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Introduction

Cyclooxygenases (COX) are inflammatory regulators that mediate the production of prostaglandins from arachidonic acid. Two COX isoforms have been identified (1). COX-1 is constitutively expressed and maintains homeostatic level of prostaglandins, whereas COX-2 is induced by growth factors, tumor promoters, and cytokines (2). To date, COX-2 has been found to be highly expressed in many types of solid cancers including breast, prostate, colon and lung (3,4) and to contribute to tumorigenesis via the inhibition of apoptosis, increased angiogenesis and invasiveness (4). Moreover, in many of these cancer types, an elevated COX-2 expression was correlated with a poor response to therapy and decreased survival (5).

Concerning hematological malignancies, Bernard et al (6) highlighted the recent interest in studying and modulating COX-2 expression in cells of hematopoietic origin. They described the different studies that were conducted on the impact of COX-2 expression in hematological diseases and showed that chronic lymphocytic leukemia, chronic myeloid leukemia, Hodgkin’s lymphoma, non-Hodgkin’s lymphoma and multiple myeloma all highly express COX-2 and that elevated COX-2 expression is often correlated with decreased survival of patients with hematological malignancies (6). As for acute myeloid leukemia, COX-2 has been shown to be expressed in various cell lines and functional genetic variations of COX-2 have been recently correlated to susceptibility to acute myeloid leukemia (7,8). However, there are scarce data focused on the effect of COX-2 expression in erythroleukemia cells, a subtype of acute myeloid leukemia with a very poor response and survival to current available therapeutic agents (9).

The interest on COX-2 activity in hematological malignancies has also been reinforced by the use of NSAIDs and COX-2 selective inhibitors in vitro, to induce proliferation arrest and apoptosis in leukemia cells (6,10,11). Furthermore, it was also shown that targeting COX-2 reduced toxicity toward low-dose chemotherapy with vinblastine and extended survival in an erythroleukemia model of juvenile mice with Friend disease (12).

Despite this evident interest of COX-2 modulation in leukemia cells, literature lacks detailed data on the role of COX-2 in myeloid leukemia onset and management and particularly in cases of erythroleukemia.

Berberis libanotica (Bl), specifically the roots, has been used in traditional herbal Lebanese remedies for rheumatic and neuralgic diseases (13,14). B. vulgaris and B. stata are the two most studied species of Berberis (15–18). Alkaloids constitute the major class of compounds reported to exist in Berberis species and represent a very wide range of secondary metabolites with important biological activities (19,20). Various herbal alkaloids exhibit in vitro and in vivo anti-proliferative and anti-metastatic effects on various types of cancers. Alkaloids, such as camptothecin (21) and vinblastine (22), have already been successfully developed into anticancer drugs. Berberine, a major alkaloid characterizing Berberis species, has been intensively investigated for its pharmacological properties. It was shown to inhibit the migration of melanoma cancer cells (23), and the growth of human tongue squamous carcinoma tumors in a murine xenograft model (24), enhance tumor necrosis factor-related apoptosis-inducing ligand in breast cancer (25), and exert a cytotoxic effect against many cell lines (23,26,27). To date, the biological and phytochemical properties of Bl extracts have only been investigated in three studies reporting the inhibition of adult T-cell leukaemia viability via ethanol fraction (28), the inhibition of key enzymes linked to Alzheimer’s disease (13), and the anti-neoplastic effects on prostate cancer stem/progenitor cells (29).

In this overall context, the aim of this study was to describe and understand the relationship between COX-2 expression and apoptosis rate in erythroleukemia cells after apoptosis induction by Bl extract. To achieve this goal we used erythroleukemia cells lines expressing COX-2 (HEL cell line) or not (K562 cell line). Moreover, we made use of COX-2 cDNA to overexpress COX-2 in K562 cells. Then, to understand the mechanisms implicated in the effect of Bl extract, we studied intracellular signalling pathways.

