Introduction
N-myc downstream-regulated gene 2 (
NDRG2) is a member of the
NDRG family [
1] and was first identified and cloned in our laboratory from a normal human brain cDNA library by subtractive hybridisation [
2]. Accumulating evidence indicates that
NDRG2 is a tumour suppressor gene that is downregulated or undetectable in many human cancers [
1,
3]. The overexpression of NDRG2 is able to enhance cell apoptosis, inhibit cell proliferation and suppress angiogenesis in many malignant tumours [
4,
5]. Recently, researchers showed that NDRG2 expression was inversely associated with TNM (tumour, node, metastasis) stage in 189 breast carcinoma tissues and paired normal breast tissues [
6].
In addition to its known antitumoural function,
NDRG2 may be a metabolism-related gene regulated by many hormones, including adrenal steroids [
7], dexamethasone [
8,
9], insulin [
10‐
12], androgen [
13], oestrogen [
14] and aldosterone [
15]. NDRG2 was found to act as a regulator of myoblast proliferation and can be regulated by anabolic and catabolic factors [
8]. In skeletal muscle, NDRG2 is a substrate for several serine-threonine protein kinases, including protein kinase B (Akt) and serum- and glucocorticoid-induced kinase 1 (SGK1) [
10,
16]. NDRG2 was also found to induce amiloride-sensitive Na
+ transport in
Xenopus laevis oocytes and Fischer rat thyroid cells [
17]. In a previous study, we found that NDRG2 promoted Na
+/K
+-ATPase activity to promote cell Na
+ transport and fluid balance [
14]. We also identified that NDRG2 acted as a key molecule in pancreatic
β cells and was involved in Akt-mediated protection of
β cells against lipotoxicity [
11]. The evidence described herein suggests that
NDRG2 is a metabolism-related gene and plays important roles in cellular physiological metabolism. Furthermore, NDRG2 was recently shown to respond to cellular stress under a series of environmental stress conditions [
1]. However, very little information is available regarding the function of NDRG2 in tumour metabolism.
Mammalian cells depend on glucose as a major substrate for energy production [
18]. Warburg showed that tumour cells could metabolise many orders of magnitude larger amounts of glucose than their differentiated normal counterparts [
19,
20]. The transport of glucose across the plasma membrane is the first rate-limiting step for glucose metabolism and is mediated via glucose transporter proteins (GLUTs) [
18]. At present, 14 members of the GLUT family have been identified [
21]. GLUT1 is broadly expressed in the body tissues and is involved in glucose uptake in the basic state. Elevated levels of GLUT1 have been shown to be present in many human cancers, including head and neck, breast, lung and ovarian [
22,
23]. Moreover, several reports have suggested that GLUT1 represents potential regulatory targets of oncogenes or tumour suppressors [
24‐
26].
We posited the following questions: (1) whether NDRG2 expression is associated with any GLUT expression, as well as the nature of its correlation with breast carcinoma; (2) whether and why NDRG2 affects the glucose uptake; (3) what would be the significance of the interactions between NDRG2 and the GLUTs; and (4) whether this regulation of NDRG2 on the GLUTs exists in vivo. In our present study, we tested the hypothesis that a possible mechanism of NDRG2 induces its participation in cancer cell energy metabolism through the regulation of GLUTs in breast carcinoma.
Methods
Tissue samples and study cohort
This study was approved by the Ethics Committee of the Fourth Military Medical University. All patients from whom we obtained the 30 pairs of breast carcinoma and adjacent normal breast tissue specimens, as well as the 269 breast carcinoma sample study cohort, provided their full consent to participate in the study at the Xijing Hospital of the Fourth Military Medical University (Xi’an, China). NDRG2 and GLUT1 expression were detected in all specimens. Tissue specimens were examined separately by two pathologists under double-blinded conditions without prior knowledge of the clinical status of the specimens.
