|Year : 2022 | Volume
| Issue : 5 | Page : 540-548
Mannose inhibits the growth of prostate cancer through a mitochondrial mechanism
Yu-Lin Deng1, Ren Liu2, Zhou-Da Cai3, Zhao-Dong Han4, Yuan-Fa Feng5, Shang-Hua Cai6, Qing-Biao Chen7, Jian-Guo Zhu8, Wei-De Zhong9
1 Guangdong Provincial Institute of Nephrology, Nanfang Hospital, Southern Medical University, Guangzhou 510515, China
Department of Andrology, Guangzhou First People's Hospital, School of Medicine, South China University of Technology, Guangzhou 510180, China
Department of Urology, Guangdong Key Laboratory of Clinical Molecular Medicine and Diagnostics, Guangzhou First People's Hospital, School of Medicine, South China University of Technology, Guangzhou 510180, China
Urology Key Laboratory of Guangdong Province, The First Affiliated Hospital of Guangzhou Medical University, Guangzhou Medical University, Guangzhou 510230, China
Department of Urology, Guizhou Provincial People's Hospital, The Affiliated Hospital of Guizhou Medical University, Guiyang 550002, China
Department of Urology Surgery, Affiliated Foshan Hospital of Southern Medical University, Foshan 528000, China
|Date of Submission||11-Jun-2021|
|Date of Acceptance||17-Nov-2021|
|Date of Web Publication||04-Feb-2022|
Department of Urology, Guizhou Provincial People's Hospital, The Affiliated Hospital of Guizhou Medical University, Guiyang 550002
Guangdong Provincial Institute of Nephrology, Nanfang Hospital, Southern Medical University, Guangzhou 510515; Department of Urology, Guangdong Key Laboratory of Clinical Molecular Medicine and Diagnostics, Guangzhou First People's Hospital, School of Medicine, South China University of Technology, Guangzhou 510180
Source of Support: None, Conflict of Interest: None
The limited treatment options for advanced prostate cancer (PCa) lead to the urgent need to discover new anticancer drugs. Mannose, an isomer of glucose, has been reported to have an anticancer effect on various tumors. However, the anticancer effect of mannose in PCa remains unclear. In this study, we demonstrated that mannose inhibits the proliferation and promotes the apoptosis of PCa cells in vitro, and mannose was observed to have an anticancer effect in mice without harming their health. Accumulation of intracellular mannose simultaneously decreased the mitochondrial membrane potential, increased mitochondrial and cellular reactive oxygen species (ROS) levels, and reduced adenosine triphosphate (ATP) production in PCa cells. Mannose treatment of PCa cells induced changes in mitochondrial morphology, caused dysregulated expression of the fission protein, such as fission, mitochondrial 1 (FIS1), and enhanced the expression of proapoptotic factors, such as BCL2-associated X (Bax) and BCL2-antagonist/killer 1 (Bak). Furthermore, lower expression of mannose phosphate isomerase (MPI), the key enzyme in mannose metabolism, indicated poorer prognosis in PCa patients, and downregulation of MPI expression in PCa cells enhanced the anticancer effect of mannose. This study reveals the anticancer effect of mannose in PCa and its clinical significance in PCa patients.
Keywords: mannose; mannose phosphate isomerase; metabolism; mitochondria; prostate cancer
|How to cite this article:|
Deng YL, Liu R, Cai ZD, Han ZD, Feng YF, Cai SH, Chen QB, Zhu JG, Zhong WD. Mannose inhibits the growth of prostate cancer through a mitochondrial mechanism. Asian J Androl 2022;24:540-8
|How to cite this URL:|
Deng YL, Liu R, Cai ZD, Han ZD, Feng YF, Cai SH, Chen QB, Zhu JG, Zhong WD. Mannose inhibits the growth of prostate cancer through a mitochondrial mechanism. Asian J Androl [serial online] 2022 [cited 2022 Nov 29];24:540-8. Available from: https://www.ajandrology.com/text.asp?2022/24/5/540/337220
Yu-Lin Deng, Ren Liu
These authors contributed equally to this article.
| Introduction|| |
Prostate cancer (PCa) is the most common malignancy and the second leading cause of cancer-related death in males. Despite the benefits of androgen deprivation targeting androgen receptor (AR) signaling in the early stages of the disease, many tumors recur in an androgen-independent form, accompanied by an increased mortality rate. Therefore, identifying a more active and less toxic antitumor agent is a major goal in the development of new targeted therapeutic strategies. Studies have demonstrated that tumorigenesis depends on the metabolic reprogramming that induces cancer cells to proliferate even under stress conditions.