Materials and methods

Materials

RPMI-1640, fetal calf serum (FCS) and penicillin streptomycin were supplied by Gibco BRL (Cergy Pontoise, France). Human antibody against caspase-9 was purchased from Cell Signaling Technology (Ozyme, France), poly-ADP-ribose polymerase (PARP), p-Akt antibodies were purchased from Santa Cruz Biotechnology (Tebu-Bio, Le Perray en Yvelines, France), cyclooxygenase-2 (COX-2) and β-actin were respectively purchased from Cayman Chemical (Bertin Pharma, Montigny le Bretonneux, France) and Sigma-Aldrich (Saint Quentin Fallavier, France).

Berberis libanotica extraction and HPLC

Berberis libanotica was collected from Ehden, North of Lebanon, in November 2012 at an altitude up to 1521 m. Botanical identity was authenticated by Professor S. Safi, Biology Department, Faculty of Science II, Lebanese University, Fanar, Lebanon. Powdered root material (10 g) was extracted with ethanol (100 ml) for 48 h under magnetic stirring at room temperature, then it was filtered using Whatman paper number 1, and concentrated using a rotator evaporator. The extraction method used has been reported (30). The filtred extract was dried with liquid nitrogen and stored at 4°C.

HPLC was done on a Waters Alliance 2690 using a reversed-phase C18 X-Terra® 5 μm (150×4.6 mm) and using a photodiode-array detector (Waters 996). TLC was performed on pre-coated silica gel aluminium sheets (kieselgel 60 F254, 0.20 mm, Merck). Visualisation of plates was carried out under UV light (254 and 365 nm) and using Draggendorf reagent. Compounds were identified by HPLC (RP-18 column, ACN-H2O-H3PO4, flow rate, 1 ml/min) with CHCL3/MeOH/NH4OH (80/20/0.5).

Cells lines and cell culture

The HEL and K562 human erythroleukemia cell lines were kindly provided, respectively, by Professor J.P. Cartron (INSERM U76, Paris, France) and Dr I. Dusanter-Fourt (INSERM U567, CNRS UMR 8104, Paris, France). Cells were seeded at 105 cells/ml in 75-cm2 tissue culture flasks and grown in RPMI-1640 medium (Gibco BRL, Cergy-Pontoise, France) supplemented with 10% fetal calf serum (Gibco BRL), 1% sodium pyruvate, 1% HEPES (N-(2-hydroxyethyl)piperazine-N′-2-ethanesulfonic acid), 100 U/ml penicillin and 100 μg/ml streptomycin (Gibco BRL). Cultures were maintained in a humidified atmosphere with 5% CO2 at 37°C. Cells were allowed to grow for 24 h in culture medium prior to exposure or not to 40–300 μg/ml Bl extract or 20 and 40 μM berberine (Sigma-Aldrich) for 6–72 h.

COX-2 cDNA transfection

COX-2 transfection-ready cDNA was purchased from OriGene Technologies (Rockville, MD, USA) and was transfected to K562 cells by electroporation using the AMAXA Nucleofactor system (Lonza). Stable K562 cell line was obtained after transfection and selection with 0.5 mg/ml of neomycin (G418, Sigma-Aldrich). COX-2 expression was confirmed by western blotting.

Cell proliferation and lactate dehydrogenase (LDH) assays

Measurement of cell proliferation was determined using the 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) assay. HEL, K562 and K562 (COX-2+) cells were cultured and plated, respectively, at 105 cells/ml in 10% FCS medium in 96-well culture plates and grown 24 h before treatment or not (time 0) with 50–300 μg/ml Bl extract for 24–72 h. MTT tests were carried out daily as previously described (31) and experiments were performed in three independent assays.

The cytotoxicity of Bl extract on the three cell lines was determined by measuring the activity of LDH released from the cytosol of damaged cells using a Cytotoxicity Detection kit PLUS (LDH) (Roche Diagnostics GmbH). The assay was conducted following the manufacturer’s instructions. Briefly, medium supernatants of control and treated cells were collected and equal volume of reaction mixture was added. The reaction mixtures were incubated for 20 min at room temperature in the dark. Following incubation, the absorbance was determined at 490 nm using an ELISA plate reader. The percentage of cytotoxicity was calculated according to the manufacturer’s instructions.

