Evidence-Based Complementary and Alternative Medicine

Evidence-Based Complementary and Alternative Medicine / 2018 / Article

Research Article | Open Access

Volume 2018 |Article ID 6049498 | 12 pages | https://doi.org/10.1155/2018/6049498

Xihuang Pill Induces Apoptosis of Human Glioblastoma U-87 MG Cells via Targeting ROS-Mediated Akt/mTOR/FOXO1 Pathway

Academic Editor: Ipek Goktepe
Received22 Feb 2018
Accepted16 May 2018
Published26 Jun 2018

Abstract

Xihuang pill (XHP), a traditional Chinese herbal formula, has long been used as an effective agent against multiple tumors. The aim of this study is to evaluate the effects of XHP on the growth inhibition and apoptosis in glioblastoma U-87 MG cells. Gas chromatography-mass spectrometry (GC-MS) was performed for constituent analysis of XHP. Cell viability, cell cycle arrest, generation of reactive oxygen species (ROS), and apoptosis were measured by CCK-8 assay, PI/RNase staining, DCFH-DA assay, TUNEL assay, Annexin V-FITC/PI double staining, and JC-1 assay, respectively. The role of XHP in the regulation of Akt/mTOR/FOXO1 interaction was clarified by using Western Blotting (WB), immunofluorescence (IF), pharmacological inhibitor or antioxidant, and siRNA silencing. The results suggested that XHP could inhibit U-87 MG cells growth and arrest cells in S-phase cell cycle significantly and that the generation of ROS, collapse of mitochondrial membrane potential, enhancement of Bax/Bcl-xL ratio, and reduction of the precursor forms of caspase-9 and caspase-3 caused by XHP prompted that a ROS-mediated mitochondria-dependent apoptosis was possibly involved. Furthermore, XHP affected the Akt/mTOR/FOXO1 pathway via inhibiting the phosphorylation of Akt, mTOR, and FOXO1 and increasing both prototype and nuclear translocation of FOXO1. Inhibition of Akt, mTOR, and FOXO1 by specific inhibitors or siRNA could interpose the apoptotic induction. In conclusion, we demonstrate for the first time that XHP may regulate glioblastoma U-87 MG cell apoptosis via ROS-mediated Akt/mTOR/FOXO1 pathway.

1. Introduction

Gliomas, a type of highly heterogeneous tumor, have been the leading lethal causes in primary central nerve system (CNS) tumors. According to the 2016 World Health Organization (WHO) classification of CNS tumors, gliomas in adults are mainly included astrocytoma (Grades I-IV), oligodendroglioma (Grades II-III), oligoastrocytoma (Grades II-III), and glioblastoma multiforme (GBM) (Grade IV) [1, 2]. GBM, the most aggressive and malignant form of gliomas, is distinguished by highly invasive behaviors with tentacle-like projections, making complete surgical removal difficult. Median overall survival of GBM patients is less than 18 months despite the adoption of optimized therapeutic scheme in combination of neurosurgery, chemotherapy, and radiotherapy [3]. In consideration of the significant toxicity and chemotherapy resistance in treatment, it is necessary to develop other effective strategies, for example, the exploration of potential benefits from traditional herbal formulas for glioblastoma treatment.

Xihuang pill (XHP, also called Xihuang Wan), a formula composed by four traditional Chinese medicines, Olibanum, Myrrh, Moschus, and Calculus bovis, has been used as a complementary and alternative medicine for tumor treatment in China since 18th century [4]. In modern clinical application, XHP has been proved effectively on various solid tumors including breast cancer [5], cervical cancer [6], glioma [7], colorectal cancer [8], and non-Hodgkin's lymphoma [9]. The experimental research showed that its ability to induce apoptosis in cancer cells or cancer stem cells (CSCs) was possibly attributed to the mitochondrial-related B-cell lymphoma- (Bcl-) 2 regulation [10, 11], extracellular signal-regulated kinase (ERK)/mitogen-activated protein kinase (MAPK) [12], or Wnt [13] signaling pathways, as well as cell cycle arrest [14, 15]. The invasion and metastasis inhibition were relevant to epithelial-mesenchymal transition (EMT) factor, Zinc finger E-box-binding homeobox 1 (ZEB1), and its downstream target genes ERK1/2, E-Cadherin, Occludin, matrix metalloprotein- (MMP-) 2, MMP-9, and junctional adhesion molecule- (JAM-) 1 [16, 17]. In addition, XHP could inhibit vasculogenic mimicry formation to reduce angiogenesis by downregulating expression of VE-Cadherin, MMP-2, and phosphorylated eph-receptor tyrosine kinase-type A2 (p-EphA2) [18]. Moreover, XHP exhibited the capability of converting tumor immunosuppressive microenvironment by reducing proportion of immunosuppressive cells such as myeloid-derived suppressor cells (MDSCs) and Treg cells [19], or by downregulating expression of cytokines such as interleukin- (IL-) 6, IL-10, and transforming growth factor- (TGF-) β [20] or by increasing IL-2, Interferon- (IFN-) γ, and the ratio of CD4+/CD8+ T cells [21, 22].

Despite the above widely described antitumor properties of XHP, little research has been devoted to GBM. On account of XHP’s definite clinical efficacy on GBM and its unclear molecular mechanisms, additional studies on this subject are necessary. In this study, we investigated the effects of XHP on human U-87 MG glioblastoma cell growth and its underlying mechanisms related to ROS-mediated Akt/mTOR/FOXO1 pathway, so as to provide some experimental data to the further research and development on antiglioblastoma application of XHP.

