The Potential Role of Bone Marrow Derived Mesenchymal Stem Cells Conditioned Medium in the Suppression of Hepatocellular Carcinoma In Vitro: Modulation of Apoptosis

Mahmoud Abdelhady Metwally1*, Mona Abdelftah Ali1, Farouk Abdelmohdy1, Mohamed Kassab1, Tarek Kamal Abouzed2 and Khalil Fathy Abou-Easa1

1Department of Cytology and Histology, Faculty of Veterinary Medicine, Kafrelsheikh University, Kafrelsheikh, Egypt

2Department of Biochemistry, Faculty of Veterinary Medicine, Kafrelsheikh University, Kafrelsheikh, Egypt.

ABSTRACT

Bone marrow mesenchymal stem cells (BMMSCs) can home to cancerous cells and suppress their growth. However, few studies have investigated the impact of conditioned medium harvested from BMMSCs on carcinogenesis. This study investigated the effect of BMMSCs-conditioned medium (BMMSCs-CM) on the hepatoma cell line HepG2 and described the underlying molecular mechanisms involved. We isolated BMMSCs and identified them using flowcytometry and culture characteristics, then prepared BMMSCs-CM. HepG2 cells were treated with various concentrations of BMMSCs-CM for up to 72 h. The methylthiazolyldiphenyl-tetrazolium (MTT) assay showed decreased proliferation, while flowcytometry showed increased apoptosis and cell cycle arrest in the G0/G1 phase with inhibition of entry into the S phase. RT-PCR showed p53 upregulation and Bcl-2 downregulation in mRNA expression. Moreover, Western blotting and flowcytometry revealed elevated p53 and lowered Bcl-2 protein levels. In addition, ELISA findings showed decreased toll-like receptor 4 (TLR4) concentration. Taken together, our findings highlight the potent therapeutic function of BMMSCs-CM in suppressing HepG2 cancerous cells across multiple platforms, including proliferation, apoptosis, cell cycle, and oncogene expression. Furthermore, our findings suggest that the Notch and TLR4/NF-kB signaling pathways may be targets of BMMSCs-CM for tumor cell suppression.

Article Information

Received 16 March 2022

Revised 25 April 2022

Accepted 11 May 2022

Available online 08 September 2022

(early access)

Published 29 September 2023

Authors’ Contribution

MAM provided the concept of the research, performed the experiments and wrote the manuscript. MAA and FA supervised the study. MK helped in manuscript writing. TKA assisted in the data analysis in the experiment. KFA supervised the study and helped in the lab work.

Key words

Bone marrow-derived Mesenchymal stem cells, Mesenchymal stem cells conditioned medium, Hepatocellular carcinoma, HepG2 cell apoptosis, Liver cancer

DOI: https://dx.doi.org/10.17582/journal.pjz/20220316180305

* Corresponding author: mahmoud_abdelhady@vet.kfs.edu.eg

030-9923/2023/0006-2595 $ 9.00/0

Copyright 2023 by the authors. Licensee Zoological Society of Pakistan.

This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license (https://creativecommons.org/licenses/by/4.0/).

Introduction

Liver cancer persists as a global health issue as its prevalence is increasing worldwide (Craig et al., 2020; Llovet et al., 2021). It is anticipated that more than 1 million people will be diagnosed with liver cancer each year by 2025 (Llovet et al., 2021). The most frequent type of liver cancer is hepatocellular carcinoma (HCC), which accounts for 90% of all liver cancer cases globally (Craig et al., 2020). Among Egyptians, HCC is ranked as the fourth most common form of cancer (Rashed et al., 2020). Moreover, HCC is the world’s fourth most common cause of cancer mortality (Yang et al., 2019).

There are multiple major risk factors for inducing HCC, including hepatitis C virus (HCV), hepatitis B virus (HBV), non-alcoholic liver disease, consumption of food contaminated with aflatoxin B1 and excessive alcohol intake (Abdelkawy et al., 2020).

