Induction of selective cytotoxicity and apoptosis in human T4-lymphoblastoid cell line (CEMss) by boesenbergin a isolated from boesenbergia rotunda rhizomes involves mitochondrial pathway, activation of caspase 3 and G2/M phase cell cycle arrest
© NG et al.; licensee BioMed Central Ltd. 2013
Received: 14 October 2012
Accepted: 14 February 2013
Published: 22 February 2013
Boesenbergia rotunda (Roxb.) Schlecht (family zingiberaceae) is a rhizomatous herb that is distributed from north-eastern India to south-east Asia, especially in Indonesia, Thailand and Malaysia. Previous research has shown that the crude extract of this plant has cytotoxic properties. The current study examines the cytotoxic properties of boesenbergin A isolated from Boesenbergia rotunda.
MTT assay was used to check the cytotoxicity of boesenbergin A. The morphological assessment of apoptosis was monitored using normal and fluorescence microscopy. The early and late phase of apoptosis was investigated using annexin V and DNA laddering assays, respectively. The mitochondrial membrane potential (MMP) was assessed by fluorescence microscopy. Human apoptosis proteome profiler assays were performed to investigate the mechanism of cell death. In addition, the protein levels of Bax, Bcl2 and HSP 70 were also analyzed using western blot. Assays of caspase =-3/7, -8 and =-9 were carried out in order to test for induction during treatment. Lastly, cell cycle progression was analyzed using flow cytometry.
Boesenbergin A was found to have the highest toxicity towards CEMss cancer cells (IC50 = 8 μg/ml). The morphology of CEMss cells after treatment showed evidence of apoptosis that included blebbing and chromatin condensation. The annexin V assay revealed that early apoptosis is induced after treatment. The DNA laddering assay confirmed that DNA fragmentation had occurred during late apoptosis. The cell cycle analysis indicated that boesenbergin A was able to induce G2/M phase arrest in CEMss cells. The activity of caspases -3/7, -8 and -9 was increased after treatment which indicates both intrinsic and extrinsic pathways are induced during apoptosis. The involvement of mitochondria was established by increased mitochondrial membrane potential and up and down regulation of Bcl2 and Bax proteins as well as HSP70.
In conclusion, the results demonstrated that boesenbergin A induced apoptosis of CEMss cells through Bcl2/Bax signaling pathways with the involvement of caspases and G2/M phase cell cycle arrest. The current findings warrant further research on boesenbergin A as a novel chemotherapeutic agent for leukemia intervention including studies in animal models.
KeywordsBoesenbergia rotunda Boesenbergin A CEMss Anticancer Cytotoxicity
Leukemia is a cancer of blood-forming organs, such as bone marrow, which is characterized by the uncontrolled proliferation of abnormal blood cells. In a national childhood cancer survey carried out in Malaysia, it was found that leukemia is the commonest childhood tumor. The crude incidence rate of pediatric malignancies in Malaysia was 77.4 per million children aged less than 15 years with leukemia as the fourth leading cause of cancer related death in 1998.
There are about 20,000 species of tropical plants, of which about 1,300 are said to be medicinal and potential sources for screening of anticancer agents. Some of the plant extracts from these medicinal plants are reported to have potential to be developed as drugs. Boesenbergia rotunda (L.) (Fingerroot), formerly known as Boesenbergia or Kaempferia pandurata (Roxb). Schltr. (Zingiberaceae), is distributed in south-east Asian countries, such as Indonesia, Malaysia and Thailand. The rhizomes of this plant have been used for the treatment of peptic ulcer, as well as colic, oral diseases, urinary disorders, dysentery and inflammation. Several studies have suggested this plant to be neuroprotective and to show anti-inflammatory, anti-mutagenic, anticancer, chemopreventive, anti-dermatophytic, anti-Helicobacter pylori and anti-dengue-2 virus NS3 protease activity. This plant possesses both anti-oxidant, as well as anticancer properties which can help to cure cancer.
The rhizomes of B. rotunda were purchased from Puchong Market, Selangor Darul Ehsan, Malaysia. The material was identified by a botanist at the Faculty of Science, University Putra Malaysia, where a voucher specimen was deposited (BR-R11-01). The isolation and identification of boesenbergin A has been previously reported by us in detail.
