ETM Experimental and Therapeutic Medicine 1792-0981 1792-1015 D.A. Spandidos 10.3892/etm.2017.4702 ETM-0-0-4702 Articles MicroRNA-33b inhibits cell proliferation and glycolysis by targeting hypoxia-inducible factor-1α in malignant melanoma ZhaoYue 1 WuCuiling 2 LiLina 3 Department of Dermatology, Heping Hospital of Changzhi Medical College, Changzhi, Shanxi 046000, P.R. China Department of Biochemistry, Changzhi Medical College, Changzhi, Shanxi 046000, P.R. China Department of Pathology, Changzhi Medical College, Changzhi, Shanxi 046000, P.R. China Correspondence to: Dr Lina Li, Department of Pathology, Changzhi Medical College, 161 Jiefang East Road, Changzhi, Shanxi 046000, P.R. China, E-mail: linali2013@sina.com 08 2017 28 06 2017 14 2 1299 1306 22022016 24022017 Copyright: © Zhao et al. 2017 This is an open access article distributed under the terms of the Creative Commons Attribution-NonCommercial-NoDerivs License, which permits use and distribution in any medium, provided the original work is properly cited, the use is non-commercial and no modifications or adaptations are made.

Malignant melanoma (MM) is the most aggressive type of skin cancer. MicroRNA (miR) has been implicated in the development and progression of MM; however, their underlying mechanism of action remains largely unknown. The present study aimed to investigate the role of miR-33b in MM. Reverse transcription-quantitative polymerase chain reaction data indicated that the expression of miR-33b was significantly reduced (P<0.01) in MM cell lines, including WM35, WM451 and SK-MEL-1, when compared with human melanocyte cells. Subsequently, WM451 and SK-MEL-1 cells were transfected with an miR-33b mimic or inhibitor. MTT assay data demonstrated that the viability of MM cells markedly decreased following miR-33b overexpression; however, viability was markedly upregulated following miR-33b knockdown. Additionally, the glycolysis level was examined. Results demonstrated that glucose consumption and lactic acid production were significantly downregulated (P<0.01) after miR-33b upregulation, whereas these levels significantly increased in MM cells transfected with miR-33b inhibitor (P<0.01), suggesting that miR-33b negatively mediates the glycolysis level in MM cells. Bioinformatics indicated that hypoxia-inducible factor (HIF)-1α was a putative target gene of miR-33b, and this was confirmed by a luciferase reporter assay, which demonstrated that miR-33b was able to directly bind to the 3′ untranslated region of HIF-1α mRNA. Furthermore, the expression of HIF-1α was negatively regulated by miR-33b at the post-transcriptional level in MM cells. Overexpression of HIF-1α reversed the inhibitory effect of miR-33b on the proliferation and glycolysis in MM cells. Finally, the results of the present study demonstrated that hexokinase 2 and lactate dehydrogenase-A may be involved in miR-33b/HIF-1α mediated glycolysis in MM cells. In conclusion, these results suggest that miR-33b inhibits cell proliferation and glycolysis by targeting HIF-1α in MM.

 melanoma microRNA proliferation glycolysis hypoxia-inducible factor-1α Introduction

Malignant melanoma (MM) is the most aggressive form of skin cancer (1). Despite the fact that significant progress has been made in the early diagnosis and treatment of this disease, the prognosis of MM remains poor, predominantly due to its recurrence and metastasis (2). Therefore, it is necessary to improve understanding of the molecular mechanisms involved in the development and progression of MM.