2. Materials and Methods

2.1. Reagents and Antibodies

XHP was purchased from Tong Ren Tang Technologies Co., Ltd. (Beijing, China). Cell counting kit- (CCK-) 8 assay kit was obtained from Dojindo (Tokyo, Japan). PI/RNase Staining Buffer (RUO) for cell cycle detection was purchased from BD Biosciences (Franklin Lakes, USA). Annexin V-FITC/PI apoptosis kit (640914) was purchased from Biolegend (San Diego, USA). Reactive oxygen species assay kit, TdT-mediated dUTP nick end labeling (TUNEL) kit, and JC-1 kit were purchased from Beyotime Biotechnology (Beijing, China). LY294002 and rapamycin were purchased from MedChemExpress (Shanghai, China). Paclitaxel (PTX) and N-acetylcysteine (NAC) were purchased from Sigma-Aldrich Corp. (St. Louis, USA). SignalSilence® FOXO1 siRNA (6256) and Control siRNA (6568) were purchased from Cell Signaling Technology (Beverly, USA). Lipofectamine™ 2000 transfection reagent was purchased from Thermo Fisher Scientific, Inc. (Carlsbad, USA); BCA protein quantification kit (FD2001) was purchased from Fdbio Science (Hangzhou, China). Mammalian target of rapamycin (mTOR) (2983), phospho-mTOR (Ser2448) (5536), Akt (pan) (4691), phospho-Akt (Ser473) (4060), forkhead transcription factor (FOXO)-1 (C29H4) (2880), phospho-FOXO1 (Thr24) (4G6) (2599), caspase-3 (9662), caspase-9 (9508), B-cell lymphoma-extra large (Bcl-xL) (B9429), Bcl-2-associated X protein (Bax) (5023), and GAPDH (5174) primary antibodies were purchased from Cell Signaling Technology.

2.2. Constituents Analysis of XHP by GC-MS

The powered XHP (3.0g) were extracted with 70% ethanol at room temperature by ultrasonic extraction for 30 min. The extract solution was concentrated and then partitioned by 2 mL of hexane and 5 mL of water. The supernatant was transferred and evaporated to dryness. The oil extract was filtered by 0.22 μM microporous membrane and stored at 4°C until analysis. The analysis was performed on an Agilent 6890/5973 GC-MS (Agilent Co., Palo Alto, CA, USA) using splitless injection mode, equipped with a TG-5MS capillary column (30 m × 0.25 mm × 0.25 μm, Thermo Fischer Co., Waltham, MA, USA). Helium was used as carrier gas at a flow rate of 1.0 mL/min. The temperature of the split injector was 250°C and the split ratio was 10:1. 1mL sample solution was injected into GC system. The column was initiated at 80°C at a rate of 8°C/min to 200°C and kept for 15 min, then to 260°C at 10°C/min and kept for 32min. The spectrometer was operated in the EI-mode at 70 eV and the photomultiplier voltage energy at 1988V. The ion source temperature was 230°C and the quadrupole temperature was 150°C. Mass scan range from 30 to 550 amu, and the components were identified by comparing with the data bank mass spectra (NIST 11 and Wiley 275).

2.3. Cell Line and Cell Culture

Human glioblastoma U-87 MG cells were obtained from the American Type Culture Collection (Rockville, USA). Cells were maintained in Dulbecco’s modified Eagle’s medium (DMEM) (Gibco, New York, USA) supplemented with 10% fetal bovine serum (Gibco, New York, USA) at 37°C in a humidified atmosphere of 5% CO2. After reaching 80% confluence, cells were used for analysis. All treatments were performed using 3% FBS supplemented medium.

2.4. Cell Viability Assay

The cell viability was examined by CCK-8 assay according to the manufacturer's instructions. Cells were seeded at a density of 5 × 103 per well in 96-well plates (Corning, New York, USA). After cultured overnight, cells were treated with various concentrations of XHP (7.5, 15 and 30 μg/mL) and incubated for 24h. Then 10 μL of CCK-8 reagent was added to the culture medium and incubated at 37°C for 1-2h. The absorbance was measured at a wavelength of 450 nm using a microplate reader (Thermo FC, Waltham, USA) to reflect cell viability. The % cell inhibition was determined using the following formula:

Nonlinear regression graph was plotted between % cell inhibition and Log10 concentration and calculation of IC50 value was determined using GraphPad Prism software 5.0 (GraphPad, San Diego, CA). Each assay was repeated in triplicate and the results were given as mean ± SD of independent experiments.

2.5. Cell Cycle Assay by Flow Cytometry

Based on CCK-8 assay results, the same three concentrations of XHP (7.5, 15, and 30 μg/mL) were used for the cell cycle assay. U-87 MG cells were collected after treatment for 24h and then fixed in 80% ethanol at 4°C overnight. On the next day, the cells were washed and suspended in phosphate-buffered saline (PBS) containing 50 μg/mL propidium iodide at 37°C for 30min. The fluorescence-activated cells were further analyzed on a FACS Calibur (BD Biosciences, San Joe, USA).

2.6. Apoptosis Assay by Flow Cytometry

Apoptotic U-87 MG cells were detected by Annexin V-FITC/PI double staining with the apoptosis detection kit. Briefly, cells were harvested after XHP (7.5, 15, and 30 μg/mL) treatment for 24h. Then, cells were centrifuged at 2000 rpm; the pellets were washed twice using PBS. Subsequently, cells were resuspended and labeled in the fluorochrome (5 μL Annexin V and 10 μL propidium iodide) and incubated for 15min at room temperature in darkness. After that, flow cytometry analysis was performed on a FACS Calibur. The fluorescence of FITC and PI were measured in the FL1 channel and FL2 channel ( = 488 nm, = 530 nm), respectively. 1 × 105 events were recorded for each sample. The data were analyzed by FlowJo software V7.6 (ETree star, Ashland, OR).

