Skip to main content
Download PDF

Proteomics reveals a therapeutic vulnerability via the combined blockade of APE1 and autophagy in lung cancer A549 cells

BMC Cancer volume 20, Article number: 634 (2020) Cite this article

Abstract

Background

Drug resistance is a major cause of therapeutic failure that is often associated with elevated autophagy and apurinic/apyrimidinic endonuclease 1 (APE1) expression. Herein, we investigated the role of APE1 and autophagy in A549 cells treated with cisplatin.

Methods

SILAC proteomics was applied to obtain a panoramic view of cisplatin treatment in KRASG12S-mutant A549 cells. Quantity analysis of cellular apoptosis and autophagy was based on flow cytometry. Western blotting was used to examine the expression levels of apoptosis- and autophagy-related proteins, as well as those of APE1. Knockdown of APE1 was achieved by RNA interference. Immunoprecipitation was further employed to reveal the molecular interaction of APE1, p53, and LC3 when A549 cells were exposed to cisplatin.

Results

SILAC proteomics revealed that 72 canonical pathways, including base excision repair (BER) and autophagy signalling pathways, were regulated after cisplatin treatment in A549 cells. Cisplatin markedly induced autophagy and apoptosis in A549 cells, accompanied by remarkable APE1 increase. Suppression of autophagy enhanced the inhibition effect of cisplatin on cell growth, proliferation, and colony formation; however, APE1 inhibition enhanced the expression of LC3-I/II, suggesting that APE1 and autophagy are compensatory for cell survival to evade the anticancer action of cisplatin. Immunoprecipitation results revealed the triple complex of APE1-p53-LC3 in response to cisplatin plus CQ in A549 cells. Dual inhibition of APE1 and autophagy significantly enhanced cisplatin-induced apoptosis, which eventually overcame drug resistance in cisplatin-resistant A549 cells.

Conclusions

Dual inhibition of APE1 and autophagy greatly enhances apoptosis in parental KRASG12S-mutant A549 cells and cisplatin-resistant A549 cells via regulation of APE1-p53-LC3 complex assembly, providing therapeutic vulnerability to overcome cisplatin resistance in the context of KRASG12S-mutant lung cancer.

Peer Review reports

Background

Lung cancer is the leading cause of cancer-related death and remains a major clinical challenge with increasing incidence and mortality [1, 2]. Due to drug resistance, recurrence, and metastasis, the treatment efficacy of lung cancer remains unsatisfactory. A better understanding of the aetiology, pathogenesis, and molecular targets is required to develop novel therapeutic modalities. Somatic gene mutations, including KRAS, EGFR, and TP53 mutations, is a major driver of lung cancer initiation [3]. Accumulating evidence has shown that not all gene mutations occur equally. In particular, compelling evidence suggests that RAS mutants function in an allele-specific manner, justifying the acquirement of a RAS allele-specific approach for RAS-driven cancer therapy [4,5,6]. Given the feature of allele specificity and the pivotal role of RAS in cellular events, including cell growth, cell survival, cell senescence, and cell death, novel strategies in a RAS allele-dependent manner are still required.

Autophagy is a cell survival-promoting mechanism following harsh stimuli and has been deeply implicated in cancer development and therapy [7,8,9]. Recently, targeting autophagy has been in the spotlight for cancer therapy via pharmacological inhibition alone or combination with other therapeutics [10, 11], providing insight into lung cancer therapy development. Cisplatin is one of the most frequently administered chemotherapeutic drugs for many solid tumours, including lung cancer. Mechanically, cisplatin kills cancer cells via interference with DNA synthesis and repair, subsequently inducing cell apoptosis [12]. However, there is limited clinical efficacy for cisplatin-based therapy because of drug resistance [13]. Several key factors contribute to cisplatin resistance, including autophagy [14] and apurinic/apyrimidinic endonuclease 1 (APE1) [15]. APE1 is a multifunctional protein with two major activities, DNA repair and transcriptional regulation [16]. Importantly, APE1 is often overexpressed in many tumours, contributing to disease progression, chemo-resistance and a poor prognosis [15, 17,18,19,20]. Our previous study found that APE1 is highly expressed in non-small cell lung cancer (NSCLC). Moreover, APE1 is a prognostic risk factor indicated by a poor overall survival [15, 19]. Herein, targeting APE1 might represent a therapeutic vulnerability for lung cancer, particularly, cisplatin-resistant lung cancer.

Thus, based on the aforementioned details, we hypothesized that APE1 and autophagy may contribute to lung cancer progression and drug resistance and that combined blockade of APE1 and autophagy enhances the therapeutic effect of cisplatin and overcomes cisplatin resistance in lung cancer. In the present study, we applied quantitative proteomics to identify the proteomic responses to cisplatin treatment in KRASG12S-mutant A549 cells. Both APE1 and autophagy were involved in the cellular responses to cisplatin exposure. In A549 cells and cisplatin-resistant A549 cells, cisplatin-induced apoptosis was significantly enhanced via the combination of autophagy inhibition by chloroquine (CQ) and APE1 knockdown by siRNA with the involvement of p53 activation.

Methods

Chemicals and reagents

CDDP was purchased from Selleckchem Inc. (Houston, TX, USA). 13C6-L-lysine, L-lysine, 13C615N4-L-arginine, L-arginine, Dulbecco’s modified Eagle’s medium (DMEM)/F12 for SILAC, APE1 siRNA, dimethyl sulfoxide (DMSO), 2-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT), bovine serum albumin, and Dulbecco’s phosphate-buffered saline (PBS) were obtained from Sigma-Aldrich (St. Louis, MO, USA). 6-Diamidino-2-phenylindole (DAPI), Opti-minimal Essential Medium (MEM), Lipofectamine 2000, and the negative control siRNA were purchased from Invitrogen Inc. (Carlsbad, CA, USA). The Annexin V-phycoerythrin (PE) apoptosis detection kit was purchased from BD Biosciences Inc. (San Jose, CA, USA). The Cyto-ID® Autophagy detection kit was obtained from Enzo Life Sciences Inc. (Farmingdale, NY, USA). The Western blotting substrate, Pierce™ bicinchoninic acid (BCA) protein assay kit, skim milk, and radioimmunoprecipitation assay buffer (RIPA) were purchased from Thermo Fisher Scientific Inc. (Hudson, NH, USA). The polyvinylidene difluoride (PVDF) membrane was obtained from Bio-Rad Inc. (Hercules, CA, USA). The antibody against human β-actin was obtained from Santa Cruz Biotechnology Inc. (Dallas, TX, USA). The remaining primary antibodies for signalling proteins related to apoptosis and autophagy were purchased from Cell Signaling Technology Inc. (Beverly, MA, USA).