HCC develops as a consequence of an imbalance between excessive cell proliferation and apoptosis, which is primarily mediated by the tumor suppressor gene p53 and the anti-apoptotic gene Bcl-2. Declined levels of p53 and elevated levels of Bcl-2 have been linked to hepatocarcinogenesis and have been extensively described in HCC (Mahfouz et al., 2021; Mansour et al., 2021).

Surgery, radiation, and chemotherapy are all traditional cancer treatments that are either invasive or produce unfavorable side effects. Therefore, finding innovative approaches to slow the course of HCC and to prevent metastasis is critical (Mohamed et al., 2019; Selim et al., 2019).

Advancements in stem cell biology have facilitated real-world clinical applications of cell therapy and tissue regeneration (Kwon et al., 2018). Stem cells, particularly mesenchymal stem cells (MSCs), have shown unique biological properties such as self-renewal, multilineage differentiation, and immunomodulation, leading to their widespread use in regenerative medicine (Tae et al., 2006).

MSCs are adult, nonhemopoietic, multipotent cells that can differentiate into various types of cells and can be isolated from numerous sources in the body, including umbilical cord (Erices et al., 2000), adipose tissue (Zuk et al., 2002), placenta (Fukuchi et al., 2004), peripheral blood (Villaron et al., 2004) and bone marrow (El-Magd et al., 2019). Bone marrow mesenchymal stem cells (BMMSCs) can be harvested with ease from a simple bone marrow aspirate, making them a simple and attractive source for acquiring MSCs.

Many studies have been conducted to clarify the interactions between MSCs and cancer cells; however, the precise roles that MSCs play in cancer modulation is debatable. On one hand, MSCs have been shown to exhibit protumor effects and promote metastasis in human breast cancer via chemokine secretion (Karnoub et al., 2007). On the contrary, using MSCs in a kaposi sarcoma model produced strong pro-apoptotic and antitumorigenic effects (Khakoo et al., 2006), and in a glioblastoma multiforme model caused disturbances in tumor cells’ growth and proliferation pathways with selective induction of cancer cell apoptosis (Akimoto et al., 2013).

MSCs transplantation carries its own risks, whether it’s infection or graft failure (Lukomska et al., 2019), making the use of MSCs secretome such as exosomes (Alzahrani et al., 2018; Zahran et al., 2020), through the preparation of conditioned medium (CM) a valid option in mitigating transplantation associated complications (Di Santo et al., 2009). Investigations regarding Adipose tissue-derived MSCs-CM have shown potent anti-tumor effects experimentally (Yang et al., 2014). However, few studies have reported the influence of BMMSCs-CM on HCC.

This study aimed to investigate how BMMSCs-CM could affect carcinogenesis in an HCC cell line, HepG2, in vitro, through modulating cellular proliferation, apoptosis, and cancer marker expression.