Cell culture conditions
Estrogen receptor positive cells (MCF-7) and cervical cancer cells (Hela) were obtained from ATCC (USA). Human T4-lymphoblastoid cell line CEMss were obtained from NIH AIDS Research and Reference Reagent Program (Division of AIDS, NIAID, NIH: USA). The cell lines were grown at 37°C in a humidified CO2 incubator with 5% CO2 in RPMI-1640 (Sigma, MO, USA) supplemented with 10% fetal bovine serum (Invitrogen Corp., Auckland, N.Z.).
Adherent cells (1× 106 cells/ml) were grown in 96-well plates overnight, whereas CEMss cells (1× 106 cells/ml) were plated directly into 96-well plates on the drug treatment day. Boesenbergin A was dissolved in dimethylsulfoxide (DMSO) and media. The final concentration of DMSO was 0.1% (v/v). Different concentrations of the sample were prepared with serial dilution. Dimethylsulfoxide (0.1%) was used as a control. The toxicity profiles of the compound were assessed using the 3-[4,5-dimethylthiazol-2-yl]-2,5-diphenyltetrazolium bromide (MTT) microculture tetrazolium viability assay as described previously. Thereafter, various concentrations of compound (with a maximum of 100 μg/ml) were plated out in triplicate. Each plate included untreated cell controls and a blank cell-free control. After 72 h of incubation, MTT (5 mg/ml) was added to each well and the plates incubated for a further 4 h before removal of the media. DMSO was then added into each well to solubilize the formazan crystals. The absorbance was read at wavelength of 595 nm using a microtitre plate reader (Labsystems iEMS Reader MF). The percentage cellular viability was calculated with the appropriate controls taken into account. The concentration which inhibited 50% of cellular growth (IC50 value) was determined. All experiments were carried out in triplicate (Figure 1B).
The inhibitory rate of cell proliferation was calculated by the following formula: Growth inhibition = (OD control – OD treated) / OD control X 100. The cytotoxicity of sample on cancer cells was expressed as IC50 values (the drug concentration reducing the absorbance of treated cells by 50% with respect to untreated cells). The determined IC50 value was used for many of the subsequent experiments.
Cytotoxicity of boesenbergin A on proliferated primary human blood lymphocytes
The ability of boesenbergin A to act selectively on cancer cells especially leukemia was evaluated by comparing the cytotoxicity of this compound towards primary human blood lymphocytes. Briefly, blood was collected into a cell preparation tube containing sodium citrate (BD Vacutainer®, New Jersey, USA). After collection, tube was stood upright for 20 min at room temperature to allow it to equilibrate and was then centrifuged at 1200xg for 20 min. Mononuclear cells and platelets underneath the plasma layer were collected using a pipette and transferred into a 15 ml centrifuge tube. The cells were washed twice with PBS and cultured in complete Quantum PBL media with phytohemagglutinin (PAA, Pasching, Austria) containing 10% FBS supplemented with 100 U/ml penicillin and 100 μg/ml streptomycin at 37°C in 5% CO2 atmosphere. Primary human blood lymphocytes (1 × 106 cells/ml) were treated at various concentrations of boesenbergin A in triplicate and cell viability was measured using MTT assay after 48 h of incubation. The cell lines used as normal cells were human peripheral blood lymphocytes obtained from normal healthy donors after informed consent was given. This project was approved by the medical research ethics committee (founded in 2002) of the medical Faculty of UPM at a meeting on April 12, 2012 (UPM 2564/004/12).
Microscopic observation of cellular morphology using phase contrast inverted microscope
This analysis examined whether apoptosis may be implicated in mediating cell death amongst CEMss cells elicited by boesenbergin A. CEMss cells at a concentration of 1 × 106 cells/ml were cultured in RPMI 1640 (PAA, Cölbe, Germany) medium containing 10% FBS was seeded into a 25 ml culture flask (TPP, Trasadingen, Switzerland) and treated with boesenbergin A (8 μg/ml) at different time periods (24, 48 and 72 h). The morphological appearance of treated cells was compared with the untreated control by using a normal inverted microscope post-treatment. CEMss cells were treated with the compound for 24, 48 and 72 h. Untreated cells served as the negative control.