Mannose is a natural monosaccharide and an isomer of glucose. Studies indicated that mannose can impair the growth of various tumors., Mannose phosphate isomerase (MPI) is the key enzyme in mannose metabolism. The expression of MPI is related to the cellular content and the anticancer effect of mannose. To date, the anticancer effect of mannose in PCa remains unclear. Here, we aim to investigate the anticancer effect of mannose in PCa and evaluate its possible application in PCa patients.
In this study, we found that mannose can inhibit the function of and induce morphological changes in mitochondria in PCa cells, thus inhibiting the growth and promoting the apoptosis of PCa cells. Furthermore, we preliminarily verified that mannose may have better antitumor effects in PCa patients with worse pathological classification.
| Materials and Methods|| |
The human PCa cell lines DU145 and PC3 were obtained from the American Type Culture Collection (ATCC® HTB-81 and ATCC® CRL1435, Manassas, VA, USA) and grown in Dulbecco's modified Eagle medium (DMEM; C11965500BT, Gibco, Paisley, UK) containing 10% fetal bovine serum, streptomycin, and penicillin. The normal human prostate epithelial cell line RWPE-1 was obtained from iCell (Shanghai, China) and grown in keratinocyte serum free medium (SFM; iCell-0019, iCell). Cells were incubated in a humidified, 5% CO2 atmosphere at 37°C. The detailed information of reagents used in this study is shown in the [Supplementary Table 1 [Additional file 1]].
Measurement of the half-maximal inhibitory concentration (IC50) of mannose and cell proliferation assay
The IC50 of mannose (M2069, Sigma-Aldrich, Saint Louis, MO, USA) in PCa cells was determined and cell proliferation assays were conducted using a Cell Counting Kit-8 (CCK-8; CCK8-500T, Meilunbio, Dalian, China). For the IC50 assay, cells were plated in 96-well plates and cultured with multiple mannose concentrations for 72 h. The mannose concentrations in DMEM were 25 mmol l−1 and 50 mmol l−1 for DU145 and PC3, respectively, based on the IC50 values.
For cell proliferation, cells were plated in 96-well plates with a normal medium with or without mannose supplementation for 4–96 h. DMEM containing 10% CCK-8 was replaced in each well and incubated for another 2 h. The absorbance of the medium at a wavelength of 450 nm was determined using a microplate reader (Bio-Rad, Hercules, CA, USA).
Colony formation assay
Cells were plated in 6-well plates and maintained in medium with or without mannose supplementation, and replaced every 2 days, for a total of 10 days. Then, cells were fixed and stained with 0.1% crystal violet for 2 h. The siMPI-DU145 and siMPI-PC3 cells were retransfected every 72 h.
Cells were plated in 6-well plates, cultured in medium with or without mannose for 48 h, and resuspended in binding buffer. Then, cells were stained with Annexin V-fluorescein isothiocyanate (FITC) and propidium iodide (PI) containing RNase A (AP105, MultiSciences, Hangzhou, China). After staining, cells were harvested and subjected to a flow cytometer (BD FACSVerse, BD Biosciences, Franklin Lakes, NJ, USA). FlowJo software (BD Biosciences) was used to analyze the data.