Materials and Methods

Chemicals and cell line

Dulbecco’s modified Eagle’s medium (DMEM) (Cat. no. 41965-039) and fetal bovine serum (Cat. no. 10270-106) were purchased from Gibco, USA. Penicillin-streptomycin (Cat. no. P4333), Amphotericin B (Cat. no. A2942), and RNase-free water (Cat. no. 7732-18-5) were bought from Sigma, USA. CyQUANT 3-[4, 5-dimethylthiazol-2-yl]-2, 5 diphenyl tetrazolium bromide (MTT) cell viability assay kit (Cat. no. V-13154), Maxima SYBR green (Cat. no. K0222), Pierce rapid gold BCA protein assay kit (Cat. no. A53225) and TMB blotting substrate solution (Cat. no. 34018) were obtained from Thermo Scientific, USA. Quanti Tects Reverse Transcription kit (Cat. no. 205310) was bought form Qiagen, USA. Annexin V-FITC stain kit (Cat. no. 556547), and the antibodies against CD44 (Cat. no. 550989), CD90 (Cat. no. 555595), CD34 (Cat. no. 348053), and CD105 (Cat. no. 561443) were acquired from BD Pharmingen, USA. The antibodies against p53 (Cat. no. ab17990) (Cat. no. ab131442), Bcl-2 (Cat. no. ab692) (Cat. no. ab196495), β-actin (Cat. no. ab8227), and HRP-conjugated secondary antibody (Cat. no. ab97185) were purchased from Abcam, UK. Human Toll-like receptor 4 (TLR4) ELISA Kit (Cat. no. ELH-TLR4) was bought from RayBiotech, USA. TRIzol reagent (Cat. no. 15596026) was acquired from Invitrogen, USA and the primers for p53, Bcl-2, and β-actin (Table I) were obtained from Integrated DNA Technologies (IDT)-Coralville, USA. HepG2 cells (human liver carcinoma cell line) was purchased from National Oncology Institute, Egypt.

Animals

Eight-week-old male albino rats from the Animal Center of Kafrelsheikh University weighing 90g were used for the isolation of BMMSCs-CM. Any operation involving the animals and their welfare followed the guidelines and was reviewed by the Research Ethics Committee of the Faculty of Veterinary Medicine, Kafrelsheikh University, giving the ethical approval.

 

Table I. The primers sequences for Real-Time PCR.

Gene	Nucleotide sequences	Reference
P53	F 5′ CCTCAGCATCTTATCCGAGTGG 3′ R 5′ TGGATGGTGGTACAGTCAGAGC 3′	(Andries et al., 2015)
Bcl-2	F 5′ CATGTGTGTGGAGAGCGTCAAC 3′ R 5′ CAGATAGGCACCCAGGGTGAT 3′	(Baharara et al., 2015)
β-actin	F 5′ CCCGCCGCCAGCTCACCATGG 3′ R 5′ AAGGTCTCAAACATGATCTGGGTC 3′	(Baharara et al., 2015)

 

Isolation of bone marrow mesenchymal stem cells

The rats were sacrificed by cervical dislocation, and both the tibia and femur of both limbs were collected. The muscular and connective tissues covering the bones were detached and eliminated. The bones were further cleaned using sterile gauze to remove any residual tissue attached, and placed on an aseptic glass dish containing a mixture of DMEM and 10% FBS to conserve the tissue. A volume of 20 ml of maintenance medium was prepared in a test tube. Both ends of each bone were cut. Using a sterile 2 ml syringe, the maintenance medium in the tube was aspirated and forced slowly into the medullary cavity of each bone from one end. From the opposite end, the flushed content containing suspended bone marrow cells was received in a 15 ml Eppendorf tube, then centrifuged (Thermo Fisher Megafuge16R, USA) at 500g for 5 min. The supernatant was removed, and the bottom layer of suspended cells was pipetted into a 25-ml tissue culture flask previously filled with 4 ml of growth medium, consisting of DMEM, 10% FBS, and a 1% antimicrobial mixture of amphotericin B and penicillin-streptomycin. These flasks were incubated (Thermo Fisher Heracell 150i, USA) at 5% CO2 and 37°C and passaged. The first and second passages took longer to adapt to in-vitro conditions, while the cells in the third passage required a relatively shorter time period to adapt to the new environment.