Glycolysis is the most common metabolic pathway of cancer cells. In tumors, the metabolism of glucose is largely fermentative with increased production of lactate, even when oxygen levels are adequate (3). Glycolysis provides tumor cells with energy and molecules, including ATP, fatty acids and nucleotides, thus ensuring the survival, rapid growth and proliferation of tumor cells under hypoxic and anoxic conditions (4,5). Furthermore, low levels of oxygen may induce the expression of hypoxia-inducible factor (HIF) during tumor progression, enhancing the glycolytic metabolism in cancer cells (6,7). It has been determined that inhibition of HIF-1á-mediated signaling drives MM toward mitochondrial oxidative metabolism, enhancing the therapeutic activity of pro-oxidants (8). Therefore, it has been suggested that glycolysis may be an effective target to treat cancer, including MM (9,10).

Recently, it has been demonstrated that microRNA (miR) may improve the diagnosis and treatment of cancer, such as MM (11). These small non-coding RNA directly bind to the 3′ untranslated region (UTR) of their target mRNA and suppress gene expression by inducing mRNA degradation or translation inhibition (12). miRs may regulate various cancer-related genes, including oncogenes and tumor suppressors (3). It has been reported that the aberrant activation of miR-148, miR-155, miR-182, miR-200c, miR-211, miR-214, miR-221 and miR-222 are associated with MM-associated genes, such as microphthalmia-associated transcription factor, receptor tyrosine kinase c-KIT and transcription factor AP-2 (11). Recently, it has been demonstrated that miR-33b suppresses the epithelial-to-mesenchymal transition (EMT) and migratory potential of MM cells by targeting high-mobility group AT-hook 2 (HMGA2) (13). Cordycepin is able to suppress HMGA2-, Twist1- and zinc finger E-box-binding homeobox 1-dependent MM invasion and metastasis by upregulating miR-33b (14). However, the exact role of miR-33b in the regulation of MM cell proliferation and glycolysis remains unknown. The present study aimed to investigate the exact role of miR-33b in the regulation of MM cell proliferation and glycolysis, and its underlying mechanism of action.

 Materials and methods <sec> <title>Cell culture and transfection

The human MM cell lines (WM35, WM451 and SK-MEL-1), human melanocyte (HM) cells and HEK293 cells were obtained from the Cell Bank of Central South University (Changsha, China). Cells were cultured in Dulbecco's modified Eagle medium (DMEM; Thermo Fisher Scientific, Inc., Waltham, MA, USA) supplemented with 10% fetal bovine serum (Thermo Fisher Scientific, Inc.) at 37°C in a humidified incubator containing 5% CO2. For cell transfection, WM451 and SK-MEL-1 cells were transfected with scramble miR (miR-NC), miR-33b mimics, negative control (NC) inhibitor, miR-33b inhibitor, or co-transfected with miR-33b mimics and HIF-1α open reading frame (ORF) plasmid (all generated by Yearthbio, Changsha, China), using Lipofectamine 2000 (Thermo Fisher Scientific, Inc.), according to the manufacturer's instructions.

 Reverse transcription-quantitative polymerase chain reaction (RT-qPCR)

Total RNA was extracted from tissues and cells using TRIzol reagent (Thermo Fisher Scientific, Inc.), in accordance with the manufacturer's protocols. DNase (Thermo Fisher Scientific, Inc.) was used to remove genomic DNA, in accordance with the manufacturer's instructions. For the analysis of miR expression, a TaqMan MicroRNA Reverse Transcription kit (Thermo Fisher Scientific, Inc.) was used to convert RNA into cDNA, according to the manufacturer's protocol. Following this, qPCR was performed by using the miRNA Q-PCR detection kit (GeneCopoeia, Inc., Rockville, MD, USA), according to the manufacturer's protocols, on an ABI 7500 thermocycler (Thermo Fisher Scientific, Inc.). Primer sequences were purchased from Sangon Biotech Co., Ltd. (Shanghai, China). The reaction conditions were: 95°C for 5 min, followed by 40 cycles of denaturation at 95°C for 15 sec and annealing/elongation at 60°C for 30 sec. U6 gene expression was used as an endogenous control. The experiment was repeated three times. The relative mRNA expression levels were analyzed by the 2−ΔΔCq method (15).