Immunohistochemistry detection
Immunohistochemistry (IHC) was performed using the avidin-biotin-peroxidase complex method on all breast carcinoma samples. All sections were deparaffinised in xylenes and dehydrated through a gradient concentration of alcohol before endogenous peroxidase activity was blocked using 0.5% H2O2 in methanol for 10 minutes. After nonspecific binding was blocked, the slides were incubated with NDRG2 antibody (1:200; Abnova, Taipei, Taiwan) or GLUT1 antibody (1:200; Santa Cruz Biotechnology, Santa Cruz, CA, USA) in phosphate-buffered saline (PBS) at 4°C overnight in a humidified container. Biotinylated goat anti-rabbit immunoglobulin G (IgG) (1:400; Sigma-Aldrich, St Louis, MO, USA) was incubated with the sections for 1 hour at room temperature and detected using a streptavidin-peroxidase complex. The brown colour indicative of peroxidase activity was developed by incubation with 0.1% 3,3′-diaminobenzidine (Sigma-Aldrich) in PBS with 0.05% H2O2 for 5 minutes at room temperature. The appropriate positive and negative controls were included in each run of IHC.
Staining evaluation
An immunoreactivity score system based on the proportion and intensity of positively stained cancer cells was applied. The two extensional standards taken were as follows: (1) the number of positively stained cells ≤5%, scored 0; 6% to 25%, scored 1; 26% to 50%, scored 2; 51% to 75%, scored 3; and >75%, scored 4; and (2) the intensity of stain colourless, scored 0; pallideflavens, scored 1; yellow, scored 2; and brown, scored 3. Extensional standards (1) and (2) were multiplied, and the staining grade was stratified as absent (score 0), weak (score 1 to 4), moderate (score 5 to 8) or strong (score 9 to 12). Specimens were rescored if the difference of scores from the two pathologists was greater than 3. Tumours with moderate or strong immunostaining were classified as having high expression, and tumours with absent or weak immunostaining were classified as having low expression.
Cell cultures and reagents
T-47D and SK-BR-3 cells were obtained from the American Type Culture Collection (Manassas, VA, USA) and cultured in a humidified incubator under 5% CO2 in Dulbecco’s modified Eagle’s medium (DMEM) (Invitrogen/Life Technologies, Carlsbad, CA, USA) supplemented with 10% foetal bovine serum (FBS) and 2 mM L-glutamine. NDRG2 antibody was purchased from Abnova. GLUT1, hemagglutinin (HA), actin, flag and tubulin antibodies were obtained from Santa Cruz Biotechnology.
Gene transfection
The cells (1 × 10
6 cells/well) were seeded into six-well plates and transfected with the following constructs using Lipofectamine 2000 (Invitrogen/Life Sciences) according to the manufacturer’s instructions as follows: NDRG2 expression plasmid (pCMV-flag-NDRG2), GLUT1 expression plasmid (pCMV-eGFP-GLUT1), HA-ubiquitin or small interfering RNA (siRNA) that targeted
NDRG2. The target sequences of NDRG2 siRNA and control siRNA are given in Additional file
1: Table S1.
Gene infection
Cells were seeded into six-well plates at a density of 1 × 106 cells/well and incubated to reach approximately 80% confluence. After the medium was removed, adenovirus expressing NDRG2 (Ad-NDRG2) or the negative control adenovirus expressing LacZ (Ad-LacZ) was added to serum-free DMEM, incubated for 2 hours, replaced with fresh DMEM supplemented with 10% FBS and incubated for another 48 hours. Recombinant adenoviruses carrying NDRG2 or LacZ were purchased from Benyuan Zhengyang Gene Technology Company (Beijing, China).
Immunoblotting
Both cells and breast tissues were lysed in radioimmunoprecipitation assay buffer (0.05 M Tris-HCl (pH 7.4), 0.15 M NaCl, 0.25% deoxycholic acid, 1% Nonidet P-40, 1 mM ethylenediaminetetraacetic acid (EDTA), 1 mM phenylmethylsulfonyl fluoride, 10 mg/ml aprotinin and 10 mg/ml leupeptin). Protein concentrations were measured using a bicinchoninic acid protein assay (Pierce Biotechnology, Rockford, IL, USA). Proteins were resolved by SDS-PAGE and transferred to Hybond enhanced chemiluminescence nitrocellulose membranes (Amersham Biosciences, Piscataway, NJ, USA). The blots were probed with the different primary antibodies and species-matched secondary antibodies. The bands were detected using enhanced chemiluminescence (Pierce Biotechnology) or the Odyssey Imaging System (LI-COR Biosciences, Lincoln, NE, USA).