Identification of BMMSCs-CM

In the third passage, cells were identified according to the International Society for Cellular Therapy (ISCT) guidelines (Dominici et al., 2006). The cells were evaluated for their fibroblast-like appearance and plastic adherence in culture (Dominici et al., 2006). In addition, flowcytometry was used to determine the expression of CD44, CD90, and CD105, which are characteristic surface markers for BMMSCs (Dominici et al., 2006; Secunda et al., 2015), and CD34, which is an endothelial and hemopoietic surface marker (Secunda et al., 2015). The flowcytometry procedure was performed according to the manufacturer’s instructions, where 100 µl of cell suspension was prepared from third passage cells, using TRIS EDTA buffer. Cells were washed with PBS then centrifuged at 2000 rpm for 5 min. The supernatant was discarded, and the produced pellet was resuspended in 100 µl PBS. 7µl of FITC-anti-CD44 antibody, FITC-anti-CD90 antibody, FITC-anti-CD105 antibody, and FITC-anti-CD105 antibody were added separately, mixed well, and incubated at room temperature in the dark for 30 min. The cells were then washed with PBS, centrifuged, resuspended, and fixed in 200 µl 4% paraformaldehyde-PBS until flowcytometry.

Preparation of BMMSCs-CM

Identified BMMSCs from passage three were cultured in 75 ml culture flasks. A serum-free medium made up of DMEM and 10% FBS was used for culture, and flasks were incubated at 5% CO2 and 37°C. After 24 h, the CM was collected, filtered through a 0.22 μm-diameter filter, and centrifuged at 1500g for 10 min, then preserved at -80°C until used.

Determination of cytotoxicity by MTT assay

Harvested BMMSCs-CM was used to treat HepG2 cells at different concentrations: 20%, 40%, 60%, 80%, and 100% which were prepared by diluting the CM using DMEM, each over the course of 24, 48, and 72 h. HepG2 cells grown in DMEM with 10% FBS were used as a negative control. The culture medium was changed every 24 h and the MTT cell viability assay was carried out according to the manufacturer’s instructions. In brief, each test well received 10 μl of a previously prepared 12 mM MTT stock solution and was incubated at 37°C for 4 h. Next, 100 μl of previously prepared SDS-HCl was added to each test well and mixed thoroughly using a pipette, then incubated at 37°C in a humidified chamber for 4 h. Each sample was mixed again and the optical density was measured using a microplate reader (Biotek ELx800, USA) at 570nm. The inhibitory rate of BMMSCs-CM on the viability of HepG2 cells was analyzed using the following formula:

Flowcytometry analysis of apoptosis and cell cycle

FITC Annexin V Apoptosis Detection Kit was used according to the manufacturer’s instructions to assess the influence of BMMSCs-CM on HepG2 cell apoptosis. In brief, HepG2 cells cultured in DMEM and 10% FBS served as a negative control group, while another group of HepG2 cells was treated with 100% BMMSCs CM for 72 h. After treatment, at least 1×106 of HepG2 cells were freshly harvested, washed twice with PBS and resuspended in binding buffer. The cells were then stained with Annexin V-FITC and incubated for at least 15 min in the dark. Following incubation, both the binding buffer and propidium iodide (PI) solutions were added. Finally, HepG2 cells were evaluated for apoptosis using flowcytometry (Biosciences BD Accuri C6 BD, USA). For cell cycle analysis, a cell suspension of 2×106 treated HepG2 cells was prepared using ice cold PBS. The cells were then treated with 50 µl of a 100 µg/ml stock solution of RNase. 400 µl of a PI/Triton X-100 staining solution was added. Cells were incubated at 37°C for 15 min, and then data was acquired on a flow cytometer.

Real time polymerase chain reaction assay of p53 and Bcl-2

Total RNA was extracted from HepG2 cells treated with 100% BMMSCs CM for 72 h using TRIzol reagent according to the manufacturer’s instructions. The RNA concentration was determined using a nanodrop spectrophotometer (Thermo Fisher Nanodrop 2000, USA) after dissolving the RNA pellet in RNase-free water. A Quanti Tects Reverse Transcription Kit was used to make cDNA from extracted RNA according to the manufacturer’s instructions. In brief, 10 µl of 2X RT reaction solution, 1 µl of Quantiscript Reverse Transcriptase enzyme mix solution, and 1 µg of RNA were combined with RNase-free water to make a total volume of 20 µl. The mixture was incubated at 42°C for 15 min and at 95°C for 3 min. The RT-qPCR analysis was carried out using Maxima SYBR green and specific primer pairs of p53, Bcl-2 and β-actin genes, with their sequences illustrated in Table I. β-actin served as the house-keeping gene. The thermal cycling was as follows: 95°C/10 min initial denaturation, followed by 45 cycles of 95°C/10 s, 60°C/15 s, and 72°C/15 s. The Rotor - Gene Q (Qiagen, USA) collected the data automatically and analyzed the value of the cycle threshold (Ct). The 2-ΔΔCt method was used to analyze the relative quantitative data (Livak and Schmittgen, 2001).