 Detection of glucose consumption

After 24 h culture, the medium supernatant was collected and diluted to 1:4,000 in Dulbecco's phosphate buffered saline (PBS; Thermo Fisher Scientific, Inc.). The amount of glucose in the supernatant was then detected using a glucose uptake colorimetric assay kit (Sigma-Aldrich; Merck Millipore, kGaA, Germany), in accordance with the manufacturer's protocol. Absorbance was detected at 412 nm with an ELx-800 type ELISA reader (Omega Bio-Tek, Inc., Norcross, GA, USA).

 Detection of lactic acid production

Lactic acid immunoassay kits (Y4324; Yearthbio) were used to determine the lactic acid levels in MM cells, according to the manufacturer's instructions. Briefly, the lactic acid antibody (1:100; included in the kit) was incubated with MM cells overnight at 4°C. Following this, the MM cells were incubated with horseradish peroxidase-labeled anti-rabbit antibody (1:5,000; included in the kit) for 30 min at room temperature. Wells were then developed with tetramethyl benzidine reagent (Sigma-Aldrich; Merck KGaA) in the dark and the absorbance was measured at 450 nm.

 MTT assay

For detection of cell viability, 10,000 MM cells/well were plated in a 96-well plate, which was then incubated at 37°C (5% CO2) for 0, 24, 48 or 72 h, respectively. Following this, 10 µl MTT in PBS (5 mg/ml) was added to each well, and incubated at 37°C (5% CO2) for 4 h. Subsequently, the supernatant was removed, and 100 µl dimethylsulfoxide was added. Absorbance was detected at 570 nm with a microplate reader (680; Bio-Rad Laboratories, Inc., Hercules, CA, USA). Incubation with DMSO was used as the control.

 Western blot analysis

Protein was extracted from WM451 and SK-MEL-1 cells using radioimmunoprecipitation assay lysis buffer (Thermo Fisher Scientific, Inc.). Protein assay reagents (Thermo Fisher Scientific, Inc.). were used to measure the protein concentration. Total protein (50 µg/well) was then separated with 12% SDS-PAGE and transferred to a polyvinylidene fluoride membrane. Following this, the membrane was blocked with 5% nonfat dried milk in PBS at room temperature for 2 h. Subsequently, the membrane was incubated with rabbit anti-HIF-1α antibody (1:50; ab51608; Abcam, Cambridge, MA, USA), rabbit anti-HK2 antibody (1:50; ab37593; Abcam), rabbit-anti-LDH-A antibody (1:100; ab101562; Abcam), or rabbit anti-GAPDH antibody (1:50; ab9485; Abcam) overnight at 4°C. After washing with PBS for 10 min, the membrane was then incubated with goat anti-rabbit secondary immunoglobulin G (1:10,000; ab7090; Abcam) at room temperature for 1 h. After washing with PBS for 10 min, enhanced chemiluminescence reagent (Thermo Fisher Scientific, Inc.) was used to detect the signal on the membrane. Data were analyzed by densitometry using Image Pro Plus v.6.0 software (Media Cybernetics, Inc., Rockville, MD, USA) and normalized to GAPDH expression.

 Bioinformatics analysis and luciferase reporter assay

miRanda software 1.0 (microrna.org) was used to analyze the putative target genes of miR-33b. HIF-1α was revealed to be a putative target gene of miR-33b. Mutations of miR-33b binding sites in the HIF-1α 3′-UTR were introduced using an Easy Mutagenesis System kit (Promega Corporation, Madison, WI, USA), according to the manufacturer's instructions. The wild type (WT) or mutant type (MT) of HIF-1α 3′-UTR was cloned into the downstream sequence of the firefly luciferase coding region of pMIR-GLOTM luciferase vector (Promega Corporation). HEK293 cells were co-transfected with WT-HIF-1α-3′-UTR or MT-HIF-1α-3′-UTR plasmid, and miR-33b mimic or miR-normal control (NC), respectively. Following transfection for 48 h, a dual-luciferase reporter assay system (Promega Corporation) was used to detect luciferase activity, according to the manufacturer's instructions.