Real-time PCR
The RNA extracted from cells with TRIzol reagent (Invitrogen/Life Technologies, Carlsbad, CA, USA) was converted to combinational cDNA with the RevertAid First Strand cDNA Synthesis Kit (Fermentas/Thermo Scientific; Pittsburgh, PA, USA). Real-time PCR analysis was performed using the Prism 7500 Real-Time PCR System (Applied Biosystems, Foster City, CA, USA) and the SYBR
Premix Ex Taq II (Tli RNase H Plus) kit (TaKaRa Bio, Shiga, Japan) according to the manufacturer’s instructions. The relative gene expression levels were calculated using the 2
-ΔΔCt method, in which Ct represented the threshold cycle and β-actin was used as a reference gene. The primer sequence is given in Additional file
1: Table S1.
Cell proliferation assay
Cell growth following transfection was evaluated by 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) assay. Cells were seeded into a 96-well plate (1 × 104 cells per well) and incubated for 24 hours. The cells were then incubated with 0.5 mg/ml MTT (Sigma-Aldrich). Four hours later, the medium was replaced with 100 μl of dimethyl sulfoxide (Sigma-Aldrich) and vortexed for 10 minutes. Absorbance was then recorded at 490 nm using an Easy Reader 340 AT plate reader (SLT-Lab Instruments, Salzburg, Austria). Relative values of optical density were calculated as a percentage of the control. All experiments were performed three times independently.
Glucose uptake assay
Prior to being harvested, adherent cultures of control and NDRG2 adenovirus- or siRNA-treated cells in DMEM containing 25 mM glucose were washed twice with cold PBS and then lysed with ion-free H2O for 5 minutes on ice. The glucose content was measured with a D-glucose measurement kit (GAHK-20; Sigma-Aldrich) according to the manufacturer’s protocol.
Immunofluorescence assay
Cells were fixed in a freshly prepared solution of 4% paraformaldehyde, rinsed and permeabilised with 0.1% Triton X-100 in PBS. Permeabilised cells were then incubated with horse serum in PBS to block nonspecific binding. After being washed with PBS, the cells were incubated overnight at 4°C with mouse anti-NDRG2 antibody (diluted 1:150), rabbit anti-GLUT1 antibody (diluted 1:150) and fluorescein isothiocyanate (FITC)-conjugated anti-mouse antibody (diluted 1:400; Sigma-Aldrich) or cyanine 3 (Cy3)-conjugated anti-rabbit antibody (diluted 1:400; Sigma-Aldrich). The isotype mouse and rabbit IgGs were used as negative controls. Dual-colour detection was performed using a laser confocal microscope after treatment with 4′,6-diamidino-2-phenylindole (DAPI) to label nuclear DNA.
Immunoprecipitation
Transfected or untransfected cells were incubated with 1 ml of lysis buffer containing 150 mM NaCl, 50 mM Tris-HCl (pH 7.4), 1% Lubrol (polyethylene glycolmonocetyl ether; MP Biomedicals, Solon, OH, USA) and 5 mM EDTA, as well as protease inhibitors, for 30 minutes at 4°C. The insoluble fraction was eliminated through centrifugation at 10,000 × g for 30 min at 4°C. After centrifugation, the lysates were incubated with the antibody of interest, and protein A or G was conjugated to sepharose (Pierce Biotechnology) for 8 hours at 4°C. To quantify the total amount of protein loaded, 20 μl of the lysates was saved. Beads were washed four times with lysis buffer. Proteins were eluted in SDS-PAGE sample buffer and separated by SDS-PAGE for immunoblot analysis. The blots were then probed with peroxidase-conjugated goat anti-mouse or goat anti-rabbit antibodies and visualised by using an enhanced chemiluminescence reagent (Pierce Biotechnology).