2.7. Apoptosis Detection by TUNEL Staining

Apoptotic cells were detected using TUNEL FITC apoptosis detection kit. Briefly, after being treated with XHP (7.5, 15 and 30 μg/mL) for 24h, U-87 MG cells were fixed with 4% Paraformaldehyde (PFA), permeabilized with 0.2% Triton X-100 and labeled with TdT reaction mix. DAPI (4′, 6-diamidino-2-phenylindole) was used to stain nuclei. Confocal microscopy (Nikon C2plus, Tokyo, Japan) was applied to observe morphological nuclear DNA fragmentation in the stained U-87 MG cells.

2.8. Measurement of Mitochondrial Membrane Potential (ΔΨm)

Mitochondrial membrane potential (MMP) was measured by a JC-1 assay kit. U-87 MG cells were seeded in 6-well plates (2 × 105/well) and incubated at 37°C overnight. Next, the cells were harvested after the desired treatments with XHP for 24h and then incubated in darkness at 37°C for 30min with 10 mM JC-1 contained PBS buffer. Finally, The green (JC-1 monomers) and red (JC-1 aggregates) fluorescence ratio that measured the proportion of mitochondrial depolarization was acquired on a FACS Calibur.

2.9. Detection of Intracellular ROS Levels by Flow Cytometry

Intracellular ROS production was detected using reactive oxygen species assay kit according to the manufacturer’s instruction. After U-87 MG cells pretreated with 30 μg/mL XHP for 0.5h, 1h, or 3h, the cells were loaded with fluorescent probe DCFH-DA at a final concentration of 10 μM in serum-free cell culture medium for 30 min at 37°C in the dark. After DCFH internalization, the cells were washed three times with serum-free cell culture medium to remove excess DCFH-DA, then the cells were collected and the fluorescence intensity of DCF was quantified on a FACS Calibur ( = 488/525 nm). 100 mM H2O2 was used as a positive control.

2.10. Western Blot Analysis

After being treated with XHP for 24h, U-87 MG cells were lysed with a NP-40 buffer and the total protein was extracted using radio immunoprecipitation assay buffer containing 1% protease inhibitor cocktail (Roche, Basel, Switzerland). The protein concentration was measured using a BCA protein assay kit (Fdbioscience, China). 20-50 μg of cellular proteins was electroblotted onto PVDF membranes following separation on 12% SDS-PAGE gel electrophoresis. Membranes were blocked with 5% no-fat milk at room temperature for 1h and then blotted with primary antibodies (Bcl-xL, Bax, caspase-3, caspase-9, Akt, p-Akt, mTOR, p-mTOR, FOXO1, p-FOXO1, and GAPDH) at 4°C overnight with a 1:1000 dilution. Blots were then incubated with HRP-conjugated secondary antibodies at room temperature for 1h, followed by ECL development (Bio-Rad Laboratories, Hercules, USA). The images were captured and documented with a CCD system (imagestation 2000 MM, Kodak, Rochester, USA) and gray density was analyzed using ImageJ software (NIH, USA). Protein expression levels were determined using GAPDH as an internal control.

2.11. Immunofluorescence Staining

After being treated with XHP for 24h, U-87 MG cells were fixed with 4% paraformaldehyde for 10min followed by washing with PBS. Then cells were immunostained with anti-FOXO1 or anti-p-FOXO1 antibody (1:100) at 4°C overnight and stained with Alexa Fluor 568-conjugated secondary IgG (1:500, Life Technologies, Carlsbad, CA, USA) for 1h at room temperature. Cells were incubated with DAPI to stain nuclei, and images were acquired with a laser scanning confocal microscope (Olympus FV1000, Japan).

2.12. Transient Transfection with siRNA

When reaching 70% confluence, the U-87 MG cells were transfected with human specific FOXO1 siRNA or a control siRNA at 10 nM by using Lipofectamine 2000 according to the manufacturer’s instruction. After being incubated with siRNA for 8h, cells were washed thrice to remove transfection reagents and then were treated with XHP and incubated for another 24h, followed by cell viability assessment using CCK-8 assay. Knockdown of FOXO1 was confirmed by western blot analysis and Q-PCR.

2.13. Quantitative RT-PCR Analysis

Total RNA was extracted from treated U-87 MG cells using Trizol reagent (Invitrogen, Carlsbad, USA) and was reverse-transcribed into cDNA using a SuperScript™ III First-Strand Synthesis SuperMix (Invitrogen, Carlsbad, USA). The primers’ sequences were as follows: FOXO1 (FP: 5′-TCGTCATAATCTGTCCCTACACA-3′; RP: 5′-CGGCTTCGGCTCTTAGCAAA-3′). Quantitative RT-PCR was performed using SYBR green supermix (Bio-Rad, Hercules, CA, USA) with GAPDH used as endogenous controls in a MX3005P multiplex quantitative qPCR system (Stratagene, California, USA).

2.14. Statistical Analysis

Statistical analysis was performed using GraphPad Prism software 5.0. All data were presented as mean value ± SD. The significance of difference between groups was assessed using Student’s t-test. values < 0.05 were considered to be statistically significant.

3. Results

3.1. Analysis of Compounds in XHP by GC-MS

To get more acquaintance about the active ingredients involved in XHP, GC-MS analysis was applied. It is revealed that total thirty-nine chromatographic peaks were separated well and thirty-two constituents were identified from them (the identified chemical compounds were presented in Table S1). Six compounds, 24-norursa-3,12-diene (17.72%), 24-norursa-3,12-dien-11-one (16.28%), 3,14,15-trihydroxypregn-16-en-20-one (11.77%), isopropyl-1,5,9-trimethyl-15-oxabicyclo[10.2.1] pentadeca-5,9-dien-2-ol (11.40%), 24-noroleana-3,12-diene (8.45%), and 24-norursa-3,9(11),12-triene (5.98%), corresponding to peaks 38, 39, 21, 22, 37, and 36 in the chromatographic spectrum, comprised 71.60% of total amount and could be regarded as the major constituents of XHP (Figure 1).