Four-week-old male nude mice (Experimental Animal Center of Sun Yat-sen University, Guangzhou, China) were raised under specific pathogen-free conditions. Animal handling and protocols were approved by the Institutional Animal Care and Use Committee of Guangzhou Medical University (Guangzhou, China) according to the National Research Council's guidelines. The certificate number of the animal breeder was 2018217474. A total of 5 × 106 DU145 cells were injected subcutaneously. Mice were randomly divided into the control group and mannose group (5 mice per group). Mice received mannose (20%) by oral gavage (200 μl) every 2 days starting on the 12th day. The mouse weight and tumor volume (length [mm] × width2 [mm2] × 1/2) were measured every 2 days. When the mice were euthanized, the tumors and organs (i.e., liver, kidney, and pancreas) were harvested to identify the effect of mannose on mouse health. The effect of mannose on the growth of PCa tumors in vivo was determined by the formula (tumor final volume [mm3] − initial volume [mm3]).
5,5', 6, 6'-tetrachloro-1,1', 3, 3'-tetraethyl-imidacarbocyanine (JC-1) staining
The mitochondrial membrane potential (MMP) was evaluated by JC-1 staining (M8650, Solarbio, Beijing, China). Cells were plated in 6-well plates and cultured in medium with or without mannose for 48 h. Cells were incubated for 30 min for mitochondrial staining with JC-1, and nuclei were then stained with Hoechst 33342 (100 nmol l−1; C1028, Beyotime, Shanghai, China) for 10 min. After staining, cells were observed under a confocal microscope (LSM880, Zeiss, Jena, Germany). JC-1 aggregates (red fluorescence) indicate a normal MMP, while JC-1 monomers (green fluorescence) indicate a decreased MMP.
Rhodamine 123 staining
The MMP was also measured by rhodamine 123 staining (HY-D8016, MCE, Monmouth Junction, NJ, USA). Cells were cultured in the same way as JC-1 staining and incubated with rhodamine 123 (200 ng ml−1) for 30 min. Cells were harvested and subjected to BD FACSVerse. FlowJo software was used to calculate the mean fluorescence intensity (MFI) of each sample. The rhodamine 123 MFI increases when the MMP decreases.
Quantification of mitochondrial and cellular reactive oxygen species (ROS)
Cells were cultured in the same way as JC-1 staining and incubated with MitoSOX red (5 μmol l−1; M36008, Invitrogen, Waltham, MA, USA) or DCFH-DA (10 μmol l−1; D6883, Sigma-Aldrich) for 30 min. Cells were harvested and subjected to BD FACSVerse. FlowJo software was used to calculate the MFI of each sample.
Measurement of adenosine triphosphate (ATP) generation
The ATP content was measured with an Enhanced ATP Assay Kit (S0027, Beyotime). Cells were cultured in the same way as JC-1 staining. Tumors were harvested from xenograft model mice. Cells were harvested and centrifuged at 12 000g and 4°C for 5 min by high speed refrigerated centrifuge (Sorvall Legend Micro 17R, ThermoFisher, Waltham, MA, USA). Then, 100 μl of ATP detection solution and 20 μl of the cell supernatant were added to a 96-well plate, and ATP was detected using a multifunctional microplate reader (Varioskan LUX, ThermoFisher). ATP content was calculated according to the standard curve.
Cells were cultured in the same way as JC-1 staining. Mitochondria in PCa cells were stained with MitoTracker Red CMXRos (100 nmol l−1; C1049, Beyotime) for 30 min. Then, cells were observed under a confocal microscope (LSM880, Zeiss).
Transmission electron microscopy
Cells were cultured in the same way as JC-1 staining. The protocols were performed, as previously described. Quantification of the mitochondrial volume was performed by first drawing a contour of the cross-section of each mitochondrion and then calculating the enclosed area in ImageJ software (National Institutes of Health, Bethesda, MD, USA).
Western blot analysis
Protein extraction and western blot analysis were performed, as previously described. The following antibodies were used at a dilution of 1:1000 unless otherwise stated: rabbit anti-MPI (ab154198, Abcam, Cambridge, UK), rabbit anti-mitofusin 1 (MFN1; 13798-1-AP, Proteintech, Chicago, IL, USA), rabbit anti-MFN2 (12186-1-AP, Proteintech), rabbit anti-fission, mitochondrial 1 (FIS1; 10956-1-AP, Proteintech), rabbit anti-dynamin related protein 1 (DRP1; 26187-1-AP, Proteintech), rabbit anti-BCL2-associated X (Bax; 9942T, CST, Boston, MA, USA), rabbit anti-BCL2-antagonist/killer 1 (Bak; 9942T, CST), mouse anti-β-actin (1:5000; ab8227, Abcam), and mouse anti-glyceraldehyde-3-phosphate dehydrogenase (GAPDH; 1:10 000; 60004-1-AP, Proteintech).