Cell line and cell culture

The human lung cancer cell line A549 (KRASG12S) was obtained from Chinese Academy of Science Cellbank (Shanghai, China) and was cultured in RPMI1640 medium supplemented with 10% heat-inactivated foetal bovine serum (FBS). The cells were maintained at 37 °C in a 5% CO2/95% air humidified incubator.

Cell viability determination

The MTT assay was used to evaluate cell viability. Briefly, cells were seeded in 96-well plates at a density of 7.0 × 103 cells/well. After 24 h. of incubation, the cells were treated for 48 h. The absorbance was measured using a Synergy™H4 Hybrid microplate reader (BioTek, Winooski, VT, USA) at wavelengths of 560 nm (MTT formazan) and 670 nm (background).

Quantitative proteomics

Quantitative proteomic experiments were performed using a stable isotope labelling by amino acids in cell culture (SILAC)-based approach to identify the molecular targets of CDDP in the treatment of A549 cells as previously described [21]. Briefly, A549 cells were cultured in DMEM/F12 medium (for SILAC) with (heavy) or without (light) stable isotope-labelled amino acids (13C6 L-lysine and 13C615N4 L-arginine) and 10% dialyzed FBS. After treatment with CDDP (5 μM) for 24 h., the cell samples were harvested, lysed, and quantified. Next, an equal amount of heavy and light protein samples were combined to reach a total volume of 50 μL containing 400 μg of protein, and the combined protein sample was digested and desalted. Next, the peptide mixtures (5 μL) were subjected to the hybrid linear ion trap. The peptide SILAC ratio was calculated using MaxQuant version 1.2.0.13. The proteins were identified using Scaffold 4.3.2, and the pathway was analysed using ingenuity pathway analysis (IPA) from QIAGEN Inc.

Quantification of cellular apoptosis

Cell apoptosis was evaluated using the Annexin V-PE apoptosis detection kit as previously described [21]. Briefly, the cells were collected after treatment and resuspended in 1× binding buffer with 5 μL of Annexin V-PE and 5 μL of 7-amino-actinomycin D (7-AAD) at 1 × 105 cells/mL in a total volume of 150 μL. The cells were gently mixed and incubated in the dark for 15 min at room temperature. The binding buffer (100 μL) was then added to each tube, and the number of apoptotic cells was quantified using flow cytometry and collecting 10,000 events for analysis.

Quantification of cellular autophagy

Cell autophagy was examined using flow cytometry as previously described [21]. Briefly, the cells were collected after treatment and resuspended in 250 μL of assay buffer containing 5% FBS, and Cyto-ID® Green stain solution (250 μL) was added to each tube and mixed gently. After 20 min of incubation at room temperature in the dark, the cells were collected by centrifugation, washed once and analysed using the green (FL1) channel of flow cytometry.

Confocal fluorescence microscopy

Confocal microscopy was performed to evaluate the cellular autophagy level in A549 cells after treatment with 5 μM CDDP, 10 μM CQ, and 5 μM CDDP + 10 μM CQ using the Cyto-ID autophagy detection kits as previously described [21]. The fluorescence was assessed using TCS SP2 laser scanning confocal microscopy (LSCM).

Western blotting assay

The protein expression level was examined using Western blotting. Protein samples were extracted using RIPA buffer, the protein concentrations were measured using the BCA kit, and an equal amount of protein was separated by SDS-PAGE. The corresponding primary and secondary antibodies were applied to evaluate the expression levels of targeted proteins. Visualization was performed using the Bio-Rad ChemiDoc™ XRS system, and the blot bands were analysed using Image Lab 3.0.

RNA interference

Small interfering RNA-mediated gene silencing was performed to investigate the role of APE1 in cisplatin-induced apoptosis and autophagy in A549 cells according to the manufacturer’s instructions. A549 cells were transfected with the negative control siRNA and APE1-siRNA using Lipofectamine 2000. The protein samples were collected and kept at − 80 °C for further analysis.

Immunoprecipitation

The interaction between APE1 and p53 was examined using immunoprecipitation as previously described [22]. After 24 h. of treatment, A549 cells were lysed in pre-chilled cell lysis buffer [50 mM Tris-HCl (pH 7.4), 150 mM NaCl, 1 mM EDTA, 1% NP40, protease inhibitors] for 5 min. The lysates were precleared with 20 μL of Proteins A/G (Invitrogen; Thermo Fisher Scientific, Inc.) at 4 °C for 45 min, followed by incubation with APE1 or p53 antibody overnight at 4 °C. Following immunoprecipitation, the samples were incubated with protein G for 3 h. at 4 °C. Thereafter, the samples were washed with lysis buffer five times to remove any un-precipitated proteins before boiling in SDS buffer for 5 min. The elution was analysed for precipitated APE1 or p53 protein using Western blotting analysis. Normal rabbit IgG antibody was used as a negative control. The antibodies used were as follows: APE1 (1:500), p53 (1:500), and normal rabbit IgG (1:1000).

Statistical analysis

The data were expressed as means ± standard deviation (SD). One-way analysis of variance (ANOVA) followed by Tukey’s multiple comparison procedure was used for comparisons of multiple groups. The value of P<0.05 was considered statistically significant. The assays were performed at least three times independently.