 Statistical analysis

SPSS v.17.0 (SPSS, Inc., Chicago, IL, USA) was used to perform statistical analysis. The results were expressed as the mean ± standard deviation of three independent experiments. Statistical analysis of differences was performed using one-way analysis of variance followed by Tukey's post hoc test. P<0.05 was considered to indicate a statistically significant difference.

 Results <sec> <title>miR-33b is downregulated in MM

To investigate the exact role of miR-33b in MM, RT-qPCR was conducted to determine miR-33b expression in three MM cell lines, including WM35, WM451 and SK-MEL-1. HM cells were used as controls. The results indicated that the expression of miR-33b was significantly reduced in WM35, WM451 and SK-MEL-1 cells compared with HM cells (all P<0.01; Fig. 1). As WM451 and SK-MEL-1 cells exhibited the most significant decrease in the miR-33b level, these two cell lines were used to investigate the effect of miR-33b on cell viability and glycolysis in melanoma cells in vitro.

 miR-33b inhibits viability and glycolysis in MM cells

In order to modulate miR-33b levels in MM cells, WM451 and SK-MEL-1 cells were transfected with miR-33b mimic or inhibitor. Following transfection, miR-33b expression was determined using RT-qPCR. miR-33b expression was significantly higher in WM451 and SK-MEL-1 cells transfected with miR-33b mimic (P<0.01) and significantly lower in cells transfected with miR-33b inhibitor (P<0.01) than that of the control group (Fig. 2A-D). However, transfection with scramble miR mimic or negative control inhibitor did not significantly affect miR-33b expression in WM451 and SK-MEL-1 cells. Following this, cell viability was determined using MTT assay. In both WM451 and SK-MEL-1 cells, cell viability was significantly decreased following overexpression of miR-33b (P<0.01) and significantly increased following knockdown of miR-33b (P<0.01) compared with the respective controls (Fig. 2E and F). Therefore, miR-33b suppresses MM cell viability.

Glycolysis serves a critical role in tumor cell proliferation (4,5). Therefore, the level of glycolysis in WM451 and SK-MEL-1 cells in each group was examined. The results indicated that glucose consumption and lactic acid production were significantly decreased in WM451 and SK-MEL-1 cells transfected with the miR-33b mimic (P<0.01) and significantly increased in cells transfected with the miR-33b inhibitor (P<0.01) compared with respective controls (Fig. 3). These results suggest that miR-33b has a suppressive role in regulating glycolysis in MM.

 HIF-1α is a direct target of miR-33b in MM cells

The putative target genes of miR-33b were investigated and bioinformatics analysis indicated that HIF-1α was a potential target. It has been suggested that HIF-1α is involved in glycolysis (6,7). To confirm this prediction, WT and MT HIF-1α-3′-UTR reporter plasmids (Fig. 4A and B) were created and luciferase reporter assays were performed. Luciferase activity was significantly decreased in HEK293 cells transfected with the miR-33b mimic and WT HIF-1α-3′-UTR reporter plasmid (P<0.01) compared with the control; however, this decrease was abolished in cells transfected with the MT HIF-1α-3′-UTR reporter plasmid (Fig. 4C). These data indicate that miR-33b is able to directly bind to the 3′-UTR of HIF-1α mRNA.

As miRs generally repress translation, the expression of HIF-1α protein in MM cells in each group was examined. It was determined that HIF-1α protein expression was markedly decreased following miR-33b overexpression and markedly increased following miR-33b inhibition compared with controls (Fig. 4D and E) in both the MM cell lines. This indicates that miR-33b negatively mediates expression of HIF-1α at the post-transcriptional level in MM cells. Taken together, these findings demonstrate that HIF-1α is a direct target of miR-33b in MM cells.