Measurement of mannose concentration
PCa cells were cultured in the same way as JC-1 staining and harvested. Tumors were harvested from xenograft model mice. The assay was performed with a Human Mannose ELISA Kit (ZK-H594, ZIKER, Shenzhen, China) following the manufacturer's instructions, and the optical density was measured at a 450 nm wavelength using a multifunctional microplate reader. Mannose concentrations were calculated according to the standard curve.
Patients and tissues
A PCa tissue microarray (TMA; PR803d, Biomax, Derwood, MD, USA) was applied for immunohistochemical analysis. Patients did not receive chemotherapy or radiotherapy before surgery. Detailed information on the TMA cohort is available in the supplementary materials. PCa tissues and paired clinical data were collected from 498 patients with information in the TCGA database (TCGA-PRAD, The Cancer Genome Atlas-Prostate Adenocarcinoma: https://www.cancer.gov/tcga), and correlations between the MPI mRNA expression level and patients' clinicopathological features were assessed. This study was approved by the Ethics Committee of Guangzhou First People's Hospital (approval No. 82072813).
MPI protein expression in our TMA cohort was assessed by IHC, as previously described. An IHC kit (KIT-9730, MXB, Fuzhou, China) and rabbit anti-MPI antibody (1:400; ab154198, Abcam) were used for immunostaining following the manufacturer's instructions.
Overexpression of FIS1 in PCa cells
PCa cells were transfected with pcDNA-FIS1 or pcDNA (GenePharma, Shanghai, China) using Lipofectamine 3000 (L3000008, Invitrogen, Waltham, MA, USA) for 72 h. After transfection, cells were collected.
Silencing of MPI using small interfering RNA (siRNA)
PCa cells were transfected with human MPI siRNA or control siRNA (GenePharma, Shanghai, China) using GP-transfect-Mate (GenePharma) for 72 h. Cells were collected, and silencing was confirmed by western blot.
All of the statistical analyses were performed with SPSS Statistics 20 (IBM, New York, NY, USA) and GraphPad Prism 8 (GraphPad Software, San Diego, CA, USA). Continuous variables were expressed as means ± standard deviation (s.d.). Student's t-test or analysis of variance (ANOVA) was used to determine the statistical significance of our quantitative data. The Kaplan–Meier method was used for survival analysis. The optimal cutoff value was determined using the R package “survminer”. Differences with P < 0.05 were considered to be statistically significant.
| Results|| |
Effect of mannose on the growth of PCa cells in vitro
The IC50 values of mannose were 67.42 mmol l−1 (95% confidence interval [CI]: 57.680–78.960) and 177.00 mmol l−1 (95% CI: 166.800–188.000) in DU145 and PC3 cells, respectively [Figure 1]a and [Figure 1]b. After mannose treatment, the intracellular mannose concentrations increased in PCa cells (P < 0.01; [Figure 1]c). The inhibitory effects of mannose on DU145 and PC3 were observed in the growth curve 72 h after mannose treatment (DU145: P < 0.01, and PC3: P < 0.05; [Figure 1]d and [Figure 1]e). Mannose reduced the number of colonies (P < 0.01; [Figure 1]f and [Figure 1]g) of PCa cells. The apoptosis rate increased after mannose treatment (DU145: P < 0.05, and PC3: P < 0.01; [Figure 1]h and [Figure 1]i). Mannose had no effect on the growth or colony formation of RWPE-1 [Supplementary Figure 1 [Additional file 2]]a and [Supplementary Figure 1]b.