Western blotting of p53 and Bcl-2

Whole-cell lysates were prepared from HepG2 cells that had been treated with 100% BMMSCs CM for 72 h. A BCA protein assay kit was used for measuring the protein concentration. Proteins (30µg) were loaded onto 12% sodium dodecyl sulfate–polyacrylamide slab gel for electrophoresis. Before immunodetection, electrolyzed proteins were transferred to a Hybond nylon membrane (GE Healthcare, USA), and then incubated overnight at 4°C with each of the following antibodies separately: anti-p53 primary antibody (1:2000), anti-Bcl-2 primary antibody (1:500), and anti β-actin primary antibody (1:1000). After washing the membrane in TBST, it was incubated at 37°C for 1hr in an appropriate HRP-conjugated secondary antibody (1:2000). The bands were observed by a 1-step TMB-blotting substrate solution. β-actin served as the house-keeping protein. TotalLab analysis software 1.0.1 was used to quantify the bands’ optical density.

Flowcytometric analysis of p53 and Bcl-2

HepG2 cells treated with 100% BMMSCs CM for 72 h were analyzed using flowcytometry for the expression of Bcl-2 and p53 proteins. In brief, 100 µl of cell suspension containing 10⁶ cells/ml was prepared from treated HepG2 cells using TRIS EDTA buffer. Cells were washed with PBS then centrifuged at 2000 rpm for 5 min. The supernatant was discarded, and the produced pellet was resuspended in 100 µl PBS. 7µl of FITC-anti-Bcl-2 antibody and FITC-anti-p53 antibody were added separately, mixed well, and incubated at room temperature in the dark for 30 min. The cells were then washed with PBS, centrifuged, resuspended, and fixed in 200 µl 4% paraformaldehyde-PBS until flowcytometry (Biosciences BD Accuri C6 BD, USA) analysis.

ELISA analysis of TLR4

The human TLR4 kit was used to determine changes in TLR4 concentration in HepG2 cells treated with 100% BMMSCs CM for 72 h. The procedure was carried out as directed by the manufacturer’s instructions. The optical density was read immediately at 450nm using a microplate reader (Biotek ELx800, USA). The Intra-Assay CV%: <10%, and the Inter-Assay CV%: <12%. Further calculations were carried out according to the manufacturer’s instructions and the TLR4 concentrations were determined.

Statistical analysis

One-way ANOVA and Student’s t-test using GraphPad Prism 9.1.0 (GraphPad Software Inc., La Jolla, CA, USA) were used to determine the difference between the groups. Comparison of means was carried out with Dunnett’s Multiple Comparison test. Data were presented as mean ± standard deviation (SD), and significance was declared at P < 0.05.

Results

Characterization of BMMSCs

BMMSCs harvested after the third passage of culture showed a positive capacity for plastic adherence. Microscopic evaluation revealed spindle, fibroblast like morphology with cytoplasmic processes extending in opposite directions. Furthermore, flowcytometric analysis revealed positive expression of BMMSCs specific markers CD44 (96.3%), CD90 (96.1%) and CD105 (98%), and negative expression of hemopoietic and endothelial marker CD34 (94.5%) (Fig. 1).