Quantification of apoptosis using propidium iodide and acridine orange double staining
Boesenbergin A-induced cell death in CEMss cells was quantified using propidium iodide (PI) and acridine orange (AO) double staining according to standard procedures and examined under a fluorescence microscope (Lieca attached with Q-Floro Software). Briefly, treatment was carried out in a 25 ml culture flask (Nunc). CEMss cells were plated at a concentration of 1 × 106 cells/ml and treated with boesenbergin A (8 μg/ml). The cells were incubated in 5% CO2 atmosphere at 37°C for 24, 48 and 72 h and then spun down at 200 g for 10 min. The supernatant was discarded and the cells were washed twice using PBS after centrifuging at 200 g for 10 min to remove the remaining media. Ten microliters of fluorescent dyes containing AO (10 μg/ml) and PI (10 μg/ml) were added into the cellular pellet at equal volumes of each. The freshly stained cell suspension was dropped into a glass slide and covered by cover slip. Slides were observed under a UV-fluorescence microscope within 30 min before the fluorescence colour started to fade. The percentages of viable, early apoptotic, late apoptotic and secondary necrotic cells were determined in more than 200 cells. Acridine orange (AO) and propidium iodide (PI) are intercalating nucleic acid specific fluorochromes which emit green and orange fluorescences respectively, when they are bound to DNA. Of the two, only AO can cross the plasma membrane of viable and early apoptotic cells. The criteria for identification are as follows: (a) viable cells appear to have a green nucleus with an intact structure; (b) early apoptotic cells exhibit a bright-green nucleus showing condensation of chromatin in the nucleus; (c) late apoptotic cells show dense orange areas of chromatin condensation; (d) secondary necrotic cells appear to have an orange intact nucleus. This assay provides a useful quantitative evaluation and was carried out in triplicate.
Flow cytometric analysis of DNA cell cycle
CEMss cells at concentration of 1 × 106 cells/ml were cultured in RPMI 1640 (PAA) medium containing 10% FBS seeded in to 25 ml culture flask (TPP) and treated with boesenbergin A (8 μg/ml) at different time periods (24, 48 and 72 h). After incubation, the cells were spun down by centrifugation at 200 g for 10 min. The supernatant was discarded and the pellet was washed with PBS twice to remove any remaining media. To restore the integrity, fixation of the cell population for flow cytometery analysis was performed. Briefly, cell pellets were fixed by mixing 500 μl of 70% cold ethanol and 250 μl of cell suspension and kept at −20°C overnight. The cells were then spun down at 200 g for 10 min and the ethanol was decanted. After washing twice with PBS, the cells were resuspended in PBS. Twenty microliters of RNase A (10 μg/ml) and 2 μl of PI (2.5 μg/ml) were added and the fixed cells were kept in the dark on ice for 30 min. Propidium iodide has the ability to bind to RNA molecules and hence RNase enzyme was added in order to allow PI to bind directly to DNA. The DNA content of cells was then analyzed using a flow cytometer (BD FACSCanto™ II). The fluorescence intensity of the subG1 cell fraction represents the apoptotic cell population.
Annexin V assay
CEMss cells (1 × 106 cells/ml) were exposed to boesenbergin A (8 μg/ml) for 24, 48 and 72 h and the annexin V assay performed using an annexin V:FITC assay kit (ABD Serotec, UK). Briefly the treated cells were centrifuged for 10 min at 200 g to remove the media. After that, PBS was added to wash the cells and the same process was repeated twice. Then 5 μl annexin V:FITC was added to 195 μl of the cell suspension binding buffer, which was prepared by diluting the binding buffer 1:4 in distilled water (50 ml binding buffer +150 ml distilled water). The suspension was then mixed and incubated for 10 min in the dark at room temperature. The cells were then washed and resuspended in 190 μl prediluted binding buffer. Then 10 μl of the PI solution was added to the cell suspension and the sample was analyzed using a flow cytometer (BD FACSCanto™ II).