|Figure 1: Mannose inhibited the proliferation and induced the apoptosis of PCa cells. The IC50 of mannose in (a) DU145 and (b) PC3 cells was determined using a CCK-8 assay. (c) Intracellular mannose concentration in PCa cells. Cell proliferation of (d) DU145 and (e) PC3 was assessed using growth curves, respectively. (f) Colony formation assays were performed and (g) colony numbers were counted in PCa cells. (h) Flow cytometric analysis was used to assess (i) the apoptosis rate of PCa cells. *P < 0.05, **P < 0.01. NC: PCa cells cultured in normal medium. MAN: PCa cells cultured in normal medium with 25 mmol l−1 mannose for DU145 or with 50 mmol l−1 mannose for PC3. PCa: prostate cancer; IC50: the half-maximal inhibitory concentration; CCK-8: Cell Counting Kit-8 ; AAD: Aminoactinomycin D; APC: Allophycocyanin.|
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Effect of mannose on the growth of PCa cells in vivo
In the xenograft tumor assay, five nude mice per group received a subcutaneous injection of DU145 cells. However, the xenograft tumor in one nude mouse did not grow after mannose treatment. Therefore, the volume of this tumor was not included in our statistical analysis. Our results showed that oral mannose administration inhibited PCa tumor growth in nude mice (P < 0.01; [Figure 2]a, [Figure 2]b, [Figure 2]c, [Figure 2]d), while oral administration of mannose had no effect on body weight [Figure 2]g or the weights of the liver, kidney, and pancreas [Figure 2]h in mice. Intratumoral mannose concentration increased (P < 0.01; [Figure 2]e) and the ATP content decreased (P < 0.01; [Figure 2]f) in the mannose group.
|Figure 2: Mannose inhibited tumor growth in a PCa xenograft model without affecting mice health. (a) Subcutaneous tumors from the xenograft model with DU145 cells. (b) Tumor growth was monitored for 30 days after mannose treatment. (c) The volume of tumor growth. (d) The weight of the tumors. (e) Intratumoral mannose concentration and (f) ATP content in subcutaneous tumors. The weights of (g) mice and (h) major metabolic organs. **P < 0.01. NC: PCa cells cultured in normal medium. MAN: PCa cells cultured in normal medium with 25 mmol l−1 mannose for DU145 or with 50 mmol l−1 mannose for PC3. PCa: prostate cancer; ATP: adenosine triphosphate.|
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Mannose disrupted mitochondrial function, led to ROS overproduction, and activated Bax/Bak in PCa cells
JC-1 staining showed an increase in JC-1 monomers and a decrease in JC-1 aggregates after mannose treatment [Figure 3]a, suggesting a reduction in the MMP. The rhodamine 123 assay showed a decreased MMP in PCa cells treated with mannose (P < 0.01; [Figure 3]b, consistent with the results of JC-1 staining. Mannose decreased the ATP content in PCa cells (P < 0.01; [Figure 3]c but had no effect in RWPE-1 [Supplementary Figure 1]c. Mannose increased both the mitochondrial (P < 0.01; [Figure 3]d) and cellular (P < 0.01; [Figure 3]e) ROS levels. Western blot analysis [Figure 3]f indicated that the expression of Bax (DU145: P < 0.05, and PC3: P < 0.01; [Figure 3]g) and Bak (P < 0.01; [Figure 3]g) was enhanced in PCa cells after mannose treatment.
|Figure 3: Mannose disrupted mitochondrial function, led to ROS overproduction, and activated Bax/Bak in PCa cells. (a) JC-1 staining and (b) rhodamine 123 staining were used to assess the MMP in DU145 and PC3 cells. (c) The ATP content in cells. (d) Mitochondrial ROS and (e) cellular ROS levels in cells. (f and g) The protein expression of Bax and Bak in cells. *P < 0.05, **P < 0.01. NC: PCa cells cultured in normal medium. MAN: PCa cells cultured in normal medium with 25 mmol l−1 mannose for DU145 or with 50 mmol l−1 mannose for PC3. JC-1: 5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethyl-imidacarbocyanine; Bax: BCL2-associated X; Bak: BCL2-antagonist/killer 1; ROS: reactive oxygen species; MMP: mitochondrial membrane potential; ATP: adenosine triphosphate; PCa: prostate cancer.|
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Mannose disrupted the balance of mitochondrial dynamics in PCa cells
Confocal microscopy revealed that mannose treatment resulted in the elongation of mitochondria in PCa cells [Figure 4]a. Transmission electron microscopy was used to further observe the structure of mitochondria and showed an increase in the mitochondrial cross-sectional area with mannose treatment (P < 0.01; [Figure 4]b).