Results

Overview of the proteomic response to cisplatin treatment in A549 cells

Until now, a lack of effective therapeutics persists for KRAS mutation-driven lung cancer. Compelling evidence has shown that RAS mutations vary and has spurred the development of new therapeutic vulnerabilities in a RAS allele-specific manner. To explore possible therapeutic targets, we applied SILAC-based proteomics to reveal the full spectrum of the molecular interactome in A549 cells in the context of the KRASG12S mutant following cisplatin exposure. We evaluated the proteomic responses to cisplatin (5 μM) treatment and identified at least 3262 protein molecules responding to cisplatin treatment, including APE1, p53, LC3-I/II, and many other functional proteins involved in DNA damage repair, cell proliferation, cell cycle, cellular metabolism, apoptosis, and autophagy. Subsequent IPA analysis revealed 1013 cellular functional proteins (450 proteins were upregulated; 563 proteins were downregulated) and 72 canonical signalling pathways that are involved in cell cycle control of chromosomal replication, RNA signalling, the BER pathway, DNA double-strand break repair by non-homologous end joining, ILK signalling, mismatch repair, mTOR signalling, ATM signalling, EGF signalling, telomere extension by telomerase, the spliceosomal cycle, the role of CHK protein in cell cycle checkpoint control, glycolysis I, gluconeogenesis I, DNA methylation and transcriptional repression signalling, the NRF2-mediated oxidative stress response, apoptosis, and autophagy (see Additional file 2: Supplementary Fig. 32A-B). As shown in Supplementary Fig. 32C, among the proteins in the BER pathway, APE1 expression was increased. Moreover, autophagy participated in the cellular responses to cisplatin treatment in A549 cells, as evident from the alteration in the expression of MAP1LC3 (also named as LC3) after cisplatin treatment (see Additional file 2: Supplementary Fig. 32D). Collectively, we speculated that both BER and autophagy pathways are involved in cisplatin-stimulated cellular responses in KRASG12S-mutant A549 cells. Thus, we subsequently investigated their roles in responses to cisplatin treatment.

Cisplatin induces autophagy and apoptosis and increases APE1 expression

As observed above regarding the proteomic responses to cisplatin treatment, autophagy and apoptosis were involved. Thus, we tested cisplatin-induced autophagy and apoptosis in A549 cells. Cisplatin decreased the number of viable A549 cells concentration-dependent manner (Fig. 1a). Cisplatin was reported to induce autophagy and apoptosis in various cancers, including lung cancer [23,24,25], and autophagy is related to chemo-resistance, providing a cell-protective mechanism that can promote tumour cell survival following different stresses, including chemotherapeutic treatment [26]. We showed that cisplatin treatment led to concentration- and time-dependent increases in autophagy in KRASG12S-mutant A549 cells and markedly increased the expression of LC3-I/II (Fig. 1b, d, f and g). Accompanying the autophagy phenomenon, the dose and timescale experiments showed that cisplatin treatment also induced remarkable apoptosis in A549 cells (Fig. 1c and e). Activation by the cleavage of PARP and caspase 3 only occurred at a high concentration of cisplatin (10 μM; Fig. 1f-g). Notably, the proteomic study showed that APE1 is involved in the responses to cisplatin treatment, and we previously showed that high APE1 expression in patients with NSCLC was positively correlated with poor overall survival, implying that APE1 is a prognostic risk factor [15, 19]. In the dose and timescale experiments, the expression of APE1 was dramatically increased following cisplatin treatment in A549 cells (Fig. 1f-g). Together, the results showed that cisplatin-induced autophagy and APE1 expression could counteract the apoptotic effect in KRASG12S-mutant A549 cells, suggesting the inhibition of autophagy or APE1 can enhance the cell-killing effect of cisplatin.

Fig. 1
figure 1

Cisplatin induces autophagy and apoptosis. a Cisplatin markedly inhibited A549 cell proliferation in a dose-dependent fashion. The IC50 value was 10.26 μM. b A549 cells were treated with cisplatin at 0.5, 5, and 10 μM for 24 h. Flow cytometry was used to determine cisplatin-induced autophagy. c A549 cells were treated with cisplatin at 0.5, 5, and 10 μM for 24 h. Flow cytometry was used to determine cisplatin-induced apoptosis. d Cisplatin-induced autophagy was performed in a time-dependent manner. A549 cells were treated with cisplatin at 5 μM for 1, 3, 6, 12 and 24 h. e A549 cells were treated with 5 μM cisplatin for 1, 3, 6, 12, and 24 h. Flow cytometry was used to determine apoptosis. f The expression levels of apoptosis- and autophagy-related proteins, as well as those of APE1, were examined using Western blotting after treatment with 0.5, 5, and 10 μM cisplatin for 24 h (see Additional file 1: Supplementary Figure 1-3). g The expression levels of apoptosis- and autophagy-related proteins, as well as APE1, were examined using Western blotting after treatment with 5 μM cisplatin for 1, 3, 6, 12, and 24 h (see Additional file 1: Supplementary Figure 4-7).

Full size image

Inhibition of autophagy enhances cisplatin-induced apoptosis

Recently, compelling evidence has shown that the inhibition of autophagic flux effectively enhances the tumour-suppressive effect of MAPK signalling inhibitors in the treatment of cancer [10, 11]. Chloroquine (CQ), originally used as an anti-malarial drug, has been in the spotlight as an autophagy inhibitor and a novel chemotherapeutic agent [10, 27]. CQ can diffuse through cell membranes and accumulate in cellular lysosomes, repressing autophagosome fusion with lysosomes [28, 29]. Thus, we tested the effect of CQ on cell growth and colony formation alone or in combination with cisplatin at low concentration (0.5 μM) in A549 cells. First, we showed that CQ decreased A549 cell viability at a high dose with an IC50 value at 38.46 μM (Fig. 2a). Next, we tested the effect of CQ on cell growth and viability alone and in combination with cisplatin. Treatment of A549 cells with 10 μM CQ did not affect cell growth compared with the control; however, 0.5 μM cisplatin remarkably suppressed cell growth after 1 week (Fig. 2b). Notably, combinatorial treatment of cells with CQ and cisplatin inhibited cell growth (Fig. 2b). Furthermore, co-treatment of A549 cells with CQ and cisplatin showed a higher inhibitory effect on cell colony formation than CQ or cisplatin treatment alone (Fig. 2c). Similarly, treatment of A549 cells with cisplatin alone increased the expression of LC3-I/II, whereas combinatorial treatment of cells with CQ and cisplatin decreased the expression of LC3-I/II (Fig. 2d), suggesting that inhibition of autophagic flux enhances the effect of cisplatin. Indeed, co-treatment of A549 cells with CQ and cisplatin enhanced cisplatin-induced apoptosis, whereas no effect of CQ on A549 cell apoptosis was observed (Fig. 3a-b). Intriguingly, APE1 expression was increased with both cisplatin treatment alone and in combination with CQ (Fig. 3b), suggesting APE1 counteracts the effect of dual treatment of cisplatin and CQ. Taken together, these data showed that inhibition of autophagic flux enhances the cisplatin-induced cell growth-suppressive effect and apoptosis.