 Overexpression of HIF-1α reverses the suppressive effect of miR-33b upregulation on viability and glycolysis in MM cells

The present study investigated whether HIF-1α was involved in miR-33b-mediated viability and glycolysis in MM cells. miR-33b-overexpressing cells were transfected with HIF-1α ORF plasmid. Following co-transfection with the miR-33b mimic and HIF-1α plasmid, expression of HIF-1α protein was markedly increased compared with cells transfected with miR-33b alone (Fig. 5A and B). The viability and glycolysis level in MM cells transfected with miR-33b mimic, or co-transfected with miR-33b mimic and HIF-1α ORF plasmid were also examined and it was demonstrated that cell viability was significantly increased in the miR-33b + HIF-1α group compared with the miR-33b group (P<0.01; Fig. 5C and D). Similarly, glucose consumption and lactic acid production were significantly increased in the miR-33b + HIF-1α group compared with the miR-33b group (P<0.01; Fig. 5E-H). This demonstrated that overexpression of HIF-1α reverses the suppressive effect of miR-33b upregulation on viability and glycolysis in MM cells.

Hexokinase 2 (HK2) and lactate dehydrogenase A (LDH-A) are two key factors of glycolysis (16). Thus, the expression of HK2 and LDH-A proteins in MM cells transfected with miR-33b mimic, or co-transfected with miR-33b mimic and HIF-1α ORF plasmid were examined. Ectopic expression of miR-33b significantly decreased the expression of HK2 and LDH-A proteins in MM cells (P<0.01); however, this reduction was significantly reversed by HIF-1α overexpression (P<0.01; Fig. 6). Therefore, HK2 and LDH-A may be involved in miR-33b/HIF-1α-mediated glycolysis in MM cells.

 Discussion

miR are key regulators in the expression of various genes associated with tumorigenesis and malignant progression (17–19). However, the exact role of miR-33b in MM remains largely unclear. The present study demonstrated that miR-33b was significantly downregulated in MM cell lines. Further investigation indicated that MM cell viability and glycolysis were significantly decreased following miR-33b overexpression; however, these levels were significantly upregulated following miR-33b knockdown. HIF-1α, a key regulator of glycolysis, was identified as a direct target gene of miR-33b, and the expression of HIF-1α was negatively regulated by miR-33b in MM cells. Furthermore, overexpression of HIF-1α reversed the inhibitory effect of miR-33b on cell viability and glycolysis in MM cells. The results indicated that HK2 and LDH-A may be involved in miR-33b/HIF-1α mediated glycolysis in MM cells.

It has been well established that various miR are involved in the development and malignant progression of MM (20,21). For example, the miR let-7b, targets important cell cycle molecules, including cyclins D1, D3 and A, and cyclin-dependent kinase 4, in MM cells and interferes with anchorage-independent growth (22). Therefore, miR-221 and miR-222 may become potential molecular candidates for MM treatment. Additionally, it has been reported that miR-34a inhibit MM cell proliferation and migration by targeting c-Met (23). Recently, it was demonstrated that miR-33a is downregulated in MM and negatively regulates the proliferation, invasion and metastasis of MM cells (24). Overexpression of miR-33a also decreased MM tumorigenesis in vivo (24). Furthermore, miR-33b was demonstrated to suppress the migration, invasion and EMT of MM cells by targeting HMGA2 (13,14). These findings suggest that the miR-33 family has a critical role in MM. However, it remains unknown whether miR-33b influences MM cell proliferation and energy metabolism. In the present study, it was demonstrated that miR-33b was downregulated in MM cell lines, including WM35, WM451 and SK-MEL-1, compared with melanocyte HM cells. These findings were supported by those from a study by Zhou et al (24), which demonstrated that miR-33b expression levels was lower in MM cell lines, including WM35, WM451, A375 and SK-MEL-1, compared with HM cells. Additionally, in the present study it was observed that overexpression of miR-33b inhibited the viability of WM35 and WM451 cells, while knockdown of miR-33b enhanced the viability of these cells. This indicates that miR-33b, like miR-33a, may negatively regulate MM cell viability and therefore may inhibit tumor growth in vivo (24). Further studies are required to investigate the exact effect of miR-33b on MM growth and metastasis in vivo.

