CAGCATGACAGATTTCTACCAC-3', reverse: 5'-CCAGGGTATGTACATGAGGAG-3') and GAPDH (forward: 5'-GGAAGGTGAAGGTCGGAGTC-3', reverse: 5'-GTCTTCTGGGTGGCAGTGAT-3') at the following conditions: 94°C, 55°C and 72°C at 30 seconds each temperature for 30 cycles.
Apoptosis and autophagy assays
Cells were treated with DMSO or celecoxib (8 and 30 μM) for 72 hours. In some cases, U87MG cells were pre-treated with PFT (25 μM) for 30 minutes prior to celecoxib treatment. For apoptosis assays, trypsinised cells were incubated with FITC-conjugated Annexin V (BD Biosciences) and propidium iodide (5 μg/ml). 10,000 events were analysed for apoptosis by FACS with CellQuest Pro software. For autophagy assays, celecoxib-treated cells were stained with acridine orange (1 μg/ml, Sigma) for 15 mins at 37°C. Trypsinised cells were re-suspended in phenol red-free growth media (Gibco BRL) and 10,000 events were analysed by FACS with CellQuest Pro software. Acridine orange-stained cells grown on cover slips were viewed under a Laser Scanning Microscope and images captured using software LSM510.
Comet assays and 3H-thymidine incorporation assays
DNA damage was analysed by Comet assays as follows: Sub-confluent cells were treated with DMSO or celecoxib (8 and 30 μM) for 5 and 18 hours. Cells were mixed with 0.5% low melting point agarose and allowed to solidify on slides. Slides were immersed in lysis buffer, electrophoresis in tris-base buffer, stained with SYBR Green 1 (Trevigen, Gaithersburg, MD) and analysed with fluorescence microscopy. DNA damage, characterised by formation of comet tails, was quantitated by tail moments (multiplication of DNA tail migration from cell nucleus with DNA content) using Comet Score Freeware (Tritek Corporation, Summerduck, VA).
DNA synthesis was quantified with 3H-thymidine incorporation assays as follows: Sub-confluent cells were labeled with [methyl-14C]-thymidine (Amersham Biosciences, Buckinghamshire, UK) overnight, followed by celecoxib treatment (8 and 30 μM, 5 hours). After wash, cells were incubated with medium containing [methyl-3H]-thymidine (Amersham Biosciences) for 20 minutes, followed by 5% trichloroacetic acid and then 100% ethanol. Cells were air-dried, lysed in 1% sodium dodecyl sulphate and 10 mM NaOH, and subsequently the radioactivity measured with a liquid scintillation counter (Wallac, Turku, Finland). A control sample labelled with [methyl-14C]-thymidine alone was included to determine [methyl-14C]-thymidine signal spillover into [methyl-3H]-thymidine channel. DNA synthesis was presented as a percentage of [methyl-3H]-thymidine/[methyl-14C]-thymidine ratio in celecoxib-treated cells over controls.
All values are presented as mean ± standard error of mean (S.E.M.) and n indicates number of independent experiments. The concentration-dependent effect of celecoxib on viability of glioblastoma cells was analysed by 2-way analysis of variance (2-way ANOVA). The effect of celecoxib on DNA damage, DNA synthesis, cell cycle progression, autophagy and cell apoptosis were analysed by 1-way ANOVA, followed by Dunnett's test (control vs. celecoxib, 8 or 30 μM). The effect of PFT on cell apoptosis and autophagy in U87MG cells was analysed by Mann-Whitney U-test. A P value of less than 0.05 was considered to be significant. GB-STAT (Dynamic Microsystems, Silver Springs, MD) statistical package was used in all calculations.