Xenograft study in nude mice
For inoculation into nude mice, SK-BR-3 or MDA-MB-231 cells were washed with PBS, digested with trypsin and resuspended in serum-free DMEM. After centrifugation (800 rpm), the cell pellets were resuspended in DMEM. The cell suspension (1 × 106 cells in a 100-ml volume of PBS) was injected subcutaneously into the hind legs of 4-week-old female BALB/c athymic (nu/nu) mice (SLAC Laboratory Animal Company, Shanghai, China). When the tumours reached a volume of approximately 200 mm3, the mice were arbitrarily assigned to different groups (n = 6 each) to receive intratumoural injections of 0.5, 1 or 2 × 109 plaque-forming units (PFU) of Ad-NDRG2, 2 × 109 Ad-LacZ or PBS. Intratumoural injections were repeated every 3 days for a total of 21 days. Tumours were measured (perpendicular diameters) every 3 days, and their volumes were calculated. On day 21, the mice were killed and their tumours were removed for analysis. Tumour volumes were calculated based on caliper measurements of the length and width of the lesions using the following formula: 0.5 × length × (width2). The tumour growth curve was then derived from these data.
All of the experimental procedures were conducted in accordance with the Detailed Rules for the Administration of Animal Experiments for Medical Research Purposes issued by the Ministry of Health of China and received ethical approval by the Animal Experiment Administration Committee of the Fourth Military Medical University (Xi’an, China). All efforts were made to minimise the animals’ suffering and reduce the number of animals used.
Statistical analysis
In vitro experiments were performed three times, and each experiment was performed in triplicate. Data from all quantitative assays are expressed as the means ± SD and were analysed statistically using one-way analysis of variance, independent samples t-test or Student’s t-test. In the clinical specimens study, the associations between NDRG2 expression and categorical variables were analysed using the χ2 test or Fisher’s exact test as appropriate. Correlations between NDRG2 expression and the expression of other molecules were analysed by using the Spearman correlation test. Kaplan–Meier analysis was used to evaluate disease-free survival and overall survival. P < 0.05 was considered statistically significant.
Discussion
Understanding the mechanisms involved in cancer cell energy metabolism may provide a reasonable interpretation for the function of NDRG2 as a tumour suppressor. To the best of our knowledge, we report for the first time that NDRG2 participated in cellular glucose uptake by regulating the protein stability of GLUT1. We also found that NDRG2 adenovirus can be used to treat breast cancer by inhibiting cellular glucose uptake in a nude mouse xenograft model. Consistent with the cell- and animal-based results, a significantly inverse correlation between NDRG2 and GLUT1 expression was observed in clinical breast cancer tissue specimens.
Much of the data obtained from tissue of breast cancer patients presented herein are supportive of previously published work by Oh
et al.[
6]. Although researchers in several studies have reported that NDRG2 inhibited breast cancer cell survival and other malignant activities [
5,
28‐
30], the available clinical data before the publication by Oh
et al. were very limited [
6]. Liu
et al. previously reported that there was a reduction in
NDRG2 mRNA levels in 5 of 21 breast cancer tissue samples tested compared with normal tissues [
31]. Anders
et al. found that NDRG2 protein was reduced in breast cancer tissue based on a slightly larger sample set (
N = 35) [
32]. Recently, the correlation between NDRG2 expression level and clinical meaning was summarized by Oh
et al. in 189 breast cancer patients who had undergone surgical resection [
6]. Similarly to Oh
et al.’s data set derived from 189 breast carcinoma patients, we show in our present study that, in specimens obtained from 269 breast cancer patients, low NDRG2 expression was associated with advanced TNM stage, high Ki67 and HER2 expression and poor histological differentiation. We also found that breast cancer patients with high NDRG2 expression had longer disease-free survival and better overall survival compared with patients with low NDRG2 expression. However, by Oh
et al. showed that high NDRG2 expression correlated only with favourable recurrence-free survival, not with overall survival [
6]. Further observations are needed to confirm the correlation of NDRG2 and breast carcinoma prognosis. Additionally, in our present study, NDRG2 expression was inversely correlated with GLUT1 expression in patient specimens, which is in agreement with our cell- and animal-based results.