|Figure 4: Mannose disrupted the balance of mitochondrial dynamics in PCa cells. (a) Mitochondria stained with MitoTracker Red were observed by confocal microscopy. (b) Mitochondrial structure under a transmission electron microscopy, and the mitochondrial cross-sectional area was quantified. (c) The protein expression of FIS1 in cells. Upregulated (d) FIS1 and (e) increased ATP content in PCa cells. *P < 0.05, **P < 0.01. NC: PCa cells cultured in normal medium. MAN: PCa cells cultured in normal medium with 25 mmol l−1 mannose for DU145 or with 50 mmol l−1 mannose for PC3. ATP: adenosine triphosphate; FIS1: fission, mitochondrial 1; PCa: prostate cancer.|
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Western blot analysis [Figure 4]c indicated that the expression of the mitochondrial fission protein FIS1 decreased in PCa cells (DU145: P < 0.01 and PC3: P < 0.05; [Figure 4]c). Cellular ATP content increased (P < 0.01; [Figure 4]e), while FIS1 overexpressed in PCa cells (P < 0.01; [Figure 4]d). No changes in MFN1, MFN2, or DRP1 expression were observed with mannose treatment [Supplementary Figure 2 [Additional file 3]]a and [Supplementary Figure 2]b.
Downregulated MPI expression enhanced the anticancer effect of mannose on PCa cells
MPI was silenced in PCa cells (P < 0.01; [Figure 5]a and [Figure 5]b). After silencing MPI, the intracellular mannose concentration increased (P < 0.01; [Figure 5]c) and the ATP content decreased (P < 0.01; [Figure 5]d) with mannose treatment. The growth curves showed that in MPI-downregulated cells, the anticancer effect of mannose was more obvious within 48 h in DU145 and appeared after 72 h in PC3 (P < 0.05; [Figure 5]e). In addition, mannose treatment more obviously reduced the number of colonies of MPI-downregulated PCa cells (P < 0.01; [Figure 5]f).
|Figure 5: Downregulation of MPI expression enhances the anticancer effect of mannose. The expression of MPI in human prostate cancer tissues and its prognostic value. (a and b) The expression of MPI was silenced by siRNA-MPI and verified by western blotting. siRNA-MPI with different base sequences including si-1, si-2 and si-3 were used for downregulating the MPI expression in PCa cells. According to the degree of down-regulation of MPI protein, si-3 and si-2 with the best interference effect were applied to DU145 and PC3 cells, respectively. (c) Intracellular mannose concentration and (d) ATP content in cells. (e) Growth curves and (f) colony formation assays of cells. (g) The IHC scores for MPI expression in PCa tissues. (h) Kaplan–Meier curves of BCR-free survival and (i) overall survival for the low and high MPI expression groups of patients in the TCGA-PRAD dataset. *P < 0.05, **P < 0.01. NC: PCa cells cultured in normal medium. MAN: PCa cells cultured in normal medium with 25 mmol l−1 mannose for DU145 or with 50 mmol l−1 mannose for PC3. MPI: mannose phosphate isomerase; si: siRNA, small interfering RNA; IHC: immunohistochemistry; PCa: prostate cancer; BCR: biochemical recurrence; TCGA-PRAD: The Cancer Genome Atlas-Prostate Adenocarcinoma; GAPDH: glyceraldehyde-3-phosphate dehydrogenase; TMA: tissue microarray; ATP: adenosine triphosphate.|
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MPI protein and mRNA expression in human PCa tissues
The expression of MPI in PCa tissues was investigated by IHC [Supplementary Figure 3 [Additional file 4]]. The mean IRS of MPI expression in PCa of GS ≥ 8 and GS ≤ 7 was 7.563 and 10.000 in the TMA chort, respectively. (P = 0.003; [Figure 5]g). In addition, the results of The Cancer Genome Atlas Prostate Adenocarcinoma (TCGA-PRAD) analysis indicated that the mean MPI mRNA expression levels in PCa tissues of GS ≥ 8 and GS ≤ 7 were 5.995 and 6.278, respectively (P < 0.001; [Table 1]).