analysis of variance
acidic vesicular organelle
bovine serum albumin
fetal bovine serum
Food and Drug Administration
Stupp R, Mason WP, Bent van den MJ, Weller M, Fisher B, Taphoorn MJ, Belanger K, Brandes AA, Marosi C, Bogdahn U, Curschmann J, Janzer RC, Ludwin SK, Gorlia T, Allgeier A, Lacombe D, Cairncross JG, Eisenhauer E, Mirimanoff RO, European Organisation for Research and Treatment of Cancer Brain Tumor and Radiotherapy Groups, National Cancer Institute of Canada Clinical Trials Group: Radiotherapy plus concomitant and adjuvant temozolomide for glioblastoma. N Engl J Med. 2005, 352: 987-996. 10.1056/NEJMoa043330
Marnett LJ, Rowlinson SW, Goodwin DC, Kalgutkar AS, Lanzo CA: Arachidonic acid oxygenation by COX-1 and COX-2. Mechanisms of catalysis and inhibition. J Biol Chem. 1999, 274: 22903-22906. 10.1074/jbc.274.33.22903
Deininger MH, Weller M, Streffer J, Mittelbronn M, Meyermann R: Patterns of cyclooxygenase-1 and -2 expression in human gliomas in vivo. Acta Neuropathol (Berl). 1999, 98: 240-244. 10.1007/s004010051075. 10.1007/s004010051075
Joki T, Heese O, Nikas DC, Bello L, Zhang J, Kraeft SK, Seyfried NT, Abe T, Chen LB, Carroll RS, Black PM: Expression of cyclooxygenase 2 (COX-2) in human glioma and in vitro inhibition by a specific COX-2 inhibitor, NS-398. Cancer Res. 2000, 60: 4926-4931.
Shono T, Tofilon PJ, Bruner JM, Owolabi O, Lang FF: Cyclooxygenase-2 expression in human gliomas: prognostic significance and molecular correlations. Cancer Res. 2001, 61: 4375-4381.
Petersen C, Petersen S, Milas L, Lang FF, Tofilon PJ: Enhancement of intrinsic tumor cell radiosensitivity induced by a selective cyclooxygenase-2 inhibitor. Clin Cancer Res. 2000, 6: 2513-2520.
Matsuo M, Yonemitsu N, Zaitsu M, Ishii K, Hamasaki Y, Fukuyama K, Tabuchi K, Miyazaki S: Expression of prostaglandin H synthase-2 in human brain tumors. Acta Neuropathol (Berl). 2001, 102: 181-187.
Kardosh A, Blumenthal M, Wang WJ, Chen TC, Schonthal AH: Differential effects of selective COX-2 inhibitors on cell cycle regulation and proliferation of glioblastoma cell lines. Cancer Biol Ther. 2004, 3: 55-62.
Nam DH, Park K, Park C, Im YH, Kim MH, Lee S, Hong SC, Shin HJ, Kim JH, Eoh W, McDonnell TJ: Intracranial inhibition of glioma cell growth by cyclooxygenase-2 inhibitor celecoxib. Oncol Rep. 2004, 11: 263-268.
Portnow J, Suleman S, Grossman SA, Eller S, Carson K: A cyclooxygenase-2 (COX-2) inhibitor compared with dexamethasone in a survival study of rats with intracerebral 9L gliosarcomas. Neuro Oncol. 2002, 4: 22-25. 10.1215/15228517-4-1-22
Levin VA, Giglio P, Puduvalli VK, Jochec J, Groves MD, Yung WK, Hess K: Combination chemotherapy with 13-cis-retinoic acid and celecoxib in the treatment of glioblastoma multiforme. J Neurooncol. 2006, 78: 85-90. 10.1007/s11060-005-9062-4
Han C, Leng J, Demetris AJ, Wu T: Cyclooxygenase-2 promotes human cholangiocarcinoma growth: evidence for cyclooxygenase-2-independent mechanism in celecoxib-mediated induction of p21waf1/cip1 and p27kip1 and cell cycle arrest. Cancer Res. 2004, 64: 1369-1376. 10.1158/0008-5472.CAN-03-1086
Maier TJ, Schilling K, Schmidt R, Geisslinger G, Grosch S: Cyclooxygenase-2 (COX-2)-dependent and -independent anticarcinogenic effects of celecoxib in human colon carcinoma cells. Biochem Pharmacol. 2004, 67: 1469-1478. 10.1016/j.bcp.2003.12.014
Narayanan BA, Condon MS, Bosland MC, Narayanan NK, Reddy BS: Suppression of N-methyl-N-nitrosourea/testosterone-induced rat prostate cancer growth by celecoxib: effects on cyclooxygenase-2, cell cycle regulation, and apoptosis mechanism(s). Clin Cancer Res. 2003, 9: 3503-3513.