3.2. XHP Inhibited U-87 MG Cell Growth

To determine the effect of XHP on U-87 MG cell growth, cells were treated with different concentrations of XHP for 24h and CCK-8 assay was performed. It could be found that cell densities were decreased obviously in a dose-dependent manner. XHP-induced cell morphological changes and decreased the viable cell number observed under optical microscope. The IC50 of XHP on U-87 MG cell was 14.60 ± 1.94 μg/mL after 24h treatment ( Figures 2(a) and 2(b)).

3.3. XHP Arrested Cell Cycle of U-87 MG Cell

FACS analysis was conducted to assess the effects of XHP on cell cycle progression. The results showed that after being treated with XHP at 7.5, 15 or 30 μg/mL, the cell accumulation percentage in S-phase was at 16.71 ± 2.18%, 21.32 ± 2.09% ( < 0.05, n = 3) and 38.76 ± 1.95% ( < 0.01, n = 3), compared with 13.53 ± 1.83% in the control group. The cell decreased percentage in G0/G1 phase was at 60.17 ± 1.08%, 51.19 ± 0.53% ( < 0.05, n = 3), and 39.33 ± 0.97% ( < 0.01, n = 3), compared with 63.73 ± 1.16% in the control group (Figure 3). No obvious change was observed in the G2/M phase. The results indicated that XHP could arrest U-87 MG cells in S-phase cell cycle and subsequently block cell growth.

3.4. XHP-Induced Apoptosis of U-87 MG Cells

TUNEL, FACS, and western blot assay were used to detect the apoptosis induced by XHP on U-87 MG cells. As shown in Figure 4(a), the increased DNA fragmentation accompanied with the increase of XHP concentrations was observed after the treatment for 24h with FITC-dUTP and DAPI double staining in the TUNEL assay. Moreover, the proapoptotic ability of XHP was evaluated by FACS. We found that the apoptotic ratio was increased in the XHP-treated group versus the control group in a concentration-dependent manner (Figures 4(b) and 4(c)), and both of the early-period and late-period apoptotic percentage were improved. In particular, the percentage of early-period apoptotic cells with 30 μg/mL of XHP was significantly higher than the untreated control cells from 3.11% to 24.30% ( < 0.01). To confirm the association between XHP treatment and apoptosis, the effects of XHP on the modulation of apoptosis-related proteins were evaluated by western blot analysis. As shown in Figure 4(d), the proapoptotic protein Bax was upregulated and the antiapoptotic protein Bcl-xL was downregulated in a dose-dependent manner. In other words, Bax/Bcl-xL ratio was increased by XHP treatment. In addition, their downstream proteins procaspase-3 and procaspase-9 were also activated by XHP. These findings suggested that XHP might induce apoptosis of U-87 MG cells by upregulating the expression of proapoptotic protein Bax and then subsequently activate its downstream proteins caspase-9 and caspase-3. From results above, it indicated that XHP could decrease the viability of U-87 MG cells, induce cell apoptotic death, and affect apoptotic associated proteins expression.

3.5. XHP-Induced Apoptosis via the ROS-Mediated Mitochondrial-Dependent Pathway

Collapse of mitochondrial membrane potential (ΔΨm) was regarded as a key factor of the mitochondrial-dependent apoptotic pathway. The changes of ΔΨm were detected by JC-1 analysis. As shown in Figures 5(a) and 5(b), the accumulation of monomer improved remarkably in the XHP-treated cells, and J-aggregates decreased at the same time, which suggested that XHP could affect early apoptosis of U-87 MG cells. Furthermore, to investigate whether ROS was involved in the mitochondrial damage, the intracellular H2O2 level was detected by the fluorescent probe DCFH. As shown in Figure 5(c), XHP triggered intracellular ROS release significantly. After using the ROS scavenger NAC, the ROS generation, cell apoptosis, and the oxidative stress induced by XHP were all reversed (Figures 5(c) and 5(d)). Taken together with the above findings, the results suggested that XHP-induced apoptosis might be related to the ROS-mediated mitochondrial-dependent pathway.

3.6. XHP Activated the Akt/mTOR/FOXO1 Signaling Pathway

Accumulating evidence suggested that Akt, mTOR, and FOXO1 played important roles in the proliferation of U-87 MG cells. To investigate the mechanism of the apoptosis induced by XHP, Akt/mTOR/FOXO1 signaling pathway deserved to be evaluated. As shown in Figure 6(a), the phosphorylation of Akt, mTOR, and FOXO1 was downregulated after treatment with different concentrations of XHP, while FOXO1 expression was significantly increased under the same manner. As a transcription factor, the nuclear localization of FOXO1 defined its role in the regulation of downstream targets. In this experiment, the distribution of FOXO1 between nuclear and cytosolic compartments was studied by immunofluorescent imaging. It was observed that FOXO1 accumulation and p-FOXO1 reduction in nuclei were synchronous in XHP-stressed U-87 MG cells (Figures 6(c) and 6(d)). Besides, it was also found that the proapoptotic effect of XHP on Akt/mTOR/FOXO1 signaling pathway could be reversed by NAC (Figure 6(b)). Moreover, Akt inhibitor LY294002, mTOR inhibitor rapamycin, and FOXO1-specific siRNA were adopted to verify the roles of Akt, mTOR, and FOXO1 in the apoptotic process. After being treated with LY294002 or rapamycin, the sensitivity of U-87 MG cells to XHP and the apoptotic cells were all increased, yet the inactivation of FOXO1 by siRNA attenuated the sensitivity of U-87 MG cells to XHP (Figure 6(g)). Consequently, it is suggested that XHP could inhibit the Akt/mTOR/FOXO1 pathway to exert its antiglioblastoma effect.