The Apoptotic DNA Ladder Detection kit (CHEMICON International Inc., CA, USA) was used for DNA extraction from cells. Briefly, CEMss cells treated with boesenbergin A (16 μg/ml) were collected at 24 and 48 h post treatment. The cells were washed with PBS and the cells were spun down by centrifugation at 500 × g for 5 min. After removal of the supernatant, the cells were lysed by the addition of 40 μl of TE lysis buffer and gentle pipetting, followed by the addition of 5 μl of Enzyme A (RNase A) into the crude lysate and incubated at 37°C for 10 min. Then 5 μl of Enzyme B (Proteinase K) was added and the lysate was further incubated at 50°C for 30 min. Then 5 μl of ammonium acetate solution and 50 μl of isopropanol were added and mixed well and the suspension was kept at −20°C for 10 min. The sample was then centrifuged 16000 × g for 10 min at to precipitate the DNA. After washing the DNA pellet with 70% ice cold ethanol, the air dried pellet was dissolved in 30 μl of DNA suspension buffer. For detecting the DNA ladder, the extracted DNA samples were run on 1% agarose gel in tris–acetic acid–EDTA buffer. After electrophoresis, the gel was stained with ethidium bromide (Gibco BRL, Paisley, Scotland), visualized with a UV light transilluminator (UVP, Upland, CA, USA) and photographed.
Caspase-3/7, -8 and -9 activity assay
Assays of caspase-3/7, -8 and =-9 was performed using the Caspase-Glo Assay kit (Promega, WI, USA). CEMss cells were plated and treated with boesenbergin A (8 μg/ml) and incubated for 24, 48 and 72 h in 96 well white plates. After allowing the cells to equilibriate at room temperature, 50 μl of Caspase-Glo® reagent was added to each well containing 50 μl of blank, negative control cells and treated cells in culture medium. The contents of the plate were gently mixed using a plate shaker at 100 g for 30 sec. It was then incubated at room temperature for 30 min in the dark. Readings were taken every 10 min for 3 h using a luminescence microplate reader (Infinite M200PRO, Tecan, Männedorf, Switzerland).
Detection of mitochondrial membrane potential (Δψm)
Rhodamine 123 (Rh123) is a fluorescent cationic dye that binds to polarized mitochondrial membrane and accumulates as aggregates in the mitochondria of normal cells. Rh123 was prepared in ethanol as a 5 mg/ml stock solution. CEMss cells were treated with 8 μg/ml boesenbergin A for 24, 48 and 72 h. At the end of the reaction time, the cells were harvested and washed twice in cold PBS, then resuspended in Rh123 (2 μg/ml) for 30 min in the dark. The Rh123 staining intensity was captured using a fluorescence microscope. Intensity of Rh 123 is directly related to mitochondrial membrane potential. The percentage of rhodamine negative cells gives the percentage collapse of Mitochondria Membrane Permeability.
Human apoptosis proteome profiler array
To investigate the pathways by which boesenbergin A induces apoptosis, we performed a determination of apoptosis-related proteins using the Proteome Profiler Array (RayBio® Human Apoptosis Antibody Array Kit, RayBiotech, GA, USA), according to the manufacturer’s instructions. Briefly, the cells where treated with boesenbergin A. Three hundred micrograms of protein from each sample were incubated with the human apoptosis array overnight. The apoptosis array data was quantified by scanning the membrane on a Biospectrum AC ChemiHR 40 (UVP, Upland, CA, USA) and analysis of the array image file was performed using image analysis software according to the manufacturer’s instructions.
Western blot analysis
CEMss cells were seeded in 12-well plates and treated with boesenbergin A (8 μg/ml) at 3, 6, 12 and 24 h. The total protein of the cells was extracted with cell lysis buffer (50 mM Tris–HCl pH 8.0, 120 mM NaCl, 0.5% NP-40, 1 mM PMSF). Forty micrograms of protein extract was separated by 10% SDS-PAGE, transferred to a polyvinylidenedifluoride (PVDF) membrane (Bio-Rad), blocked with 5% nonfat milk in TBS-Tween buffer 7 (0.12 M Tris-base, 1.5 M NaCl, 0.1% Tween20) for 1 h at room temperature, incubated with the appropriate antibody overnight at 4°C and then incubated with horseradish peroxidase conjugated secondary antibody for 30 min at room temperature. The bound antibody was detected with peroxidase-conjugated anti-rabbit antibody (1:10000) or anti-mouse antibody (1:10000) followed by chemiluminescence (ECL System) and exposed by autoradiography. The following primary antibodies β-actin (1:10000), Bcl2 (1:1000), Bax (1:1000), HSP70 (1:1000), were purchased from Santa Cruz Biotechnology, Inc, (California, USA).