Effect of BMMSCs on HepG2 cell viability

To determine the effect of BMMSCs-CM on HepG2 cell viability, HepG2 cells were treated with 20%, 40%, 60%, 80%, and 100% BMMSCs-CM for 24, 48, and 72 h. The viability of HepG2 cells was determined using the MTT method. Results confirmed the presence of an inhibitory effect exerted by BMMSCs-CM on HepG2 cells. The inhibitory effect was elevated as the BMMSCs-CM concentration was increased and as the period of treatment was prolonged. All BMMSCs-CM groups (20%, 40%, 60%, 80%, and 100%) showed a significant inhibitory effect when compared to the control group, reaching as high as 48.23% at 100% BMMSCs-CM after 72 h of treatment, and as low as 16.89% at 20% BMMSCs-CM after 24 h of treatment (Fig. 2). Depending on the previous data, 100% BMMSCs-CM for 72h was the treatment of choice for further investigations; as it produced the highest cytotoxic effect on HepG2.

 

 

Effect of BMMSCs-CM on HepG2 cell apoptosis and cell cycle

Flowcytometric detection of apoptosis revealed an increase in the apoptotic % of HepG2 cells after treatment with 100% BMMSCs-CM for 72 h. The apoptotic % of non-treated HepG2 cells was 5.4%, which increased to 26.2% after treatment with 100% BMMSCs-CM for 72 h. The apoptotic % of HepG2 cells treated with BMMSCs-CM was significantly different from that of the non-treated HepG2 cells (P < 0.01) (Fig. 3). Cell cycle analysis using flowcytometry showed a significant increase in Sub-G1 (5.5% to 17.8%) and G0/G1 (38.3% to 67.23%) phases indicating cell cycle arrest in the G0/G1 phase, and a significant decrease in S (40.1% to 15.87%) and G2/M (18.5% to 1.5%) phases of the HepG2 cell cycle after treatment with 100%BMMSCs-CM for 72 h compared to non-treated HepG2 cells (Fig. 4).

 

Effect of BMMSCs-CM on p53 and Bcl-2 mRNA expression levels in HepG2 cells

P53 and Bcl-2 mRNA expression levels were evaluated after treating HepG2 cells with 100% BMMSCs-CM for 72 h. The mRNA expression level of p53 increased significantly in the treated group compared to that of the control group (P < 0.05), while the mRNA expression level of Bcl-2 decreased significantly in the treated group compared to that of the control group (P < 0.05) (Fig. 5).

 

 

Effect of BMMSCs-CM on p53 and Bcl-2 protein levels in HepG2 cells by western blotting

HepG2 cells treated with 100% BMMSCs-CM for 72 h were evaluated by western blotting for p53 and Bcl-2 protein levels. HepG2 cells cultured for 72 h without treatment served as the control group. The results revealed a significant upregulation in p53 protein level in the treated group compared to that of the control group (P < 0.05). However, Bcl-2 protein level was significantly downregulated in the treated group compared to that of the control group (P < 0.01) (Fig. 6).

 

Effect of BMMSCs-CM on p53 and Bcl-2 protein levels in HepG2 cells by flowcytometry

The protein levels of p53 and Bcl-2 were evaluated by flowcytometry after HepG2 cells were treated with 100% BMMSCs-CM for 72 h. HepG2 cells cultured for 72 h without treatment served as the control group. The results revealed a significant upregulation in p53 protein level from 22.87% in the control group to 70.5% in the treated group (P < 0.001). However, Bcl-2 protein level was significantly downregulated from 81.7% in the control group to 19.8% in the treated group (P < 0.001) (Fig. 7).

Effect of BMMSCs-CM on TLR4 concentration in HepG2 cells by ELISA

HepG2 cells were evaluated by ELISA for TLR4 concentration after treatment with 100% BMMSCs-CM for 72 h. HepG2 cells cultured for 72 h without treatment served as the control group. The results revealed a significant reduction in TLR4 concentration from 21.83 ng/ml in the control group to 6.31 ng/ml in the treated group (P < 0.05) (Fig. 8).