4. Discussion

XHP, a representative traditional Chinese medicine formula for clearing heat and relieving toxin, shows remarkable antineoplastic properties against several cancers including glioma in clinical practice. However, its pharmacological activity and underlying mechanism on glioblastoma have not been well studied until now. Herein, human U-87 MG cells were used as an experimental model to examine its antiglioma effects. Our findings preliminary demonstrated that XHP could inhibit U-87 MG cells proliferation and induce apoptosis via mitochondrial damage and inhibition of ROS-mediated Akt/mTOR/FOXO1 signal pathway.

Apoptosis is a vital mechanism to balance cell proliferation and death. In our study, after being treated with XHP, apoptosis-related morphology changes in cells, such as cell shrinkage, chromatic agglutination, and nuclear fragmentation, were observed. Many reports showed that apoptosis often occurred with cell cycle arrest in G1 or G2/M phase via interfering with the particular cyclins [23, 24]. However, cells were found to be blocked from G1 to S-phase in our study. This result was in agreement with the previous reports on XHP treatments in human hepatocellular carcinoma BEL-7404 cells and human ovary carcinoma Sk-OV-3 cells [25, 26]. It could be presumed that XHP might impact DNA synthesis and/or a certain cyclin that regulated S-phase [27, 28].

Bcl-2 family proteins regulate mitochondria-dependent apoptosis by controlling mitochondrial permeability and the release of cytochrome c (Cyt c) [29, 30], with the balance of anti- and proapoptotic members arbitrating cell fate. Antiapoptotic proteins Bcl-2 and Bcl-xL reside in the outer mitochondrial wall and inhibit Cyt c release. Proapoptotic Bcl-2 proteins such as Bad (Bcl-xL/Bcl-2 associated death promoter), Bid (BH3 interacting agonist), Bax and Bim (Bcl-2 interacting mediator of cell death) reside in the cytosol but translocate to mitochondria following death signaling, where they could promote the release of Cyt c. Activated Bad, an essential initiator of the apoptotic cascade, translocates to mitochondria and forms a proapoptotic complex with the antiapoptotic mitochondrial proteins Bcl-2 and Bcl-xL, as well as to antagonize their antiapoptotic activity and promote the proapoptotic activity of Bax [3133]. Bax and Bim translocate to mitochondria in response to death stimuli including survival factor withdrawal, activated following DNA damage, inducing transcription of Bax. Bax translocates to the outer mitochondrial membrane through BH3 and multimerizates, which forms membrane channels to stimulate the release of mitochondrial Cyt c and apoptosis-inducing factor (AIF). Released Cyt c binds apoptotic protease-activating factor 1 (Apaf1) and forms activated apoptotic bodies with caspase-9, leading to a cascade of downstream caspase reaction [34, 35]. Although the mechanism(s) regulating mitochondrial permeability and the release of Cyt c during apoptosis are not totally understood, Bcl-xL and Bax apparently influence the release of Cyt c [33, 36]. In this study, we observed that XHP-induced apoptosis in U-87 MG cells from Annexin V/PI staining and DNA fragmentation (Figures 4 and 5). The appeared mitochondrial dysfunction detected by JC-1 assay confirmed that the U-87 MG cell apoptosis occurred via mitochondria-dependent pathway. In addition, oxidative imbalance was accompanied with the decreased mitochondrial membrane potential. As is well known, increased intracellular ROS level plays a critical role in mitochondria-dependent apoptotic pathway [37, 38]. Excessive ROS could cause dysfunction of the mitochondrial membrane proteins and collapse of mitochondrial membrane potential. Application of NAC, the ROS inhibitor, could usually alleviate oxidative stress and reduce ROS generation, as well as the ratio of apoptosis. In our study, after being pretreated with XHP, rapid ROS generation and relief by NAC were observed (Figure 5). It is implied that XHP-induced apoptosis was at least partly depending on ROS generation. Furthermore, it was found that XHP significantly alter Bax and Bcl-xL levels in U-87 MG cells, increase the Bax/Bcl-xL ratio, and decline of the precursor forms of caspase-9 and caspase-3. Further investigation might be needed to clarify whether XHP affects other Bcl-2 family members such as Bim, Bad, and BH3-only proteins in U-87 MG cells.

It is clear that the clinical significance of Akt and mTOR are crucial in GBM. Both of them can be used as markers to predict prognosis and target candidates for personalized medicine [3942]. Their activation promotes cell proliferation, regulates cellular energy metabolism, and provides protection from apoptosis. PI3K/Akt/mTOR pathway emerges as a potential treatment for GBM patients. FOXOs, comprising FOXO1, FOXO3, FOXO4, and FOXO6, are the focus of cancer research recently [43, 44]. FOXOs have emerged as tumor suppressors via inhibiting PI3K/Akt signaling pathway, which can be phosphorylated at various serine and threonine residues (S253, S315 and Thr32) by activated Akt. Once phosphorylation accomplished, FOXOs are exported from nucleus to cytoplasm and become inactive, which leads to inhibition of transcriptional activity [45]. Therefore, nuclear localization of FOXOs is required for their transcriptional regulatory functions, such as cell proliferation, differentiation, cell cycle regulation, protection from oxidative stress, and apoptosis [46]. In this study, we attempted to investigate whether XHP exerted U-87 MG cells apoptosis by regulating the above-mentioned signaling pathways.