Tumor energy metabolism is characterized by preferential dependence on glycolysis, which is able to rapidly provide cancer cells with energy and metabolic intermediates for biosynthesis, despite being less efficient than oxidative phosphorylation in the yield of ATP (25,26). Therefore, in recent years, glycolysis has been suggested as a therapeutic target for cancer treatment (25,26). In the present study, overexpression of miR-33b was able to inhibit glucose consumption and lactic acid production in MM cells, suggesting that glycolysis was decreased. By contrast, inhibition of miR-33b increased the level of glycolysis in MM cells. Therefore, the suppressive effect of miR-33b on MM cell viability may occur via the inhibition of glycolysis. To verify this speculation, the putative target of miR-33b was investigated and HIF-1α was identified as a direct target gene of miR-33b in MM cells. It has previously been demonstrated that HIF-1α serves a key role in glycolysis (27). It is rapidly degraded by the proteasome under normal conditions and is stabilized by hypoxia (7,27). In advanced melanoma, the expression of HIF-1α is higher than that in the melanocytic nevi or thin melanomas localized to the skin (6). Furthermore, increased expression of HIF-1α is significantly associated with poor prognosis of MM (6,28). In the present study, it was determined that overexpression of HIF-1α reversed the suppressive effect of miR-33b on MM cell viability and glycolysis, suggesting that miR-33b inhibits MM cell viability by targeting HIF-1α-mediated glycolysis.

HK2 and LDH are two key enzymes involved in glycolysis (16). A previous study demonstrated that high expression of LDH was significantly associated with increasing tumor thickness and reduced disease-free and overall survival in MM (29). The serum level of LDH may be used to predict the prognosis and treatment response in MM patients (30). The present study also investigated whether HK2 and LDH-A were affected by miR-33b in MM cells. The results indicated that overexpression of miR-33b decreased expression of HIF-1α and LDH-A, while knockdown of miR-33b increased the expression of HIF-1α and LDH-A in MM cells. Thus, HK2 and LDH-A may be involved in miR-33b/HIF-1α-mediated glycolysis in MM cells.

In conclusion, the results of the present study demonstrate that miR-33b serves an inhibitory role in the regulation of MM cells, at least partially, by directly targeting HIF-1α, thus suppressing glycolysis. Therefore, miR-33b may serve as a potential candidate for MM treatment.

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Reverse transcription-quantitative polymerase chain reaction analysis was conducted to examine the miR-33b levels in three MM cell lines (WM35, WM451 and SK-MEL-1). HM cells were used as controls. Levels of expression were normalized to U6 gene expression. Data are expressed as the mean ± standard deviation. **P<0.01 vs. HM. MM, malignant melanoma; HM, human melanocyte; miR, microRNA.

Reverse transcription-quantitative polymerase chain reaction was conducted to examine miR-33b expression in WM451 and SK-MEL-1 MM cells. Levels of miR-33b expression in WM451 cells transfected with (A) miR-NC and miR-33b mimic, and (B) NC inhibitor and miR-33b inhibitor. Levels of miR-33b expression in SK-MEL-1 cells transfected with (C) miR-NC and miR-33b mimic, and (D) NC inhibitor and miR-33b inhibitor. Non-transfected WM451 or SK-MEL-1 cells were used as controls. Levels of expression were normalized to U6 gene expression. Data are expressed as the mean ± SD. An MTT assay was used to examine cell viability in (E) WM451 and (F) SK-MEL-1 cells. Data are presented as the mean ± SD. **P<0.01 vs. WM451 or SK-MEL-1 control. miR, microRNA; MM, malignant melanoma; miR-NC, scramble miR mimic; NC, negative control; OD, optical density; SD, standard deviation; A570 nm, absorbance at 570 nm.