 

 

Discussion

MSCs have been the focus of recent investigations for their antitumorigenic effects. They have been reported by multiple studies to inhibit cancer development, including cases of Lewis’ lung carcinoma, B16 melanoma (Maestroni et al., 1999), colon carcinoma (Ohlsson et al., 2003), Kaposi’s sarcoma (Khakoo et al., 2006), lymphoma, insulinoma (Lu et al., 2008), breast cancer (Sun et al., 2009), pancreatic cancer (Kidd et al., 2010) and hepatic cancer, specifically HCC (Qiao et al., 2008). Furthermore, it has been proposed that MSCs-CM contain soluble factors that are involved in tumor suppression (Hou et al., 2014; Serhal et al., 2019). In our experiment, we investigated the in vitro effect of BMMSCs-CM on HepG2, and it clearly showed that BMMSCs-CM can suppress the proliferation of HepG2.

The CM of BMMSCs was cocultured with HepG2 at different concentrations for up to 72 h. The MTT assay revealed a significant reduction in the viability of HepG2 cells, reaching its lowest when cocultured with 100% BMMSCs-CM for 72 h. These findings matched those of (Hou et al., 2014), but our results were more significant, with lower HepG2 cell viability. Further evaluation of the HepG2 cell cycle in our experiment showed cycle arrest in the G0/G1 phase with inhibition of entry into the S phase. These findings were almost indistinguishable from those of Ramasamy et al. (2007), who used MSCs and showed G0/G1 cell cycle arrest, whereas we used BMMSCs-CM instead of the cells themselves. To a similar extent, Khakoo et al. (2006) showed that MSCs were capable of suppressing the development of Kaposi’s sarcoma via cell-cell interactions. However, the results from our MTT and cell cycle assays indicated that direct contact was not required for BMMSCs to exert their inhibitory effect on HepG2 cells, and that BMMSCs-CM was capable of producing the same suppressive effect.

We further investigated the suppressive effect of BMMSCs-CM on hepG2 cells by flowcytometric analysis of HepG2 cell apoptosis. Our findings revealed significant apoptotic activity of HepG2 cells after treatment with 100% BMMSCs-CM for 72 h. It has been demonstrated that BMMSCs coculture with ascitogenous hepatoma cells (H22) causes a dramatic increase in H22 cell apoptosis (Lu et al., 2008), whereas in this current study, BMMSCs-CM was found to exhibit a similar apoptotic effect on HepG2 cells. The activation of several signaling pathways has been implicated in human hepatocarcinogenesis (Villanueva et al., 2007). Their importance stems from their ability to serve as targets for new therapies (Llovet et al., 2008; Miele et al., 2006). Of these, Notch signaling has been reported to play a critical role in HCC (Villanueva et al., 2007). Cantarini et al. (2006) demonstrated overexpression of Notch 1 in all 15 paired HCC human samples, and the evaluation of 87 resected HCC tumors by Gao et al. (2008) revealed upregulation of Notch 1 in 89% of tumor specimens. Furthermore, Notch signaling has been shown to positively regulate cell proliferation in the hepatoma HepG2 cell line (Suwanjunee et al., 2008; Wang et al., 2010). However, in a limited number of tumors such as skin and small lung tumors, Notch signaling was antiproliferative rather than oncogenic (Miele et al., 2006). Several mechanisms have been suggested to explain the oncogenic role of Notch signaling. It was reported that Notch signaling influenced both p53 and Bcl-2, where activated Notch 1 has been negatively associated with p53 transactivation (Kim et al., 2007) and inhibited p53-dependant apoptosis (Nair et al., 2003), and Notch 3 depletion allowed the upregulation of p53 with subsequent suppression of HepG2 cells (Giovannini et al., 2006). On the other hand, activated Notch 1 led to overexpression of Bcl-2 (Ferreira et al., 2012), and the antiapoptotic effect of activated Notch proteins has been attributed to the induction of Bcl-2 (MacKenzie et al., 2004). Overall, Notch activation led to downregulation of p53 and upregulation of Bcl-2, causing enhanced cancer cell survival and increased resistance to apoptosis. MSCs have been reported to both upregulate p53 (Serhal et al., 2019) and downregulate Bcl-2 (Hou et al., 2014). In the present study, p53 and Bcl-2 mRNA and protein expressions were investigated using RT-PCR, flowcytometry, and western blotting, respectively. After treating HepG2 cells with 100% BMMSCs-CM for 72 h, we found significant upregulation of p53 mRNA and protein expression, as well as significant downregulation of Bcl-2 mRNA and protein expression in HepG2 cells. These results can explain the suppressive apoptotic activity that was revealed by the MTT assay, apoptosis analysis, and cell cycle analysis exerted by BMMSCs-CM on HepG2 cells. We suggest that these results might have been caused by the influence of soluble factors present in BMMSCs-CM through their potential involvement in Notch signaling inhibition.