From western blot results, we found that XHP could inhibit the phosphorylation of the key protein members in PI3K/Akt pathway, including p-Akt (Ser473), p-mTOR (Ser2448), and p-FOXO1 (Thr24), and upregulate total FOXO1 expression in U-87 MG cells (Figure 6). This result coincided well with the enhancement in nuclear localization and the potentiated cytoplasmic degradation of FOXO1 observed in immunofluorescence images. Activation of FOXO1 subsequently led to transcriptional activation of genes controlling cell cycle arrest or cell apoptosis, such as proapoptotic proteins [47]. We verified in this study that their ability of permeabilizing mitochondrial membrane could result in activation of executioner caspases such as caspase-9, caspase-3, and pinnacle of cell death [48]. Moreover, we found that synergetic effects occurred when XHP was combined with either Akt or mTOR inhibitors. Inhibition of Akt or mTOR can increase the cytotoxic and apoptotic effects of XHP, while FOXO1 knockdown could rescue U-87 MG cells from XHP-induced apoptosis. From above, it was obvious that the PI3K pathway proteins including Akt, mTOR, and FOXO1 are involved in XHP-induced apoptosis followed by the enhanced downstream proapoptotic target FOXO1’s nuclear import. The activation of the dephosphorylated FOXO1 potentiated proapoptotic protein Bax expression and oxidative stress generation, which induced mitochondria-mediated activation of apoptotic cascade. Therefore, based on literature and our preliminary results, we hypothesized that XHP might inhibit glioblastoma cells apoptosis resistance by inducing Akt and mTOR dephosphorylation, decreasing phosphorylation of FOXO1, causing FOXO1 nuclear transport and enhancing its transcriptional activity, and finally triggering U-87 MG cell apoptosis.

5. Conclusion

The present study provided a consideration that XHP regulated glioblastoma cell apoptosis through suppressing Akt/mTOR/FOXO1 signaling cascade. This research might be helpful in understanding the mechanisms related to XHP against GBM.

Data Availability

All relevant data are included within the article.

Conflicts of Interest

The authors declare that they have no conflicts of interest.

Authors’ Contributions

Meng Shao and Zhenqiang He contributed equally to this study.

Acknowledgments

This study was financially supported by Natural Science Foundation of Guangdong Province (no. 2017A030313772), Administration of Traditional Chinese Medicine of Guangdong Province (nos. 20181167 and 20181169), and Technology Research and Development Project of Guangdong Province (no. 2017A020215036).

Supplementary Materials

Supplementary 1. Table S1: Compounds identified by GC-MS analysis.

Supplementary 2. Figure S1: The total ion chromatogram of XHP obtained from GC-MS analysis.