Mitochondrial membrane potential (Δψm)

Δψm was estimated using 5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethylbenzimidazole carbocyanide iodide (JC-1, Molecular Probes). JC-1 is a fluorescent compound that exists as a monomer at low concentrations. At higher concentrations, it forms aggregates. Fluorescence of the JC-1 monomers is green, whereas that of aggregates is red. Mitochondria with intact membrane potential concentrate JC-1 into aggregates, which fluoresces red, whereas de-energized mitochondria cannot concentrate it and are stained green (31,32).

HEL, K562 and K562 (COX-2+) cells were grown for 24 h before treatment with 50–300 μg/ml Bl extract for 6 and 24 h. Control cells were grown in medium containing the same amount of vehicle as treated cells. Then cells were incubated in 1 ml of medium containing JC-1 (1 μg/ml) for 30 min at 37°C and images were taken with a confocal laser microscope (Zeiss LSM 510 Meta).

Protein expression

After treatment, HEL, K562 and K562 (COX-2+) cells were washed and lysed in RIPA lysis buffer (50 mM HEPES pH 7.5, 150 mM NaCl, 1% deoxycholate, 1% NP-40, 0.1% SDS, 20 μg/ml aprotinin) containing protease inhibitors (Complete™ Mini, Roche Diagnostics, Meylan, France). Briefly, as previously described (33), proteins (10–100 μg) were separated by electrophoresis on SDS-polyacrylamide gels, transferred to PVDF membranes (Amersham Pharmacia Biotech, Saclay, France) and probed with respective human antibodies against caspase-9 (Cell Signaling Technology, Ozyme, France), poly-ADP-ribose polymerase (PARP), p-Akt (Santa Cruz Biotechnology) and COX-2 (Cayman Chemical, Bertin Pharma). After incubation with secondary antibodies (Dako France S.A.S., Trappes, France), blots were developed using the ECL Plus Western Blotting Detection system (Amersham Pharmacia Biotech) and G:BOX system (Syngene, Ozyme, Saint Quentin en Yvelines, France). Membranes were then reblotted with anti-β-actin (Sigma-Aldrich) used as a loading control.

Caspase-3 activity

Caspase-3 activity was assayed using Quantikine® human active caspase-3 (R&D Systems) as previously described (34). HEL, K562 and K562 (COX-2+) cells were treated or not with 50–300 μg/ml Bl extract for 24 and 48 h, and then incubated with 10 μM biotin-ZVKD-fmk inhibitor for 1 h at 37°C. Caspase-3 activity was measured in accordance with the manufacturer’s protocol (R&D Systems). Briefly, cells were harvested, washed in PBS and resuspended in extraction buffer containing protease inhibitors. Standards and sample extracts containing covalently linked active caspase-3-ZVKD-biotin were added to a microplate pre-coated with monoclonal antibody specific for caspase-3. Then, streptavidin conjugated to horseradish peroxidase was added to the wells. The amount of active caspase-3 was quantified by colorimetry at 450 nm after addition of HRP substrate.

Apoptosis quantification: DNA fragmentation

HEL, K562 and K562 (COX-2+) cells were seeded at 105 cells/ml in 75-cm2 tissue culture flasks and then treated or not with 50–300 μg/ml Bl extract for 24 and 48 h, or with 20 and 40 μM berberine for 48 h. Apoptosis was quantified on pooled cells (floating and adherent) using ‘cell death’ enzyme-linked immunosorbent assay (ELISA) (Cell Death Detection ELISAPlus, Roche Diagnostics). Cytosol extracts were obtained according to the manufacturer’s protocol and apoptosis was measured as previously described (35).

Subcellular protein fractionation

HEL and K562 (COX-2+) cells were incubated alone or with 300 μg/ml Bl extract for 12, 24 and 48 h, or with 20 and 40 μM berberine for 48 h. Cytosolic and nuclear fractions were obtained using the Subcellular Protein Fractionation kit according to the manufacturer’s protocol (Thermo Fischer Scientific, Rockford, IL, USA) as previously described (31).