Another important signaling mechanism related to notch signaling is the (Toll Like Receptor 4) TLR4/ (Nuclear factor kappa B) NF-kB pathway, in which activated TLR4 directly stimulates NF-kB (Kawai and Akira, 2007), enhancing cancer cells’ apoptosis resistance and survival (Naugler and Karin, 2008), but when inhibited, apoptosis is more easily triggered. In addition, NF-kB stimulation has been shown to directly activate Notch 1 signaling and further support cancer development (Yao et al., 2007). Seki and Brenner (2008) reported that mice deficient in TLR4 exhibited a much lower frequency of HCC generation. Furthermore, Yang et al. (2015) reported that TLR4 was associated with HCC through activating NF-kB. These reports collectively indicate that TLR4/NF-kB signaling plays a critical role in hepatocarcinogenesis. It was reported by Li et al. (2016) that BMMSCs were able to suppress the TLR4/NF-kB signaling pathway, and in another study, MSCs were found to reduce TLR4 expression in HepG2 cells (Hsiao et al., 2015). In this present study, we found that treating HepG2 cells with 100% BMMSCs-CM for 72 h caused significant TLR4 downregulation in HepG2 cells, which matches the results of previous studies, except we used BMMSCs-CM. These results signify the presence of a role for soluble factors of BMMSCs-CM in TLR4/NF-kB pathway inhibition, rendering cancerous cells less resistant to apoptosis. This aligns with the elevated apoptosis of HepG2 cells by BMMSCs-CM recorded in our current study.

We speculate that the inhibitory effect of BMMSCs-CM on HepG2 cells was possible through the BMMSCs’ secretome, possibly via extracellular vesicles such as exosomes (Hassanzadeh et al., 2021) that potentially interfered with the expression of tumorigenic proteins of HepG2 cells through involvement in multiple signaling pathways. However, the precise fraction(s) of BMMSCs-CM that is responsible for the suppressive effect on cancer cells has yet to be defined. Our limitations in financial support and the scarcity of previous literature on BMMSCs’ secretome have prevented us from describing the specific portion of the secretome responsible for the anti-tumor effects. Additionally, larger group sizes would have provided us with a more accurate representation. Therefore, future investigations into the BMMSCs’ secretome are recommended to specify the exact role of particular fractions of BMMSCs-CM on cancer cells.

Conclusions

The present study shows that BMMSCs-CM had a direct suppressive effect on HepG2 cell proliferation, observed by a decrease in cell viability, induction of apoptosis and cell cycle arrest with elevated expression of apoptotic genes and reduced expression of antiapoptotic genes through possible involvement in multiple signaling pathways such as TLR4 signaling pathway, making BMMSCs-CM a potent candidate for cancer treatment.

Statement of conflict of interest

The authors have declared no conflict of interest.

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