References

  1. A. Perry and P. Wesseling, “Histologic classification of gliomas,” Handbook of Clinical Neurology, vol. 134, pp. 71–95, 2016. View at: Publisher Site | Google Scholar
  2. D. N. Louis, A. Perry, G. Reifenberger et al., “The 2016 world health organization classification of tumors of the central nervous system: a summary,” Acta Neuropathologica, vol. 131, no. 6, pp. 803–820, 2016. View at: Publisher Site | Google Scholar
  3. D. Schiff, K. A. Jaeckle, S. K. Anderson et al., “Phase 1/2 trial of temsirolimus and sorafenib in the treatment of patients with recurrent glioblastoma: North Central Cancer Treatment Group Study/Alliance N0572,” Cancer, vol. 124, no. 7, pp. 1455–1463, 2018. View at: Publisher Site | Google Scholar
  4. Q. Guo, J. Lin, R. Liu et al., “Review on the applications and molecular mechanisms of xihuang pill in tumor treatment,” Evidence-Based Complementary and Alternative Medicine, vol. 2015, Article ID 854307, 10 pages, 2015. View at: Publisher Site | Google Scholar
  5. G. Pan, W. Wang, L. Wang et al., “Anti-breast cancer effects and mechanisms of Xihuang pill on human breast cancer cell lines,” Journal of Traditional Chinese Medicine, vol. 33, no. 6, pp. 770–778, 2013. View at: Publisher Site | Google Scholar
  6. X. L. Sang and G. Y. Liu, “Effect of Xihuang Pill on curative effect of paclitaxel combined with platinum based neoadjuvant chemotherapy in patients with advanced cervical cancer after operation,” Drug Evaluation Research, vol. 40, no. 8, pp. 1112–1116, 2017. View at: Google Scholar
  7. Y. P. Fan, “1 case of brain stem glioma treated by syndrome differentiation of TCM and Xihuangwan,” Journal of Traditional Chinese Medicine and Pharmacy, vol. 25, no. 2, pp. 245–248, 2010. View at: Google Scholar
  8. D. Yu and G. Y. An, “Clinical effects of Xihuang pill combined with chemotherapy in patients with advanced colorectal cancer,” Evidence-Based Complementary and Alternative Medicine, vol. 2017, Article ID 5936086, pp. 1–5, 2017. View at: Publisher Site | Google Scholar
  9. L. Y. Wang, H. F. Li, Q. Zu, H. G. Xiao, and Y. Y. Dang, “Sixty patients with Non-Hodgkin's Lymphoma treated with Xihuang Pill and CHOP Chemotherapy combination therapy,” Journal of Shandong University of Traditional Chinese Medicine, vol. 36, no. 4, pp. 313–315, 2012. View at: Google Scholar
  10. X. T. Chen, X.-Y. Ge, L. Bin, W. Yan, W. Jin, and J. Q. Li, “Xihuang Pills drug serum on the apoptosis of SW480 human colorectal cancer cells and the protein expression of Bcl-2, Bax,” China Journal of Traditional Chinese Medicine and Pharmacy, vol. 30, no. 2, pp. 507–509, 2015. View at: Google Scholar
  11. H. Xu, L. R. Cui, and J. C. Liu, “Study on the effects of Xihuang pill on the expression of bcl-2 mRNA of mice bearing H22,” Modern Preventive Medicine, vol. 38, no. 11, pp. 2120-2121, 2011. View at: Google Scholar
  12. Y. H. Duo, L. N. Sun, S. L. Ying, and J. Y. Meng, “Effects of Xihuang Pill on the growth of human colorectal cancer cell xenografts in nude mice through the ERK/MAPK pathway,” China Journal of Traditional Chinese Medicine and Pharmacy, vol. 28, no. 10, pp. 3055–3058, 2013. View at: Google Scholar
  13. H. Xiao, X. H. Qin, S. R. Jin, P. Mm, and L. Lai, “The mechanism of Xihuang Pill regulating the growth of the lung cancer stem cells by controlling ß-catenin of Wnt pathway,” Pharmacology and Clinics of Chinese MateriaMedica, vol. 30, no. 2, pp. 21–23, 2014. View at: Google Scholar
  14. W. Zheng, S. Han, S. Jiang et al., “Multiple effects of Xihuang pill aqueous extract on the Hs578T triple-negative breast cancer cell line,” Biomedical Reports, vol. 5, no. 5, pp. 559–566, 2016. View at: Publisher Site | Google Scholar
  15. S. R. Jin, B. D. Zhu, X. H. Qin, and H. L. Chen, “Effects of xihuang pill on cell cycles of human hepatoma carcinoma cell strain (SMMC7721) and mouse uterine cervix cancer(U14),” Li Shi Zhen Medicine and Material Medica Research, vol. 18, no. 11, pp. 2782-2783, 2007. View at: Google Scholar
  16. M. Wang, J.-Y. Meng, and S.-F. He, “Xihuang Pill induces mesenchymal-epithelial transition and inhibits loss of apical-basal polarity in colorectal cancer cell through regulating ZEB1-SCRIB loop,” Chinese Journal of Integrative Medicine, vol. 20, no. 10, pp. 751–757, 2014. View at: Publisher Site | Google Scholar
  17. L. N. Sun, J. Y. Meng, W. Wang et al., “Effect of Xihuang pills on protein expressions of MMP-2 and MMP-9 in human colorectal carcinoma LoVo cell,” Tianjin Journal of Traditional Chinese Medicine, vol. 29, no. 4, pp. 378–380, 2012. View at: Google Scholar
  18. Q. Guo, Exploration on the Mechanism of Xihuang Pill in Anti-Proliferation and Inhibition of Vasculogenic Mimicy Formation of Gastric Cancer, Beijing University of Chinese Medicine, Beijing, China, 2017.
  19. Y. Y. Wang, Y. Z. Ren, Z. Jiao, C. Q. Zeng, W. B. Gao, and W. B. Liang, “The influence of Xihuang Pill (西) on the formation of con tumor-bearing mice,” Pharmacology and Clinics of Chinese Materia Medica, vol. 30, no. 4, pp. 11–13, 2014. View at: Google Scholar
  20. W. Yang, S. Guan, J. X. Hu et al., “Antitumor activity of Xihuang Pill and its regulatory role of inflammatory cytokines,” Drugs & Clinic, vol. 28, no. 6, pp. 847–850, 2013. View at: Google Scholar
  21. Z. H. Wang, Z. X. Wang, C. Liu et al., “Xihuangwan dripping pill's anti-tumor function and its effect on immunity,” Journal Of Shandong University (Health Sciences), vol. 51, no. 4, pp. 18–20, 2013. View at: Google Scholar
  22. J. Jin and Z. H. Li, “Integrated Xihuang Pill and chemotherapy in treating 30 patients with breast cancer,” China Journal of Traditional Chinese Medicine and Pharmacy, vol. 25, no. 5, pp. 715-716, 2010. View at: Google Scholar
  23. S.-Y. Xi, Y.-H. Teng, Y. Chen et al., “Jianpi Huayu Decoction inhibits proliferation in human colorectal cancer cells (SW480) by inducing G0/G1-phase cell cycle arrest and apoptosis,” Evidence-Based Complementary and Alternative Medicine, vol. 2015, Article ID 236506, 8 pages, 2015. View at: Publisher Site | Google Scholar
  24. C.-J. Yao, J.-M. Chow, C.-M. Yang et al., “Chinese herbal mixture, Tien-Hsien liquid, induces G2/M cycle arrest and radiosensitivity in MCF-7 human breast cancer cells through mechanisms involving DNMT1 and Rad51 downregulation,” Evidence-Based Complementary and Alternative Medicine, vol. 2016, Article ID 3251046, pp. 1–13, 2016. View at: Publisher Site | Google Scholar