Electromobility shift assay (EMSA)

EMSA experiments were performed using DIG Gel Shift kit (Roche Diagnostics) (36). Briefly, nuclear extracts were prepared from HEL and K562 (COX-2+) cells treated or not with 300 μg/ml Bl extract for 12, 24 and 48 h, or with 20 and 40 μM berberine for 48 h. NF-κB binding reactions were carried out with 10 μg nuclear proteins incubated with digoxigenin (DIG) labeled NF-κB probe according to the manufacturer’s protocol. The samples were loaded on a 5% native polyacrylamide gel in Tris-borate-EDTA buffer. After transfer to nylon membranes and incubation with anti-DIG antibody conjugated with alkaline phosphatase, gel mobility shift was visualized by incubation with CSPD® chemiluminescence reagent and G:BOX system (Syngene). Quantification of each band was performed by densitometry analysis software in respect of band intensity and band area. Results are expressed relative to controls in arbitrary units.

Statistical analysis

Data are expressed as the arithmetic means ± standard deviation (SD) of separate experiments. The statistical significance of results obtained from in vitro studies was evaluated by the two tailed unpaired Student’s t-test, with p<0.05 being considered as statistically significant.

Results and Discussion

The HPLC chromatogram show three main peaks at tR = 12.5, 17.5 and 20.1 min (Fig. 1A). By comparing the control, we found that the peak with a tR = 20 min matches to berberine. The two other peaks matched with alkaloids derived from berberine regarding close similarities between their UV spectrum and the UV spectrum of the control (Fig. 1B).

Figure 1 HPLC chromatogram (A) and UV spectra of the three main peaks of ethanolic extract of Berberis libanotica (B).

In light of the reported chemopreventive and chemosensitive effects of natural products on various tumor cells and animal models, we postulated that our Bl extract may mediate its effects through apoptosis induction with suppression of cell survival pathways. Our study is the first report on the specific examination of intrinsic apoptosis and Akt/NF-κB/COX-2 pathways in human erythroleukemia cells upon Bl extract exposure.

In this study, we aimed to establish cellular models of erythroleukemia cells in which we could study the effect of COX-2 expression. As COX-2 has been widely implicated in apoptosis resistance in various cancer cells (4,37–39) including leukemia cells (6–8,40), we further checked for the first time whether COX-2 expression could modulate apoptosis induction by Bl extract in erythroleukemia cells.

We first demonstrated that, under our experimental conditions, a decrease in proliferation was observed as early as 24 h after Bl extract treatment in a dose- and time-dependent manner for the three cell lines (Fig. 2) without significative difference between K562 and K562 (COX-2+) cells. Furthermore, Bl extract engendered only a very low cytotoxicity on HEL cells (5.2% at 60 μg/ml for 72 h versus control, p<0.05) and K562 cells (7.8% at 60 μg/ml for 72 h versus control, p<0.05) (Fig. 3).

Figure 2 Effect of Bl extract on human erythroleukemia cell growth. Cells were cultured in 10% FCS medium during 24 h and treated or not with 50–300 μg/ml Bl extract for 24–72 h. Cell proliferation was followed by MTT test. *p<0.05 versus control.

Figure 3 Effect of Bl extract on human erythroleukemia cell cytotoxicity. Cells were cultured in 10% FCS medium during 24 h and treated or not with 40–60 μg/ml Bl extract for 24–72 h. Cell cytotoxicity was followed by LDH test. *p<0.05 versus control.