Fig. 2
figure 2

Inhibition of autophagy enhances the inhibitory effect of cisplatin in A549 cells. a Inhibition of autophagy by CQ markedly decreased A549 cell viability. The IC50 value was 38.46 μM. b CQ (10 μM) enhanced the inhibitory effect of 0.5 μM cisplatin on cell proliferation. c CQ enhanced the inhibitory effect of cisplatin on cell colony formation. d CQ suppressed the expression level of cisplatin-induced autophagy (see Additional file 1: Supplementary Figure 8-9).

Full size image
Fig. 3
figure 3

Inhibition of autophagy enhances cisplatin-induced apoptosis in A549 cells. a Inhibition of autophagy by CQ markedly enhanced cisplatin-induced apoptosis in A549 cells. b Western blotting showed that CQ enhanced cisplatin-induced apoptosis in A549 cells (see Additional file 1: Supplementary Figure 10-12).

Full size image

Inhibition of APE1 stimulates autophagy in A549 cells

We first tested the effect of the mono-inhibition of APE1 on autophagy in A549 cells, which show high APE1 expression [30]. SiRNA-mediated knockdown or chemical inhibition of APE1 increased the expression of LC3-II (Fig. 4a-c). Confocal microscopic examination also showed that knockdown of APE1 increased autophagy compared with control siRNA (Fig. 4d). However, in the presence of cisplatin and CQ treatment alone or together, knockdown of APE1 not only reduced the expression level of LC3-I/II but also prevented nuclei accumulation (Fig. 4d). Additionally, the merged images showed co-localization of APE1 and LC3-I/II in A549 cells (Fig. 4d). Next, we performed immunoprecipitation to examine the possible interactions between LC3-I/II and key proteins involved in DNA damage, including APE1 and p53. Immunoprecipitation showed complex formation of APE1-p53-LC3 in response to cisplatin and CQ alone or in combination (Fig. 4e). Combinatorial treatment enhanced the formation of APE1-p53 but decreased LC3-II (Fig. 4E). Collectively, the data suggested that suppression of APE1 induces LC3-II expression, and autophagy plays an important role in cell survival in response to APE1 deficiency with the involvement of the interaction between APE1, p53, and LC3.

Fig. 4
figure 4

APE1 knockdown induces autophagy. a Si-RNA-mediated APE1 knockdown increased LC3-I/II expression (see Additional file 1: Supplementary Figure 13-14). b and c Inhibition of APE1 via E3330 or AT-101 increased LC3-I/II expression in A549 cells (see Additional file 1: Supplementary Figure 15-16). d Confocal microscopy showed that depletion of APE1 affected LC-3I/II localization. e Immunoprecipitation showed the interaction between APE1, LC3, and p53 in A549 cells (see Additional file 1: Supplementary Figure 17-20).

Full size image

Combined blockade of APE1 and autophagy promotes cisplatin-induced apoptosis in A549 cells

As demonstrated above, inhibition of autophagy or APE1 alone did not show an effective cell-killing effect in A549 cells because of the compensatory effect of autophagy and APE1. Thus, we speculated that combined blockade of autophagy and APE1 would further enhance the cell-killing effect of cisplatin in A549 cells. We applied a low concentration of cisplatin (2.5 μM), but the results showed no effect on autophagy in A549 cells (Fig. 5a). Knockdown of APE1 attenuated autophagy in the presence of cisplatin or CQ treatment alone or in combination; however, the depletion of APE1 enhanced apoptosis following treatment with cisplatin alone or in combination with CQ. Notably, the combinatorial treatment of CQ and cisplatin exerted the most effective apoptotic effect in the presence of APE1 knockdown (Fig. 5b). The protein expression level of LC3 and activation by the cleavage of PARP and caspase 3 reflected the autophagy and apoptosis (Fig. 5c). Notably, emerging data found that cisplatin stimulates p53 activity [31]. Consistent with the results, our data showed that cisplatin treatment alone or in combination with CQ increased p53 expression, as well as p-p53 (ser15) expression (Fig. 5c), suggesting that p53 is involved in the response to cisplatin treatment in A549 cells. Taken together, these results suggest that combined blockade of APE1 and autophagy enhances cisplatin-induced apoptosis with the involvement of p53 activation in A549 cells.

Fig. 5
figure 5

Combined blockade of autophagy and APE1 increases chemosensitivity and overcomes cisplatin resistance. a and b Knockdown of APE1 enhanced cisplatin-induced apoptosis in combination with autophagy inhibition by CQ. c Western blotting showed the enhancing effect of APE1 silencing on cisplatin-induced apoptosis in combination with autophagy inhibition by CQ (see Additional file 1: Supplementary Figure 21-26). d Knockdown of APE1 enhanced cisplatin sensitivity in combination with autophagy inhibition in cisplatin-resistant A549 cells. e Knockdown of APE1 enhanced cisplatin-induced apoptosis in combination with autophagy inhibition in cisplatin-resistant A549 cells. f Western blotting showed the enhancing effect of APE1 silencing on cisplatin-induced apoptosis in combination with autophagy inhibition in cisplatin-resistant A549 cells (see Additional file 1: Supplementary Figure 27-31).