Arico S, Pattingre S, Bauvy C, Gane P, Barbat A, Codogno P, Ogier-Denis E: Celecoxib induces apoptosis by inhibiting 3-phosphoinositide-dependent protein kinase-1 activity in the human colon cancer HT-29 cell line. J Biol Chem. 2002, 277: 27613-27621. 10.1074/jbc.M201119200
Dvory-Sobol H, Cohen-Noyman E, Kazanov D, Figer A, Birkenfeld S, Madar-Shapiro L, Benamouzig R, Arber N: Celecoxib leads to G2/M arrest by induction of p21 and down-regulation of cyclin B1 expression in a p53-independent manner. Eur J Cancer. 2006, 42: 422-426. 10.1016/j.ejca.2005.11.009
Grosch S, Tegeder I, Niederberger E, Brautigam L, Geisslinger G: COX-2 independent induction of cell cycle arrest and apoptosis in colon cancer cells by the selective COX-2 inhibitor celecoxib. Faseb J. 2001, 15: 2742-2744.
Masferrer JL, Leahy KM, Koki AT, Zweifel BS, Settle SL, Woerner BM, Edwards DA, Flickinger AG, Moore RJ, Seibert K: Antiangiogenic and antitumor activities of cyclooxygenase-2 inhibitors. Cancer Res. 2000, 60: 1306-1311.
Milas L, Furuta Y, Hunter N, Nishiguchi I, Runkel S: Dependence of indomethacin-induced potentiation of murine tumor radioresponse on tumor host immunocompetence. Cancer Res. 1990, 50: 4473-4477.
Shiff SJ, Rigas B: The role of cyclooxygenase inhibition in the antineoplastic effects of nonsteroidal antiinflammatory drugs (NSAIDs). J Exp Med. 1999, 190: 445-450. 10.1084/jem.190.4.445
Lee SH, Williams MV, Dubois RN, Blair IA: Cyclooxygenase-2-mediated DNA damage. J Biol Chem. 2005, 280: 28337-28346. 10.1074/jbc.M504178200
Hsu CS, Li Y: Aspirin potently inhibits oxidative DNA strand breaks: implications for cancer chemoprevention. Biochem Biophys Res Commun. 2002, 293: 705-709. 10.1016/S0006-291X(02)00271-1
Tardieu D, Jaeg JP, Deloly A, Corpet DE, Cadet J, Petit CR: The COX-2 inhibitor nimesulide suppresses superoxide and 8-hydroxy-deoxyguanosine formation, and stimulates apoptosis in mucosa during early colonic inflammation in rats. Carcinogenesis. 2000, 21: 973-976. 10.1093/carcin/21.5.973
Matthias C, Schuster MT, Zieger S, Harreus U: COX-2 inhibitors celecoxib and rofecoxib prevent oxidative DNA fragmentation. Anticancer Res. 2006, 26: 2003-2007.
Qiao L, Hanif R, Sphicas E, Shiff SJ, Rigas B: Effect of aspirin on induction of apoptosis in HT-29 human colon adenocarcinoma cells. Biochem Pharmacol. 1998, 55: 53-64. 10.1016/S0006-2952(97)00400-0
Liu W, Chen Y, Wang W, Keng P, Finkelstein J, Hu D, Liang L, Guo M, Fenton B, Okunieff P, Ding I: Combination of radiation and celebrex (celecoxib) reduce mammary and lung tumor growth. Am J Clin Oncol. 2003, 26: S103-109. 10.1097/00000421-200306000-00015
Newcomb EW, Madonia WJ, Pisharody S, Lang FF, Koslow M, Miller DC: A correlative study of p53 protein alteration and p53 gene mutation in glioblastoma multiforme. Brain Pathol. 1993, 3: 229-235. 10.1111/j.1750-3639.1993.tb00749.x
Norbury CJ, Zhivotovsky B: DNA damage-induced apoptosis. Oncogene. 2004, 23: 2797-2808. 10.1038/sj.onc.1207532
Zeng X, Yan T, Schupp JE, Seo Y, Kinsella TJ: DNA mismatch repair initiates 6-thioguanine–induced autophagy through p53 activation in human tumor cells. Clin Cancer Res. 2007, 13: 1315-1321. 10.1158/1078-0432.CCR-06-1517
Feng Z, Zhang H, Levine AJ, Jin S: The coordinate regulation of the p53 and mTOR pathways in cells. Proc Natl Acad Sci USA. 2005, 102: 8204-8209. 10.1073/pnas.0502857102