|Table 1: Association of mannose phosphate isomerase expression with clinicopathological characteristics of patients with prostate cancer in the TMA and TCGA-PRAD|
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Reduced MPI expression is associated with aggressive progression and poor prognosis of PCa
The associations between MPI expression and clinicopathological characteristics of PCa patients based on our TMA data and TCGA-PRAD database analysis are shown in [Table 1]. Low MPI expression in PCa tissues was associated with high Gleason scores (IHC data: P = 0.003, TCGA-PRAD database: P < 0.001), advanced pathological stage (TCGA-PRAD database: P < 0.001), and positive metastasis (TCGA-PRAD database: P < 0.001).
Survival analysis was performed using the TCGA-PRAD database. Patients were stratified into a high-expression group and a low-expression group based on the optimal cutoff value (cutoff value = 5.940; [Supplementary Figure 4 [Additional file 5]]a) for MPI expression. Kaplan–Meier analysis showed that patients in the low-expression group had significantly worse BCR outcomes than those in the high-expression group (HR = 0.455, 95% CI: 0.250–0.830, P = 0.003; [Figure 5]h). Kaplan–Meier analysis also suggested that there was no statistically significant difference in OS between the high-expression and low-expression groups (HR = 0.411, 95% CI: 0.110–1.610, P = 0.144; [Figure 5]i) using the optimal cutoff value (cutoff value: 6.000; [Supplementary Figure 4]b).
| Discussion|| |
Most PCa patients develop androgen resistance accompanied by poor therapeutic effects; thus, a new potential therapy is urgently needed. Metabolic reprogramming is a major hallmark of cancer. In normal prostatic peripheral zone epithelial cells, the tricarboxylic acid (TCA) cycle is halted in mitochondria. PCa cells reversed this phenotype and the TCA cycle is activated.
Mannose has shown potential therapeutic properties in a variety of cancers.,, We found that mannose can inhibit the growth of PCa cells. Furthermore, mannose can regulate metabolic reprogramming of osteosarcoma cells., Similar to these results, we found mannose-induced metabolic changes in PCa cells. After mannose treatment, decreased mitochondrial membrane potential indicated mitochondrial dysfunction, resulting in a decrease in ATP production, suggesting that mannose inhibits mitochondrial ATP production in PCa cells.
Accumulated intracellular mannose inhibits the growth of osteosarcoma and enhances the chemotherapeutic effect of doxorubicin. We found that mannose accumulated in PCa cells and tumors treated with mannose. Furthermore, silencing MPI increased the intracellular mannose concentration and enhanced the anticancer effect of mannose on PCa, consistent with a previous study. These results suggest that MPI plays a role in promoting intracellular accumulation of mannose, thus inhibiting PCa cell proliferation.
ROS are mainly produced when mitochondria consume oxygen. ROS are toxic to cancer cells when ROS production exceeds the ROS scavenging ability. Aberrant elevated ROS can be achieved with cytotoxic stimulation, and we observed that after mannose treatment, the mitochondrial and cellular ROS levels in PCa cells significantly increased, while the growth of PCa cells was inhibited and their apoptosis was promoted. These results suggest that intracellular accumulation of mannose can lead to excessive production of ROS and toxic effects on PCa cells. Overproduction of ROS may also affect the activity of apoptotic effectors. Bax and Bak are proapoptotic proteins that play a core role in mitochondrial membrane permeabilization and apoptotic signaling. Upon cytotoxic stress, Bax and Bak disrupt the mitochondrial outer membrane to allow the release of proapoptotic factors into the cytosol, thus inducing the apoptosis of cells. We found upregulated expression of Bax and Bak and increased apoptosis in PCa cells under mannose treatment, suggesting that mannose induced apoptosis in PCa cells via the proapoptotic signaling of Bax and Bak.