Apoptosis is characterized by chromatin condensation and DNA fragmentation, and is mediated by caspases (41). Mitochondria are involved in a variety of key events, including release of caspase activators, changes in electron transport, loss of mitochondrial membrane potential (Δψm), and participation of both pro- and anti-apoptotic Bcl-2 family proteins (42). Alterations in mitochondrial structure and function have been shown to play a crucial role in caspase-9-dependent apoptosis (43). Caspase-9 cleaves and activates caspase-3, the executioner caspase, which cleaves PARP and activates endonucleases leading to DNA fragmentation (43). Mitochondria have, apart from their function in respiration, an important role in the apoptotic-signalling pathway. It is well known that the modification of Δψm depends on the nature of the stimulus and the cell system and the collapse of Δψm is an early step in the apoptotic cascade (44). To determine potential mechanisms by which Bl extract inhibited the human erythroleukemia cell proliferation, we analyzed the effect of Bl extract on Δψm. Δψm was analyzed after 6- and 24-h treatment with Bl extract using JC-1. We found that Bl extract decreased Δψm in a dose- and time-dependent manner for the three cell lines (Fig. 4), shown by the incorporation of JC-1 monomers into mitochondria (green fluorescence), compared with cytosolic JC-1 aggregate formation at high membrane potentials in control cells (red fluorescence). Furthermore, this assay showed a dominant effect of 50 μg/ml Bl extract on early intrinsic apoptosis of K562 cells for 24-h treatment (Fig. 4B) compared to K562 (COX-2+) cells (Fig. 4C).

Figure 4 Effect of Bl extract on HEL (A), K562 (B) and K562 (COX-2+) (C) cell mitochondrial membrane potential. Cells were cultured in 10% FCS medium for 24 h and treated or not with Bl extract at 50–300 μg/ml for 6 and 24 h. After treatment, cells were incubated with medium containing JC-1 (1 μg/ml) for 30 min at 37°C. Red fluorescence represents mitochondria with intact membrane potential whereas green fluorescence represents de-energized mitochondria. Images were taken with a confocal laser microscope (Zeiss LSM 510 Meta) (×100). The images are representative of three separate experiments.

Caspase-3 is a key executioner of apoptosis, its activation is mediated by the initiator caspases such as caspase-8 and caspase-9 (45). In our study, we showed that intrinsic apoptosis pathway was implicated in Bl extract-induced apoptosis in human erythroleukemia cells. Indeed, we showed that Bl extract induced an activation of caspase-9 especially at 300 μg/ml after 48-h treatment as shown in Fig. 5. Bl extract induced a cleavage of caspase-9 at 48 h but the expression of cleaved fragment of caspase-9 after 300 μg/ml Bl extract treatment for HEL and K562 (COX-2+) cells was more important than in K562 cells. Consequently, 300 μg/ml Bl extract induced activation of executive caspase-3 activity in the three cell lines (+3-fold versus control at 48 h for HEL cells, +6-fold versus control at 48 h for K562 cells, and +5-fold versus control at 48 h for K562 (COX-2+) cells, p<0.05) (Fig. 6). These observations were directly correlated with PARP cleavage because western blot analysis detected the cleaved form of PARP in 300 μg/ml Bl extract treated cells (Fig. 7). Cleaved fragment of PARP was expressed starting at 24 h for 300 μg/ml Bl extract treatment and strongly maintained after 48-h treatment (Fig. 7). PARP is a nuclear enzyme involved in the repair of DNA damage (46). Moreover, it is known that PARP is a substrate for caspases such as caspase-3 and is typically cleaved and inactivated during the apoptotic process (47).

Figure 5 Effect of Bl extract on caspase-9 expression in human erythroleukemia cells. Cells were cultured in 10% FCS medium for 24 h and treated or not with 50–300 μg/ml Bl extract for 24 and 48 h. Protein expression was analyzed by western blotting. β-actin was used as a loading control. Blots are representative of three separate experiments.

Figure 6 Effect of Bl extract on caspase-3 activity in human erythroleukemia cells. Cells were cultured in 10% FCS medium for 24 h and treated or not with 50–300 μg/ml Bl extract for 24 and 48 h. Caspase-3 activity was assayed using Quantikine human active caspase-3 (R&D Systems). Following treatment, cells were incubated with 10 μM biotin-ZVKD-fmk inhibitor for 1 h at 37°C. The amount of active caspase-3 was quantified by colorimetry at 450 nm; values are expressed as mean ± SD of three separate experiments and reported as n-fold (*p<0.05) compared to control.