Full size image

Dual repression of APE1 and autophagy reverses cisplatin resistance in cisplatin-resistant A549 cells

Acquired cisplatin resistance is the major cause of chemotherapy failure in the treatment of lung cancer; thus, we speculated that dual inhibition of APE1 and autophagic flux would overcome cisplatin resistance. We tested the effects on cell proliferation and apoptosis in acquired cisplatin-resistant A549 cells (parental A549 cells were exposed to cisplatin to develop the acquired resistant cell line, named A549/CDDP [32]) following dual inhibition of both the APE1 and autophagy. The cell viability was decreased in A549/CDDP cells receiving combinatorial treatment with cisplatin and CQ or cisplatin and APE1 siRNA compared with the vehicle or mono-treatment (Fig. 5d). Moreover, the most inhibitory effect on cell viability was observed in A549/CDDP cells receiving the combinatorial treatment with cisplatin, CQ, and APE1 knockdown (Fig. 5d). Next, the A549/CDDP cells were treated with a high concentration of cisplatin (20 μM) alone or in combination. Co-treatment with cisplatin and CQ resulted in increased apoptosis compared with mono-treatment in A549/CDDP cells, but co-treatment with APE1-SiRNA and cisplatin or CQ showed no enhancement in apoptosis compared with mono-treatment (Fig. 5e). The most potent apoptotic effect was observed in A549/CDDP cells treated with cisplatin, CQ, and APE1-SiRNA together. Knockdown of APE1 markedly sensitized A549/CDDP cells to the cisplatin/CQ combinatorial treatment (Fig. 5e). Protein expression also showed that the activation of p53 and PARP and caspase 3 cleavage occurred in A549/CDDP cells treated with cisplatin, CQ, and APE1-SiRNA together (Fig. 5f). No significant cleavage of PARP and caspase 3 was observed in the absence of APE1-SiRNA (Fig. 5F), suggesting the enhancing role of APE1 knockdown in apoptosis in cisplatin-resistant cells exposed to an autophagy inhibitor. Together, the data suggest that the combined blockade of APE1 and autophagy may be an effective strategy to overcome cisplatin resistance.

Discussion

Lung cancer is the leading cause of cancer death, and a lack of efficacious therapeutics exists. Cisplatin, the most important chemotherapeutic drug in lung cancer therapy, has shown limited clinical efficacy due to drug resistance. Autophagy and other key cellular events, including the DNA damage repair response, are involved in chemo-drug resistance. Notably, there is increasing attention on the genetic context dependence in lung cancer therapy. Compelling evidence has shown that oncogenic RAS mutations vary, although they all promote cancer cell proliferation [4,5,6]. Zhong et al. found that inhibition of RAS-AKT-mTOR signalling and blockage of late stage autophagy could synergistically enhance the cytotoxicity of a tumour suppressor gene ARHI [33]. Specific RAS alleles exhibit differential biochemical features, displaying preferential signalling output and favouring differential downstream effectors that are subject to differential feedforward and feedback regulations. Therefore, individualized therapeutics are advocated in cancer therapy.

In this study, we first applied SILAC proteomics to obtain a panoramic view of cisplatin treatment in KRASG12S-mutant A549 cells. At least 3262 protein molecules responded to cisplatin treatment and included APE1, p53, and LC3-I/II, which are involved in DNA damage repair, cell proliferation, apoptosis, and autophagy. Subsequent IPA analysis revealed 72 canonical signalling pathways including the BER pathway, DNA double-strand break repair, and autophagy pathways. Autophagy is a well-known cell-protective mechanism related to tumor progression, drug-resistance, and survive [8], and blockade of RAS/RAF/MEK/ERK signalling flux promotes autophagy [10], suggesting that inhibition of autophagy is beneficial. Kinsey et al. [10] and Bryant et al. [11] have shown synergistic antitumor effects of autophagy inhibition and MAPK inhibition in RAS-driven cancers, including pancreatic ductal adenocarcinoma, melanoma, and colorectal cancer, in preclinical settings [10, 11]. This combined blockade of autophagy with other therapeutics revealed a novel therapeutic vulnerability to treat RAS-driven cancers, including lung cancer. Based on our previous research concerning BER pathway in platinum-resistance of lung cancer [30] and present proteomic results, we herein aimed to investigate whether BER and autophagy have interaction upon cisplatin treatment in lung cancer cells. By methods of flow cytometry, fluorescence microscopy, Western blotting and RNA interference, we found that cisplatin markedly induced autophagy and apoptosis in A549 cells, accompanied by remarkable increase of DNA repair protein APE1. Suppression of autophagy enhanced the inhibition effect of cisplatin on cell growth, proliferation, and colony formation. The combination treatment of CQ, an autophagy inhibitor, with cisplatin dramatically enhanced cisplatin-induced apoptosis.

Moreover, APE1 is a major contributor to cisplatin resistance in lung cancer [15]. In the present study, knockdown of APE1 enhanced cisplatin-induced apoptosis in both A549 cells and cisplatin-resistant A549 cells. Noteworthy, APE1 knockdown significantly synergized the apoptosis-inducing effect of cisplatin plus CQ. This dual inhibition of APE1 and autophagy could minimize the curative concentration of cisplatin in cisplatin-resistant A549 cells. The lower concentration of cisplatin was beneficial in reducing the side effects of chemotherapy that commonly occur in clinical settings. Besides, the specific targeting of autophagy without affecting other cellular processes has drawn a great attention of researchers. Mutations in the RAS pathway are often associated with the high levels of autophagy that are required to maintain cancer cell metabolism [34, 35]. The optimal dosage of autophagy inhibitors and timing of inhibition are vital parameters for maximal therapeutic efficiency. Hopefully, Levy et al. reported that the treatment of CQ as an autophagy inhibitor in some cancer patients showed no adverse toxicity for extended time periods [36]. This demonstrates that long-term treatment with lysosomal autophagy inhibitors is feasible. Provided that cancer cells are more dependent than normal tissues on autophagy, even a drug that causes some normal tissue toxicity can have a valuable therapeutic window for an effective cancer treatment [8]. In inducible Atg7-knockout mice, the growth of KRAS-driven lung tumors was significantly inhibited before any signs of neurotoxicity [37], indicating that therapeutic window for autophagy inhibition exists in some cancers.