Mitochondria are highly dynamic organelles, and their morphology is determined by mitochondrial dynamics through the interplay of fusion and fission. The main mediator of mitochondrial fission is DRP1, which is recruited from the cytoplasm by FIS1 and then induces mitochondrial division. Cellular metabolic state can affect the balance of mitochondrial dynamics. Changes in mitochondrial dynamics-related proteins are accompanied by cellular metabolic changes and have been observed in bladder cancer cells. It was shown that miR-483-5p controls mitochondrial fission by targeting FIS1. Deletion of FIS1 can lead to the elongation and swelling of mitochondria. After mannose stimulation, the mitochondrial morphology became increasingly swollen and elongated along with the downregulation of FIS1. Besides, the ATP content increased in FIS1-overexpressing PCa cells under mannose treatment. Therefore, we considered that these changes in mitochondria were due to the downregulation of FIS1, which led to dysregulation of mitochondrial division under mannose treatment, although the mechanism has yet to be determined. Studies suggest that inhibiting the fission of mitochondria can inhibit the growth of cancer cells. In contrast, increasing mitochondrial fission can inhibit mitochondria-dependent apoptosis, promote the proliferation of liver cancer cells, and promote the migration and invasion of breast cancer cells. The role of mitochondrial fission in apoptosis is still controversial;, however, it is widely believed that dynamin related protein 1 (DRP1) is not required for activation of Bax and Bak., In addition, we observed increased apoptosis of PCa cells without DRP1 upregulation under mannose treatment, consistent with previous findings.
Consistent with the results of a relevant study on osteosarcoma, silencing MPI expression enhanced the anticancer effect of mannose on PCa. Moreover, our analysis indicated that low MPI expression in PCa tissues was associated with high Gleason scores, advanced pathological classification, and poor clinical prognosis of PCa patients. This suggests that mannose may have an important potential therapeutic effect in advanced PCa patients.
In summary, our findings demonstrate that mannose can effectively inhibit the growth and promote the apoptosis of PCa cells through a change in mitochondrial function and morphology and a ROS-activated Bax- and Bak-dependent mitochondrial mechanism. Long-term oral mannose administration can inhibit the growth of PCa cells in nude mice without affecting their health. Moreover, MPI has important prognostic significance in PCa patients. Silencing MPI can increase the intracellular mannose concentration and enhance the anticancer effect of mannose in PCa. Thus, mannose may be used as a potential therapeutic agent for PCa.
| Author Contributions|| |
YLD performed the cellular studies and the statistical analysis. RL performed the IHC assays and the statistical analysis. ZDC performed the xenograft model studies and the statistical analysis. YLD, RL, and ZDC participated in drafting the manuscript. ZDH and YFF performed the bioinformatic analysis. SHC and QBC participated in the cellular studies. WDZ and JGZ conceived of the study, participated in its design and coordination, and helped to revise the manuscript. All authors read and approved the final manuscript.
| Competing Interests|| |
All authors declare no competing financial interests.
| Acknowledgments|| |
We thank Zhi-Duan Cai, Jian-Heng Ye, Xue-Jin Zhu, Yi-Xun Zhang, Yu-Xiang Liang, Yang-Jia Zhuo, Ying-Ke Liang, and Shao-You Liu from the Department of Urology, Guangdong Key Laboratory of Clinical Molecular Medicine and Diagnostics, Guangzhou First People's Hospital, School of Medicine, South China University of Technology (Guangzhou, China), for supporting the assay performance. We also thank Jian-Heng Ye and Yu-Xiang Liang for their financial support. This work was supported by grants from the National Natural Science Foundation of China (No. 82072813), Natural Science Foundation of Guangdong Province (No. 2020A1515010473 and No. 2018A030313668), and China Postdoctoral Science Foundation (No. 2020M682666).
Supplementary Information is linked to the online version of the paper on the Asian Journal of Andrology website.
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