Klionsky DJ, Emr SD: Autophagy as a regulated pathway of cellular degradation. Science. 2000, 290: 1717-1721. 10.1126/science.290.5497.1717
Crighton D, Wilkinson S, O'Prey J, Syed N, Smith P, Harrison PR, Gasco M, Garrone O, Crook T, Ryan KM: DRAM, a p53-induced modulator of autophagy, is critical for apoptosis. Cell. 2006, 126: 121-134. 10.1016/j.cell.2006.05.034
Grosch S, Schilling K, Janssen A, Maier TJ, Niederberger E, Geisslinger G: Induction of apoptosis by R-flurbiprofen in human colon carcinoma cells: involvement of p53. Biochem Pharmacol. 2005, 69: 831-839. 10.1016/j.bcp.2004.11.026
Ho CC, Yang XW, Lee TL, Liao PH, Yang SH, Tsai CH, Chou MY: Activation of p53 signalling in acetylsalicylic acid-induced apoptosis in OC2 human oral cancer cells. Eur J Clin Invest. 2003, 33: 875-882. 10.1046/j.1365-2362.2003.01240.x
Mazzanti R, Platini F, Bottini C, Fantappie O, Solazzo M, Tessitore L: Down-regulation of the HGF/MET autocrine loop induced by celecoxib and mediated by P-gp in MDR-positive human hepatocellular carcinoma cell line. Biochem Pharmacol. 2009, 78: 21-32. 10.1016/j.bcp.2009.03.013
Pyrko P, Soriano N, Kardosh A, Liu YT, Uddin J, Petasis NA, Hofman FM, Chen CS, Chen TC, Schonthal AH: Downregulation of survivin expression and concomitant induction of apoptosis by celecoxib and its non-cyclooxygenase-2-inhibitory analog, dimethyl-celecoxib (DMC), in tumor cells in vitro and in vivo. Mol Cancer. 2006, 5: 19- 10.1186/1476-4598-5-19
Levine AJ: p53, the cellular gatekeeper for growth and division. Cell. 1997, 88: 323-331. 10.1016/S0092-8674(00)81871-1
Komarova EA, Gudkov AV: Suppression of p53: a new approach to overcome side effects of antitumor therapy. Biochemistry (Mosc). 2000, 65: 41-48.
McAdam BF, Catella-Lawson F, Mardini IA, Kapoor S, Lawson JA, FitzGerald GA: Systemic biosynthesis of prostacyclin by cyclooxygenase (COX)-2: the human pharmacology of a selective inhibitor of COX-2. Proc Natl Acad Sci USA. 1999, 96: 272-277. 10.1073/pnas.96.1.272
Xu GW, Mymryk JS, Cairncross JG: Pharmaceutical-mediated inactivation of p53 sensitizes U87MG glioma cells to BCNU and temozolomide. Int J Cancer. 2005, 116: 187-192. 10.1002/ijc.21071
Xu GW, Nutt CL, Zlatescu MC, Keeney M, Chin-Yee I, Cairncross JG: Inactivation of p53 sensitizes U87MG glioma cells to 1, 3-bis(2-chloroethyl)-1-nitrosourea. Cancer Res. 2001, 61: 4155-4159.
el-Deiry WS, Harper JW, O'Connor PM, Velculescu VE, Canman CE, Jackman J, Pietenpol JA, Burrell M, Hill DE, Wang Y: WAF1/CIP1 is induced in p53-mediated G1 arrest and apoptosis. Cancer Res. 1994, 54: 1169-1174.
Batista LF, Roos WP, Christmann M, Menck CF, Kaina B: Differential sensitivity of malignant glioma cells to methylating and chloroethylating anticancer drugs: p53 determines the switch by regulating xpc, ddb2, and DNA double-strand breaks. Cancer Res. 2007, 67: 11886-11895. 10.1158/0008-5472.CAN-07-2964
Yao KC, Komata T, Kondo Y, Kanzawa T, Kondo S, Germano IM: Molecular response of human glioblastoma multiforme cells to ionizing radiation: cell cycle arrest, modulation of the expression of cyclin-dependent kinase inhibitors, and autophagy. J Neurosurg. 2003, 98: 378-384. 10.3171/jns.2003.98.2.0378
Paglin S, Hollister T, Delohery T, Hackett N, McMahill M, Sphicas E, Domingo D, Yahalom J: A novel response of cancer cells to radiation involves autophagy and formation of acidic vesicles. Cancer Res. 2001, 61: 439-444.