Additionally, our previous data found that promoting p53 intracellular stability by interfering with APE1 is a possible mechanism in genistein-induced apoptosis [38]. In the present study, we applied immunoprecipitation to explore the possible interactions between LC3-I/II and key proteins involved in DNA damage, including APE1 and p53. An interesting triple complex comprising APE1-p53-LC3 was formed in response to cisplatin plus CQ in A549 cells. Taken together, our results suggest that dual inhibition of APE1 and autophagy could enhance chemo-sensitivity and overcome cisplatin resistance by boosting apoptosis via the modulation of APE1-p53-LC3 complex assembly in a KRASG12S context. Whether the current findings regarding the cellular events recapitulate other RAS mutations in lung cancer or KRASG12S mutation in other cancer types in response to cisplatin treatment is unknown and warrants further investigation to better tailor specific therapeutic vulnerabilities for lung cancer treatment [3].

Conclusions

In summary, this study revealed a proteomic response to cisplatin in KRASG12S-mutant A549 cells. APE1, p53, and LC3-I/II were identified to be involved in DNA damage repair, cell proliferation, apoptosis, and autophagy. Dual inhibition of APE1 and autophagy synergistically enhanced cisplatin-induced apoptosis via the regulation of APE1-p53-LC3 complex assembly. This novel combination strategy is of great potential to overcome cisplatin resistance in the context of KRASG12S-mutant lung cancer.

Availability of data and materials

The datasets used in the current study are available from the corresponding author on reasonable request.

Abbreviations

APE1:

Apurinic/apyrimidinic endonuclease 1

NSCLC:

Non-small cell lung cancer

CDDP:

Cisplatin

CQ:

Chloroquine

DMSO:

Dimethyl sulfoxide

DMEM:

Dulbecco’s modified Eagle’s medium

PBS:

Dulbecco’s phosphate-buffered saline

FBS:

Foetal bovine serum

SILAC:

Stable isotope labelling by amino acids in cell culture

LSCM:

Laser scanning confocal microscope

DAPI:

6-diamidino-2-phenylindole

MTT:

2-(4,5-dimethylthiazol-2-yl)-2,5- diphenyltetrazolium bromide

RIPA:

Radioimmunoprecipitation assay buffer

PVDF:

Polyvinylidene difluoride

IPA:

INGENUITY Pathway Analysis

References

  1. Bray F, Ferlay J, Soerjomataram I, Siegel RL, Torre LA, Jemal A. Global cancer statistics 2018: GLOBOCAN estimates of incidence and mortality worldwide for 36 cancers in 185 countries. CA Cancer J Clin. 2018;68(6):394–424.

    Article  Google Scholar 

  2. Feng RM, Zong YN, Cao SM, Xu RH. Current cancer situation in China: good or bad news from the 2018 global Cancer statistics? Cancer Commun (Lond). 2019;39(1):22. https://doi.org/10.1186/s40880-019-0368-6.

    Article  Google Scholar 

  3. Rosell R, Bivona TG, Karachaliou N. Genetics and biomarkers in personalisation of lung cancer treatment. Lancet. 2013;382(9893):720–31.

    Article  CAS  Google Scholar 

  4. Haigis KM. KRAS alleles: the devil is in the detail. Trends Cancer. 2017;3(10):686–97.

    Article  CAS  Google Scholar 

  5. Hobbs GA, Der CJ. RAS mutations are not created equal. Cancer Discov. 2019;9(6):696–8.

    Article  Google Scholar 

  6. Gao Y, Chang MT, McKay D, Na N, Zhou B, Yaeger R, Torres NM, Muniz K, Drosten M, Barbacid M, et al. Allele-specific mechanisms of activation of MEK1 mutants determine their properties. Cancer Discov. 2018;8(5):648–61.

    Article  CAS  Google Scholar 

  7. White E. The role for autophagy in cancer. J Clin Invest. 2015;125(1):42–6.

    Article  Google Scholar 

  8. Levy JMM, Towers CG, Thorburn A. Targeting autophagy in cancer. Nat Rev Cancer. 2017;17(9):528–42.

    Article  CAS  Google Scholar 

  9. Garcia-Cano J, Ambroise G, Pascual-Serra R, Carrion MC, Serrano-Oviedo L, Ortega-Muelas M, Cimas FJ, Sabater S, Ruiz-Hidalgo MJ, Sanchez Perez I, et al. Exploiting the potential of autophagy in cisplatin therapy: a new strategy to overcome resistance. Oncotarget. 2015;6(17):15551–65.

    Article  Google Scholar 

  10. Kinsey CG, Camolotto SA, Boespflug AM, Guillen KP, Foth M, Truong A, Schuman SS, Shea JE, Seipp MT, Yap JT, et al. Protective autophagy elicited by RAF-->MEK-->ERK inhibition suggests a treatment strategy for RAS-driven cancers. Nat Med. 2019;25(4):620–7.

    Article  CAS  Google Scholar 

  11. Bryant KL, Stalnecker CA, Zeitouni D, Klomp JE, Peng S, Tikunov AP, Gunda V, Pierobon M, Waters AM, George SD, et al. Combination of ERK and autophagy inhibition as a treatment approach for pancreatic cancer. Nat Med. 2019;25(4):628–40.

    Article  CAS  Google Scholar 

  12. Dasari S, Tchounwou PB. Cisplatin in cancer therapy: molecular mechanisms of action. Eur J Pharmacol. 2014;740:364–78.

    Article  CAS  Google Scholar 

  13. Hill DP, Harper A, Malcolm J, McAndrews MS, Mockus SM, Patterson SE, Reynolds T, Baker EJ, Bult CJ, Chesler EJ, et al. Cisplatin-resistant triple-negative breast cancer subtypes: multiple mechanisms of resistance. BMC Cancer. 2019;19(1):1039. https://doi.org/10.1186/s12885-019-6278-9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  14. Wang J, Wu GS. Role of autophagy in cisplatin resistance in ovarian cancer cells. J Biol Chem. 2014;289(24):17163–73.