  25. Y. Xiong, X. Y. Kong, and R. S. Chen, “Experimental study on the effect of xihuang pill drug serum on the growth and cell cycle of human hepatic carcinoma cells,” Chinese Journal of Traditional Medical Science and Technology, vol. 8, no. 4, pp. 217–219, 2001. View at: Google Scholar
  26. F. Y. Xing, The Effects of Xihuang Pill Drug Serum on Human Breast Carcinoma Cells and Human Ovary Carcinoma Cells (SK-OV-3), Xun Cui, Yanbian University, Yanji, China, 2007.
  27. C. B. De Araujo, L. C. Russo, L. M. Castro et al., “A novel intracellular peptide derived from G1/S cyclin D2 induces cell death,” The Journal of Biological Chemistry, vol. 289, no. 24, pp. 16711–16726, 2014. View at: Publisher Site | Google Scholar
  28. S.-T. Yang, A.-C. Huang, N.-Y. Tang et al., “Bisdemethoxycurcumin-induced S phase arrest through the inhibition of cyclin A and E and induction of apoptosis via endoplasmic reticulum stress and mitochondria-dependent pathways in human lung cancer NCI H460 cells,” Environmental Toxicology, vol. 31, no. 12, pp. 1899–1908, 2016. View at: Publisher Site | Google Scholar
  29. A. P. G. Dingeldein, Š. Pokorná, M. Lidman et al., “Apoptotic bax at oxidatively stressed mitochondrial membranes: Lipid dynamics and permeabilization,” Biophysical Journal, vol. 112, no. 10, pp. 2147–2158, 2017. View at: Publisher Site | Google Scholar
  30. R. Roufayel, “Regulation of stressed-induced cell death by the Bcl-2 family of apoptotic proteins,” Molecular Membrane Biology, vol. 33, no. 6-8, pp. 89–99, 2016. View at: Publisher Site | Google Scholar
  31. T. T. Renault, R. Elkholi, A. Bharti, and J. E. Chipuk, “B cell lymphoma-2 (BCL-2) homology domain 3 (BH3) mimetics demonstrate differential activities dependent upon the functional repertoire of pro- and anti-apoptotic BCL-2 family proteins,” The Journal of Biological Chemistry, vol. 289, no. 38, pp. 26481–26491, 2014. View at: Publisher Site | Google Scholar
  32. S.-Y. Jeong, B. Gaume, Y.-J. Lee et al., “Bcl-xL sequesters its C-terminal membrane anchor in soluble, cytosolic homodimers,” EMBO Journal, vol. 23, no. 10, pp. 2146–2155, 2004. View at: Publisher Site | Google Scholar
  33. D. Garenne, T. T. Renault, and S. Manon, “Bax mitochondrial relocation is linked to its phosphorylation and its interaction with Bcl-xL,” Microbial Cell, vol. 3, no. 12, pp. 597–605, 2016. View at: Publisher Site | Google Scholar
  34. Z. Y. Jiang, H. S. Zhang, and R. A. Bockmann, “Allostery in BAX protein activation,” Journal of Biomolecular Structure & Dynamics, vol. 34, no. 11, pp. 2469–2480, 2016. View at: Publisher Site | Google Scholar
  35. N. Joza, S. A. Susin, E. Daugas et al., “Essential role of the mitochondrial apoptosis-inducing factor in programmed cell death,” Nature, vol. 410, no. 6828, pp. 549–554, 2001. View at: Publisher Site | Google Scholar
  36. M. C. Wei, W. X. Zong, E. H. Y. Cheng et al., “Proapoptotic BAX and BAK: a requisite gateway to mitochondrial dysfunction and death,” Science, vol. 292, no. 5517, pp. 727–730, 2001. View at: Publisher Site | Google Scholar
  37. E. Zamani, F. Shaki, S. AbedianKenari, and M. Shokrzadeh, “Acrylamide induces immunotoxicity through reactive oxygen species production and caspase-dependent apoptosis in mice splenocytes via the mitochondria-dependent signaling pathways,” Biomedicine & Pharmacotherapy, vol. 94, pp. 523–530, 2017. View at: Publisher Site | Google Scholar
  38. L.-H. Shang, C.-M. Li, Z.-Y. Yang, D.-H. Che, J.-Y. Cao, and Y. Yu, “Luffa echinata Roxb. induces human colon cancer cell (HT-29) death by triggering the mitochondrial apoptosis pathway,” Molecules, vol. 17, no. 5, pp. 5780–5794, 2012. View at: Publisher Site | Google Scholar
  39. A. W. Alvarenga, L. E. Machado, B. R. Rodrigues et al., “Evaluation of Akt and RICTOR expression levels in astrocytomas of all grades,” Journal of Histochemistry & Cytochemistry, vol. 65, no. 2, pp. 93–103, 2017. View at: Publisher Site | Google Scholar
  40. M. J. Riemenschneider, R. A. Betensky, S. M. Pasedag, and D. N. Louis, “AKT activation in human glioblastomas enhances proliferation via TSC2 and S6 kinase signaling,” Cancer Research, vol. 66, no. 11, pp. 5618–5623, 2006. View at: Publisher Site | Google Scholar
  41. D. A. Guertin and D. M. Sabatini, “Defining the role of mTOR in cancer,” Cancer Cell, vol. 12, no. 1, pp. 9–22, 2007. View at: Publisher Site | Google Scholar
  42. M. Liu, Y. Lin, X.-C. Zhang et al., “Phosphorylated mTOR and YAP serve as prognostic markers and therapeutic targets in gliomas,” Laboratory Investigation, vol. 97, no. 11, pp. 1354–1363, 2017. View at: Publisher Site | Google Scholar
  43. Y. Wang, Y. Zhou, and D. T. Graves, “FOXO transcription factors: their clinical significance and regulation,” BioMed Research International, vol. 2014, Article ID 925350, 13 pages, 2014. View at: Publisher Site | Google Scholar
  44. C. J. Lau, Z. Koty, and J. Nalbantoglu, “Differential response of glioma cells to FOXO1-directed therapy,” Cancer Research, vol. 69, no. 13, pp. 5433–5440, 2009. View at: Publisher Site | Google Scholar
  45. A. Brunet, A. Bonni, M. J. Zigmond et al., “Akt promotes cell survival by phosphorylating and inhibiting a forkhead transcription factor,” Cell, vol. 96, no. 6, pp. 857–868, 1999. View at: Publisher Site | Google Scholar
  46. J. J. Brosens, M. S. Wilson, and E. W. Lam, “FOXO transcription factors: From cell fate decisions to regulation of human female reproduction,” in Forkhead Transcription Factors, vol. 665 of Advances in Experimental Medicine and Biology, pp. 227–241, Springer New York, New York, NY, USA, 2009. View at: Publisher Site | Google Scholar
  47. M. Moeinifard, Z. M. Hassan, F. Fallahian, M. Hamzeloo-Moghadam, and M. Taghikhani, “Britannin induces apoptosis through AKT-FOXO1 pathway in human pancreatic cancer cells,” Biomedicine & Pharmacotherapy, vol. 94, pp. 1101–1110, 2017. View at: Publisher Site | Google Scholar
  48. J. Li, L. Zhao, X. Zhao, P. Wang, Y. Liu, and J. Ruan, “Foxo1 attenuates NaF-induced apoptosis of LS8 cells through the JNK and mitochondrial pathways,” Biological Trace Element Research, vol. 181, no. 1, pp. 104–111, 2018. View at: Publisher Site | Google Scholar

Copyright © 2018 Meng Shao et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.


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