Figure 7 Effect of Bl extract on PARP cleavage in human erythroleukemia cells. Cells were cultured in 10% FCS medium for 24 h and treated or not with 50–300 μg/ml Bl extract for 24 and 48 h. PARP cleavage was analyzed by western blotting. PARP cleavage was assessed by detection of the 85-kDa band (cleaved PARP) after probing with a mouse anti-human PARP antibody. β-actin was used as a loading control. Blots are representative of three separate experiments.

DNA fragmentation occurs simultaneously with this phenomenon and is considered as a major marker of apoptotic cells. DNA fragmentation was observed in human erythroleukemia cells after Bl extract treatment. Quantitative determination of cytoplasmic histone-associated DNA fragments (mono and oligonucleosomes) was performed by ELISA in our study. Results showed that DNA fragmentation was strongly induced in the three cell lines after 48-h Bl extract treatment [+3.3-, +6.5 and +5.8-fold versus control respectively for HEL, K562 and K562 (COX-2+), p<0.05] (Fig. 8). It is important to note that DNA fragmentation is the strongest in K562 cells not expressing COX-2.

Figure 8 Effect of Bl extract on DNA fragmentation in human erythroleukemia cells. Cells were cultured in 10% FCS medium for 24 h and treated or not with 50–300 μg/ml Bl extract for 24 and 48 h. DNA fragmentation was quantified from cytosol extracts according to the manufacturer’s instructions (Cell Death Detection ELISAplus, Roche Diagnostics). Results were reported as n-fold compared to control. Values are expressed as mean ± SD (p-value relative to control group, *p<0.05).

In summary, even if Bl extract induced apoptosis of three human erythroleukemia cell lines, a dominant effect of Bl extract treatment on K562 cells was observed resulting in activation of the late markers of apoptosis with caspase-3 activation, PARP cleavage and DNA fragmentation.

It is well known that COX-2 expression is correlated with the activities of intracellular signalling proteins such as NF-κB (48). Furthermore, we showed recently that COX-2 positively regulated Akt signalling and enhanced survival of cancer cells exposed to anticancer agents (35). Numerous studies have shown that COX-2 expression prevents apoptosis in cancer cells, especially in colon (49,50) and prostate cancer (51–53). Here, we showed that Bl extract reduced significantly expression of COX-2 by a dose-dependent manner at 48-h treatment in HEL and K562 (COX-2+) cells (Fig. 9).

Figure 9 Effect of Bl extract on COX-2 expression. HEL and K562 (COX-2+) cells were cultured in 10% FCS medium for 24 h and treated or not with 50–300 μg/ml Bl extract for 24 and 48 h. COX-2 expression was determined by western blot analysis. β-actin was used as a loading control. Blots are representative of three separate experiments.

Among the cell signalling pathways that promote cell survival, Akt is one of the most important (54). Activated Akt can also exert anti-apoptotic effects, positively regulate NF-κB transcription, modulate angiogenesis, promote tumor invasion/metastasis and antagonize cell cycle arrest (55). Akt is also reported to modulate the NF-κB transcription factor through the phosphorylation of p65 to enhance the transcriptional activity of NF-κB (56). In turn, NF-κB activation can regulate the expression of cell survival, proliferative, metastatic and angiogenic gene products (57). We analyzed the effect of Bl extract on two survival pathways: Akt and NF-κB. Western blot analysis showed that 300 μg/ml Bl extract markedly inhibited Akt phosphorylation in HEL and K562 (COX-2+) cells at 48-h treatment (Fig. 10A). Since NF-κB activation is critical for apoptosis resistance, we examined the effect of Bl extract on nuclear activation of NF-κB. Our results showed that 300 μg/ml Bl extract inhibited NF-κB activation at 12- and 48-h treatment (Fig. 10B). In regard to these results, it is clear that the simultaneous inhibition of Akt and NF-κB signalling can significantly contribute to the anticancer effects of Bl extract in human erythroleukemia cells.