Levine B, Abrams J: p53: The Janus of autophagy?. Nat Cell Biol. 2008, 10: 637-639. 10.1038/ncb0608-637
Kabeya Y, Mizushima N, Ueno T, Yamamoto A, Kirisako T, Noda T, Kominami E, Ohsumi Y, Yoshimori T: LC3, a mammalian homologue of yeast Apg8p, is localized in autophagosome membranes after processing. Embo J. 2000, 19: 5720-5728. 10.1093/emboj/19.21.5720
Cervi D, Truong AH, Lee JS, Sukhai N, Li YJ, Koki A, Ben-David Y: Phosphorylation status of c-Kit and Epo receptors, and the presence of wild-type p53 confer in vitro resistance of murine erythroleukemic cells to Celecoxib. Oncogene. 2004, 23: 2305-2314. 10.1038/sj.onc.1207400
Hida T, Yatabe Y, Achiwa H, Muramatsu H, Kozaki K, Nakamura S, Ogawa M, Mitsudomi T, Sugiura T, Takahashi T: Increased expression of cyclooxygenase 2 occurs frequently in human lung cancers, specifically in adenocarcinomas. Cancer Res. 1998, 58: 3761-3764.
Yoshinaka R, Shibata MA, Morimoto J, Tanigawa N, Otsuki Y: COX-2 inhibitor celecoxib suppresses tumor growth and lung metastasis of a murine mammary cancer. Anticancer Res. 2006, 26: 4245-4254.
Kang KB, Wang TT, Woon CT, Cheah ES, Moore XL, Zhu C, Wong MC: Enhancement of glioblastoma radioresponse by a selective COX-2 inhibitor celecoxib: inhibition of tumor angiogenesis with extensive tumor necrosis. Int J Radiat Oncol Biol Phys. 2007, 67: 888-896.
Swamy MV, Herzog CR, Rao CV: Inhibition of COX-2 in colon cancer cell lines by celecoxib increases the nuclear localization of active p53. Cancer Res. 2003, 63: 5239-5242.
Hippert MM, O'Toole PS, Thorburn A: Autophagy in cancer: good, bad, or both?. Cancer Res. 2006, 66: 9349-9351. 10.1158/0008-5472.CAN-06-1597
Tessitore L, Bonelli G, Cecchini G, Autelli R, Amenta JS, Baccino FM: Regulation of protein turnover versus growth state. Studies on the mechanism(s) of initiation of acidic vacuolar proteolysis in cells of stationary ascites hepatoma. Biochem J. 1988, 251: 483-490.
Ryan EP, Bushnell TP, Friedman AE, Rahman I, Phipps RP: Cyclooxygenase-2 independent effects of cyclooxygenase-2 inhibitors on oxidative stress and intracellular glutathione content in normal and malignant human B-cells. Cancer Immunol Immunother. 2008, 57: 347-358. 10.1007/s00262-007-0374-4
Seo SK, Lee HC, Woo SH, Jin HO, Yoo DH, Lee SJ, An S, Choe TB, Park MJ, Hong SI, Park IC, Rhee CH: Sulindac-derived reactive oxygen species induce apoptosis of human multiple myeloma cells via p38 mitogen activated protein kinase-induced mitochondrial dysfunction. Apoptosis. 2007, 12: 195-209. 10.1007/s10495-006-0527-5
The authors would like to thank A/Prof. Russell Pieper (UCSF Comprehensive Cancer Centre, San Francisco, CA) for providing the stable transfectant U87MG-E6 cells, and Yin Ling Wong for technical assistance in performing part of the cell viability assays. This study was supported by a grant from Singhealth Foundation, Singapore (SHF/FG023/2004). K.B. Kang was a recipient of the Post-doctoral Research Fellowship from the Singapore Millennium Foundation, Singapore.
The authors declare that they have no competing interests.
KBK, SKY and QHG performed the experiments. KBK drafted the manuscript, analysed and interpreted the experimental findings. KBK and ZCJ conceived the study and participated in experimental concept and design. KBK, ZCJ and WMC wrote the final version of manuscript. All authors read and approved the final manuscript.
Authors’ original submitted files for images
Below are the links to the authors’ original submitted files for images.
About this article
Cite this article
Kang, K.B., Zhu, C., Yong, S.K. et al. Enhanced sensitivity of celecoxib in human glioblastoma cells: Induction of DNA damage leading to p53-dependent G1 cell cycle arrest and autophagy. Mol Cancer 8, 66 (2009). https://doi.org/10.1186/1476-4598-8-66
- Glioblastoma Cell
- U87MG Cell
- Human Glioblastoma Cell
- LN229 Cell