    Article  CAS  Google Scholar 

  15. Wang D, Xiang DB, Yang XQ, Chen LS, Li MX, Zhong ZY, Zhang YS. APE1 overexpression is associated with cisplatin resistance in non-small cell lung cancer and targeted inhibition of APE1 enhances the activity of cisplatin in A549 cells. Lung Cancer. 2009;66(3):298–304.

    Article  Google Scholar 

  16. Li M, Wilson DM. Human apurinic/apyrimidinic endonuclease 1. Antioxid Redox Signal. 2014;20(4):678–707.

    Article  CAS  Google Scholar 

  17. Wen X, Lu R, Xie S, Zheng H, Wang H, Wang Y, Sun J, Gao X, Guo L. APE1 overexpression promotes the progression of ovarian cancer and serves as a potential therapeutic target. Cancer Biomark. 2016;17(3):313–22.

    Article  CAS  Google Scholar 

  18. Xiao X, Yang Y, Ren Y, Zou D, Zhang K, Wu Y. rs1760944 Polymorphism in the APE1 Region is Associated with Risk and Prognosis of Osteosarcoma in the Chinese Han Population. Sci Rep. 2017;7(1):9331. https://doi.org/10.1038/s41598-017-09750-9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  19. Peng Y, Li Z, Zhang S, Xiong Y, Cun Y, Qian C, Li M, Ren T, Xia L, Cheng Y, et al. Association of DNA base excision repair genes (OGG1, APE1 and XRCC1) polymorphisms with outcome to platinum-based chemotherapy in advanced nonsmall-cell lung cancer patients. Int J Cancer. 2014;135(11):2687–96.

    Article  CAS  Google Scholar 

  20. Juhnke M, Heumann A, Chirico V, Hoflmayer D, Menz A, Hinsch A, Hube-Magg C, Kluth M, Lang DS, Moller-Koop C, et al. Apurinic/apyrimidinic endonuclease 1 (APE1/Ref-1) overexpression is an independent prognostic marker in prostate cancer without TMPRSS2:ERG fusion. Mol Carcinog. 2017;56(9):2135–45.

    Article  CAS  Google Scholar 

  21. He SJ, Shu LP, Zhou ZW, Yang T, Duan W, Zhang X, He ZX, Zhou SF. Inhibition of Aurora kinases induces apoptosis and autophagy via AURKB/p70S6K/RPL15 axis in human leukemia cells. Cancer Lett. 2016;382(2):215–30.

    Article  CAS  Google Scholar 

  22. Zhai D, Cui C, Xie L, Cai L, Yu J. Sterol regulatory element-binding protein 1 cooperates with c-Myc to promote epithelial-mesenchymal transition in colorectal cancer. Oncol Lett. 2018;15(4):5959–65.

    PubMed  PubMed Central  Google Scholar 

  23. Zhang Z, Shao Z, Xiong L, Yang S. Inhibition of autophagy enhances cisplatin-induced apoptosis in the MG63 human osteosarcoma cell line. Oncol Lett. 2015;10(5):2941–6.

    Article  CAS  Google Scholar 

  24. Shi S, Tan P, Yan B, Gao R, Zhao J, Wang J, Guo J, Li N, Ma Z. ER stress and autophagy are involved in the apoptosis induced by cisplatin in human lung cancer cells. Oncol Rep. 2016;35(5):2606–14.

    Article  CAS  Google Scholar 

  25. Chen JH, Zhang P, Chen WD, Li DD, Wu XQ, Deng R, Jiao L, Li X, Ji J, Feng GK, et al. ATM-mediated PTEN phosphorylation promotes PTEN nuclear translocation and autophagy in response to DNA-damaging agents in cancer cells. Autophagy. 2015;11(2):239–52.

    Article  Google Scholar 

  26. Das CK, Mandal M, Kogel D. Pro-survival autophagy and cancer cell resistance to therapy. Cancer Metastasis Rev. 2018;37(4):749–66.

    Article  CAS  Google Scholar 

  27. Hall EA, Ramsey JE, Peng Z, Hayrapetyan D, Shkepu V, O'Rourke B, Geiger W, Lam K, Verschraegen CF. Novel organometallic chloroquine derivative inhibits tumor growth. J Cell Biochem. 2018;119(7). https://doi.org/10.1002/jcb.26787.

  28. Circu M, Cardelli J, Barr M, O'Byrne K, Mills G, El-Osta H. Modulating lysosomal function through lysosome membrane permeabilization or autophagy suppression restores sensitivity to cisplatin in refractory non-small-cell lung cancer cells. PLoS One. 2017;12(9):e0184922. https://doi.org/10.1371/journal.pone.0184922.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  29. Zhang Y, Liao Z, Zhang LJ, Xiao HT. The utility of chloroquine in cancer therapy. Curr Med Res Opin. 2015;31(5):1009–13.

    Article  CAS  Google Scholar 

  30. Ren T, Shan J, Qing Y, Qian C, Li Q, Lu G, Li M, Li C, Peng Y, Luo H, et al. Sequential treatment with AT-101 enhances cisplatin chemosensitivity in human non-small cell lung cancer cells through inhibition of apurinic/apyrimidinic endonuclease 1-activated IL-6/STAT3 signaling pathway. Drug Des Devel Ther. 2014;8:2517–29.

    Article  CAS  Google Scholar 

  31. Hu F, Guo XL, Zhang SS, Zhao QD, Li R, Xu Q, Wei LX. Suppression of p53 potentiates chemosensitivity in nutrient-deprived cholangiocarcinoma cells via inhibition of autophagy. Oncol Lett. 2017;14(2):1959–66.