Glucose consumption of WM451 cells transfected with (A) miR-NC and miR-33b mimic, and (B) NC inhibitor and miR-33b inhibitor. Glucose consumption of SK-MEL-1 cells transfected with (C) miR-NC and miR-33b mimic, and (D) NC inhibitor and miR-33b inhibitor. Lactic acid production of (E) WM451 and (F) SK-MEL-1 cells transfected with miR-NC and miR-33b mimic. Lactic acid production of (G) WM451 and (H) SK-MEL-1 cells transfected with NC inhibitor and miR-33b inhibitor. Non-transfected WM451 or SK-MEL-1 cells were used as controls. Data are presented as the mean ± standard deviation. **P<0.01 vs. WM451 or SK-MEL-1 control. miR, microRNA; miR-NC, scramble miR mimic; NC, negative control.

(A) WT or MT of HIF-1α 3′UTR was (B) cloned into a luciferase reporter vector to generate the WT or MT HIF-1α-3′UTR reporter plasmid, respectively. (C) Relative luciferase activity of HEK293 cells transfected with miR-NC or miR-33b mimic, and WT or MT HIF-1α-3′UTR reporter plasmid. Western blot analysis was performed to measure the expression of HIF-1α protein in (D) WM451 and (E) SK-MEL-1 cells transfected with miR-NC, miR-33b mimic, NC inhibitor or miR-33b inhibitor. GAPDH was used as an internal control. Data are presented as the mean ± standard deviation. **P<0.01 vs. the control. WT, wild type; MT, mutant type; HIF-1α, hypoxia-inducible factor-1α; UTR, untranslated region; miR, microRNA; miR-NC, scramble miR mimic; NC, negative control.

pcDNA3.1-HIF-1α plasmid was transfected into miR-33b-overexpressing WM451 and SK-MEL-1 cells. Western blot analysis was conducted to examine the expression of HIF-1α protein in (A) WM451 and (B) SK-MEL-1 cells transfected with miR-33b mimic or co-transfected with miR-33b mimic and pcDNA3.1-HIF-1α plasmid. GAPDH was used as an internal control. MTT assay was used to examine viability of (C) WM451 and (D) SK-MEL-1 cells transfected with miR-33b mimic or co-transfected with miR-33b mimic and pcDNA3.1-HIF-1α plasmid. Data are presented as the mean ± SD. Glucose consumption of (E) WM451 and (F) SK-MEL-1 cells transfected with miR-33b mimic or co-transfected with miR-33b mimic and pcDNA3.1-HIF-1α plasmid. Lactic acid secretion of (G) WM451 and (H) SK-MEL-1 cells transfected with miR-33b mimic or co-transfected with miR-33b mimic and pcDNA3.1-HIF-1α plasmid. Data are presented as the mean ± SD. **P<0.01 vs. miR-33b. HIF-1α, hypoxia-inducible factor-1α; miR, microRNA; OD, optical density; SD, standard deviation; A570 nm, absorbance at 570 nm.

Western blot analysis was conducted to examine the expression of HK2 and LDH-A protein in (A) WM451 and (B) SK-MEL-1 cells transfected with miR-33b mimic or co-transfected with miR-33b mimic and pcDNA3.1-HIF-1α plasmid. Non-transfected WM451 and SK-MEL-1 cells were used as controls. GAPDH was used as an internal control. Data are presented as the mean ± standard deviation. **P<0.01 vs. control; ##P<0.01 vs. miR-33b. miR, microRNA; HK2, hexokinase 2; LDH-A, lactate dehydrogenase A; HIF-1α, hypoxia-inducible factor-1α.