Data is reported as the mean ± SD of three replicates. The independent t-test and ANOVA were used for comparisons with P < 0.05 considered to be significant. All statistical analyses were performed using the SPSS software (Release 18, SPSS Inc, Chicago, IL, USA).
Cell growth cytotoxic assay
Effect of boesenbergin A on the viability of MCF-7, Hela and CEMss cells for 72 h
IC50± SD (μg /ml)
25.43 ± 0.36
12.21 ± 0.28
8.11 ± 0.44
Cytotoxicity of boesenbergin A on proliferated primary human blood lymphocytes
Effect of boesenbergin A on proliferated primary human blood lymphocyte for 48 h
Boesenbergin A concentration (μg /ml)
Percentage viable cells (%)
Microscopic observation of cellular morphology using phase contrast inverted microscope
Quantification of apoptosis using propidium iodide and acridine orange double staining
Cell cycle analysis
Annexin V assay
Caspase-3/7, -8 and =-9 analyses
Mitochondrial membrane potential analysis
Protein array analysis
Western blot analysis
The rhizome of Boesenbergia rotunda is known to be able to treat a lot of ailments including colic, oral diseases, urinary disorders, dysentery and inflammation, however few studies have been carried out on the pure active compounds derived from this plant. Recently, it was found that boesenbergin A possesses cytotoxic activities against cancer cell lines including HepG2, HT-29, A549 and PC3. In this study, the MTT assay revealed that boesenbergin A had different degrees of cytotoxicity against MCF-7, Hela and CEMss cells (Table 1). with the IC50 for CEMss cells being found to be lower than for the other cells screened. Thus, in the present study, we focused on investigating the cytotoxic activity of boesenbergin A and its underlying mechanism of action against CEMss cells. One of the other benefits found from boesenbergin A is that it has no toxic effects against primary human blood lymphocytes.
Microscopic observations showed that, following treatment with boesembergin A, the numbers of viable CEMss cells were reduced with increasing treatment time. In addition, indications of apoptosis in treated CEMss cells such as cytoplasmic shrinkage and membrane blebbing were observed. It was found that the number of cells undergoing apoptosis was more greater at earlier stages of treatment such as after 24 h and 48 h periods. However, when treatment time increased to 72 h, the presence of necrosis amongst treated CEMss cells was evident. This is possible since treated CEMss cells undergoing apoptosis may have progressed into necrosis due to the prolonged incubation with boesenbergin A. Treated CEMss cells showed morphological changes that included chromatin condensation, DNA fragmentation and membrane blebbing when observed under confocal microscopy using AO/PI staining. Following cell cycle analysis, we were able to further confirm the involvement of apoptosis in CEMss cells upon treatment with boesenbergin A in a time-dependent pattern, as well as observing that the compound induced cell cycle arrest at G2/M phase. Results from the Annexin V assay also point to the involvement of apoptosis in boesenbergin A treated CEMss cells. Similar findings have been reported that panduratin A from Boesenbergia rotunda also has the capability to arrest cells at the G2/M phase and induce apoptosis in PC3 and DU145 human prostate cancer cells and A549 human non-small cell lung cancer cells.
In order to elucidate the mechanism of apoptosis, DNA laddering was performed. DNA fragmentation of CEMss cells was clearly detected after treatment with 16 μg/ml of boesenbergin A for 6 and 12 h. The ability to cause DNA fragmentation is one of the hallmarks of apoptotic cell death[20–22], including nuclear condensation and fragmentation, cleavage of chromosomal DNA into internucleosomal fragments and packaging of the dead cells into apoptotic bodies without plasma membrane breakdown. These features of apoptosis differ significantly from those of necrosis, which is morphologically characterized by vacuolation of the cytoplasm, breakdown of the plasma membrane and induction of inflammation around the dying cell, attributable to the release of cellular contents and pro-inflammatory molecules.