    Article  CAS  Google Scholar 

  32. Kuang P, Zhou C, Li X, Ren S, Li B, Wang Y, Li J, Tang L, Zhang J, Zhao Y. Proteomics-based identification of secreted protein dihydrodiol dehydrogenase 2 as a potential biomarker for predicting cisplatin efficacy in advanced NSCLC patients. Lung Cancer. 2012;77(2):427–32.

    Article  Google Scholar 

  33. Zhong C, Shu M, Ye J, Wang X, Liu Z, Zhao W, Zhao B, Zheng Z, Yin Z, Gao M, et al. Oncogenic Ras is downregulated by ARHI and induces autophagy by Ras/AKT/mTOR pathway in glioblastoma. BMC Cancer. 2019;19:441. https://doi.org/10.1186/s12885-019-5643-z.

    Article  PubMed  PubMed Central  Google Scholar 

  34. Lock R, Roy S, Kenific CM, Su JS, Salas E, Ronen SM, Debnath J. Autophagy facilitates glycolysis during Ras-mediated oncogenic transformation. Mol Biol Cell. 2011;22(2):165–78.

    Article  CAS  Google Scholar 

  35. Guo JY, Chen HY, Mathew R, Fan J, Strohecker AM, Karsli-Uzunbas G, Kamphorst JJ, Chen G, Lemons JM, Karantza V, et al. Activated Ras requires autophagy to maintain oxidative metabolism and tumorigenesis. Genes Dev. 2011;25(5):460–70.

    Article  CAS  Google Scholar 

  36. Levy JM, Thompson JC, Griesinger AM, Amani V, Donson AM, Birks DK, Morgan MJ, Mirsky DM, Handler MH, Foreman NK, et al. Autophagy inhibition improves chemosensitivity in BRAF(V600E) brain tumors. Cancer Discov. 2014;4(7):773–80.

    Article  CAS  Google Scholar 

  37. Karsli-Uzunbas G, Guo JY, Price S, Teng X, Laddha SV, Khor S, Kalaany NY, Jacks T, Chan CS, Rabinowitz JD, et al. Autophagy is required for glucose homeostasis and lung tumor maintenance. Cancer Discov. 2014;4(8):914–27.

    Article  CAS  Google Scholar 

  38. Zhu J, Zhang C, Qing Y, Cheng Y, Jiang X, Li M, Yang Z, Wang D. Genistein induces apoptosis by stabilizing intracellular p53 protein through an APE1-mediated pathway. Free Radical Bio Med. 2015;86:209–18.

    Article  CAS  Google Scholar 

Download references

Acknowledgements

We thank Prof. Dong Wang (from Daping Hospital, Army Medical University) for his kind advice concerning the design of the study and for improving the language and data interpretation of the manuscript.

Funding

The collection, analysis, and interpretation of data in this study were supported by grants from the Science & Technology Department of Sichuan Province (2020YJ0451), Introduction Foundation of High-level Talents of The First Affiliated Hospital, Chengdu Medical College (CYFY-GQ22), Health Commission of Sichuan Province (17PJ586). The manuscript writing and editing was supported by National Natural Science Foundation of China (81860480) and Youth Science Fund Project of Science and Technology Department of Jiangxi Province (20181BAB215022). The sponsor reviewed and approved the study protocol and the final version of the manuscript. All the analytic decisions were made by the authors, and the final version of the manuscript was approved by all authors.

Author information

Author notes

  1. Shu-Ting Pan and Ji Zhou contributed equally to this work.

Authors and Affiliations

  1. Department of Oral and Maxillofacial Surgery, The First Affiliated Hospital of Nanchang University, 17 Yongwai Main St, Nanchang, 330006, Jiangxi, China

    Shu-Ting Pan

  2. Health Management Centre, The First Affiliated Hospital, Chengdu Medical College, 278 Baoguang St, Xindu Distr, Chengdu, 610500, Sichuan, China

    Ji Zhou & Fang Yang

  3. Department of Pharmaceutical Sciences, College of Pharmacy, University of South Florida, 12901 Bruce B. Downs Boulevard, Tampa, Florida, 33612, USA

    Shu-Feng Zhou

  4. Oncology Department, The First Affiliated Hospital, Chengdu Medical College, 278 Baoguang St, Xindu Distr, Chengdu, 610500, Sichuan, China

    Tao Ren

Authors
  1. Shu-Ting Pan
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Ji Zhou
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Fang Yang
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Shu-Feng Zhou
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Tao Ren
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

STP performed most of the experiments. JZ and FY performed some of the experiments and prepared Figs. 1, 2, 3, 4 and 5. SFZ contributed to the study design and revised the manuscript. TR sponsored and performed the study and was a major contributor to the writing of the manuscript. All the authors read and approved the final manuscript.

Corresponding authors

Correspondence to Shu-Feng Zhou or Tao Ren.

Ethics declarations

Ethics approval and consent to participate

This study was approved by the Ethics Committee of The First Affiliated Hospital of Chengdu Medical College (the approval number is 2019CYFYHEC-MS-02). No ethics approval was required for the use of human cell lines in this study. Not applicable about data from any individual person and animal.

Consent for publication

Not Applicable.

Competing interests

The authors declare no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Additional file 1: Figure S1-S31.

Original gels and blot images. Image Lab 3.0 software (Bio-Rad, USA) was used to analyse the blots. The cropping of the blots was labelled with the symbol of “↓”. Corresponding uncropped full-length blots are presented in Supplementary Figure [1–31].

Additional file 2: Figure 32.

SILAC-based proteomics identifies cellular response molecules and some related signalling pathways in cells. A Twenty-seven cranial signalling pathways. B Hot-point picture. C BER signalling pathway. D Autophagy signalling.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Pan, ST., Zhou, J., Yang, F. et al. Proteomics reveals a therapeutic vulnerability via the combined blockade of APE1 and autophagy in lung cancer A549 cells. BMC Cancer 20, 634 (2020). https://doi.org/10.1186/s12885-020-07111-w

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s12885-020-07111-w

Keywords

  • Cisplatin
  • APE1
  • Autophagy
  • Chemotherapy
  • Non-small cell lung cancer
  • Apoptosis

BMC Cancer

ISSN: 1471-2407

Contact us