Figure 10 Effect of Bl extract on p-Akt expression and NF-κB activation. HEL and K562 (COX-2+) cells were cultured in 10% FCS medium for 24 h and treated or not with 50–300 μg/ml Bl extract for 24 and 48 h. Akt phosphorylation (A) was determined by western blot analysis. β-actin was used as a loading control. Blots are representative of three separate experiments. (B) EMSA experiments were performed using DIG Gel Shift kit (Roche Diagnostics) on nuclear extracts. Blots are representative of three separate experiments.

The results of Bl extract HPLC profile showed that berberine is the major product (Fig. 1), thus, we then tested this molecule on the induction of DNA fragmentation, the expression of COX-2 and phospho-Akt (p-Akt) and the activation of NF-κB. From the report of Bonesi et al giving the chemical composition of Bl extract, 300 μg/ml of our Bl extract would correspond to 40 μM of pure berberine (13). Based on these calculations, we then tested berberine in 20 and 40 μM on human erythroleukemia cells. Our results showed that especially 40 μM berberine induced DNA fragmentation of three cell lines [+1.6-fold for HEL cells, +2.7-fold for K562 cells and +2-fold for K562 (COX-2+) versus control, p<0.05] (Fig. 11). Whereas, western blot analysis showed that 40 μM berberine markedly inhibited COX-2 expression and Akt phosphorylation in HEL and K562 (COX-2+) cells at 48-h treatment (Fig. 12A). Furthermore, our results showed that 40 μM berberine inhibited NF-κB activation at 48-h treatment (Fig. 12B). Recently, Fu et al demonstrated that berberine inhibited human non-small cell lung cancer cell growth by simultaneously targeting NF-κB/COX-2, PI3K/Akt and caspase signalling pathways (58). Furthermore, others studies showed an antitumor effect of berberine via inhibition of NK-κB pathway and induction of apoptosis (59,60).

Figure 11 Effect of berberine on DNA fragmentation in human erythroleukemia cells. Cells were cultured in 10% FCS medium for 24 h and treated or not with 20 or 40 μM berberine for 48 h. DNA fragmentation was quantified from cytosol extracts according to the manufacturer’s instructions (Cell Death Detection ELISAplus). Results were reported as n-fold compared to control. Values are expressed as mean ± SD (p-value relative to control group, *p<0.05).

Figure 12 Effect of berberine on COX-2 and p-Akt expression and NF-κB activation. HEL and K562 (COX-2+) cells were cultured in 10% FCS medium for 24 h and treated or not with 20 or 40 μM berberine for 48 h. COX-2 expression and Akt phosphorylation (A) were determined by western blot analysis. β-actin was used as a loading control. Blots are representative of three separate experiments. (B) EMSA experiments were performed using DIG Gel Shift kit on nuclear extracts. Blots are representative of three separate experiments.

Our results clearly indicate for the first time that Bl extract exert their potent anti-proliferative and pro-apoptotic effects through the modulation of Akt/NF-κB/COX-2 signal transduction pathways in human erythroleukemia cells and do not act specifically on any one cellular signalling cascade. It is obvious that Bl extract is not active against a specific signalling cascade but it can interfere with a multitude of targets in human erythroleukemia cells. This is quite relevant to the changing paradigm in cancer therapy, as increasing evidence indicates that the mono-targeted drugs, once called smart drugs, have not had a significant impact on cancer treatment and the use of multi-targeted drugs has become increasingly accepted, as it is obvious that cancer is caused by dysregulation of multiple pathways (61). Our results show that Bl extract has a dominant effect on K562 cells do not expressing COX-2 compared to HEL and K562 (COX-2+) cells. Furthermore, the significance of our in vitro study between Bl extract and berberine effects in human erythroleukemia cells is very encouraging suggesting the relevance of testing these compounds in xenograft animal models.

Acknowledgements

We thank Claire CARRION (UMR CNRS 7276, Platform CIM) for the analyses of imaging. This study was supported by grants from the French Ministry of Education and Research and from the Lebanese University.

References