The caspase cascade signaling system is an important component in the process of apoptosis as it is controlled by various molecules that either enhance apoptosis or inhibit apoptosis. In this study, the levels of caspases =-3/7, -8, and =-9 were found to increase when CEMss cells were incubated with boesenbergin A. The activation of caspase-9 provides evidence that the compound is capable of triggering apoptosis via the mitochondrial pathway, whereas the increase in the caspase-3 level suggests that it can trigger DNA fragmentation. The increase in the caspase-8 level is also an indication of apoptosis taking place since this caspase is involved in mediating Fas-induced apoptosis[24–27]. The increase in levels of caspase =-3/7, -8, and =-9 induced in the CEMss cells after treatment with boesenbergin A allows fragmentation of DNA to proceed towards cell death during apoptosis induction. The activation of caspase-9 has previously been found to be the step prior to the activation of caspase-3 in the activation cascade of the mitochondrial intrinsic pathway leading towards apoptosis. This activation of caspase-9 is well controlled by the apoptosome, which converts procaspase-9 to caspase-9. The formation of the apoptosome is fully dependent upon the release of cytochrome c from the mitochondria to the cytosol and adhering to Apaf-1. Since the role of mitochondria in apoptosis is inevitable, we observed a reduction in MMP as the treatment time with boesenbergin A increased. This increase in mitochondria membrane permeability may be due to the up and down regulation of apoptosis proteins involved in the cell death mechanism.
There are a large number of proteins involved in the process of apoptosis[30, 31]. In order to identify the contribution of central apoptosis proteins, we performed a protein array analysis. Several proteins in both the extrinsic and intrinsic pathways were investigated in the current study, including those known to induce apoptosis, such as Bax, caspase-3, caspase-8, SMAC and TRAILR-1 and those known to be anti-apoptotic, such as Bcl-2, X-linked IAP (XIAP) and surviving, where survivin and XIAP are members of the inhibitors of apoptosis (IAP) family of proteins previously and SMAC is a pro-apoptosis protein that interacts with IAP to relieve their inhibitory effects[33, 34].
The obtained protein array results showed a typical profile of protein levels associated with mitochondrial apoptosis in boesenbergin A treated CEMss cells. Hence we then selected the most important proteins involved in this pathway (Bax and Bcl-2) and conducted an immunoblot analysis. The expression of Bax showed an increase, whereas the expression of Bcl-2 was decreased, further confirming the protein array results. The decreased expression of Bcl-2 was expected since Bcl-2 prevents induction of apoptosis by blocking the release of cytochrome c from mitochondria. Moreover, proteins of the Bcl-2 family are known to regulate the promotion and inhibition of apoptosis. These Bcl-2 family proteins are highly expressed in CEMss cancer cells and therefore inhibiting its expression in the cancer cell will trigger cell death[37, 38]. Along with Bcl-2 family members, heat shock proteins also have considered as apoptosis inhibitors, as they play a significant role in the survival of cells either my blocking the release of cytochrome c from mitochondria or by blocking the formation of apoptosome. The immunoblot analysis demonstrated showed that Hsp70 was significantly reduced upon treatment with boesenbergin A. This correlates well to a previous study that showed that over-expression of Hsp70 was able to suppress apoptosis.
On the basis of the observations mentioned in this report, it can be concluded that the treatment of CEMss with boesenbergin A induced apoptosis with cell death-transducing signals that regulate the MMP by down-regulation of Bcl2 and up-regulation of Bax. Cell death was significantly controlled by both initiator and executioner caspases and resulting in the cleavage of specific substrates leading to the process of apoptotic changes. This form of apoptosis was found to be closely associated with the down regulation of Hsp70 and G2/M phase cell cycle arrest. The positive outcomes of our research provide a strong basis for developing boesenbergin A as a novel chemotherapeutic agent for leukemia intervention, which warrants further investigations including in animal models.
In this current study, the results that we gather demonstrated that boesenbergin A induced apoptosis of CEMss cells through Bcl2/Bax signaling pathways with the involvement of caspases and G2/M phase cell cycle arrest. The current findings also warrant further research on boesenbergin A as a novel chemotherapeutic agent for leukemia intervention including studies in animal models.
The authors thank the University of Malaya (UMRG grant RG043/11BIO) and the Ministry of Higher Education (HIR grant F00009-21001) for their financial support. The authors would further like to thank Universiti Putra Malaysia for providing facilities for pursing this investigation.
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