Many tumour suppressor genes play important roles in the regulation of glucose metabolism, in addition to their established roles in cell survival and apoptosis. p53, one of the most highly studied tumour suppressors, which can upregulate NDRG2 expression [
4], has been reported to reduce intracellular glucose levels by inhibiting the expression of GLUTs [
27]. For example, p53 directly represses the transcriptional activity of
GLUT1 and
GLUT4 gene promoters [
33]. In addition, p53 represses
GLUT3 gene expression indirectly by preventing the activation of the inhibitor of the nuclear factor κB pathway [
34]. In our present study, we show that NDRG2 could regulate GLUT1 posttranslational modification without affecting other glucose transporters, including GLUT2, GLUT3 and GLUT4. We also found that NDRG2 decreased GLUT1 protein stability by promoting the ubiquitin-mediated protein degradation pathway, whereas the transcription levels of both
GLUT1 and other
GLUT genes were not affected.
Investigators in previous studies have shown that the expression of
NDRG2 is regulated by some transcription factors, including p53 [
4], Myc [
35] and Hif-1 [
36].
NDRG2 is a novel p53-inducible target involved in the p53-mediated apoptosis pathway in lung cancer cells [
4], and the expression of
NDRG2 was upregulated by Hif-1 in tumour cells under hypoxic conditions [
36]. However, the expression of human
NDRG2 is downregulated by Myc via transcriptional repression [
35]. c-Myc directly transactivates genes encoding GLUT1 protein and increases glucose uptake in Rat1 fibroblasts [
37]. Under hypoxic conditions, a transcription factor complex including Hif-1α was shown to bind the
GLUT1 promoter to upregulate
GLUT1 mRNA expression [
38]. Interestingly, among the above-mentioned transcription factors, p53 might promote
NDRG2 expression [
4] and inhibit
GLUT1 transcriptional activity [
33], and Myc might suppress
NDRG2 expression [
35] and transactivate
GLUT1[
37].
NDRG2 and
GLUT1 were inversely regulated by p53 [
4,
33] and Myc [
35,
37], which suggests that
NDRG2 may function as a tumour suppressor by decreasing glucose uptake. Surprisingly, Hif-1 increases the expression of both
NDRG2[
36] and
GLUT1[
38]. We cannot explain why Hif-1 positively regulates both
NDRG2 and
GLUT1 in a manner different from p53 or Myc. We hypothesise that this difference is due to the fact that Hif-1-related experiments were performed under different hypoxic conditions and cell physiological contexts. Whether hypoxia-inducible factors are involved in NDRG2-mediated GLUT1 content and glucose intake regulation in breast cancer needs to be directly determined in future studies.
NDRG2 appears to be broadly involved in stress responses, cell proliferation and cell differentiation [
1]. The proteins with which NDRG2 interacts may provide important information contributing to understanding its precise molecular and cellular functions. Our previous study characterised a cell-cycle-dependent transcription factor, MSP58, as a binding partner of NDRG2. NDRG2 may colocalise with MSP58 in the nuclear region of the HeLa cell during cell stress [
39]. In another of our previous studies, we found that the β1 subunit of Na
+/K
+-ATPase interacted and colocalised with NDRG2 in the perinuclear cytoplasmic region in human salivary cells and that NDRG2 could protect the β1 subunit protein and inhibit its degradation [
14]. In that previous study, we detected that NDRG2 bound to and partly colocalised with GLUT1 in the cytoplasmic region of breast cancer cells. We showed that NDRG2 can decrease GLUT1 protein stability and promote the ubiquitination and degradation of GLUT1. Collectively, these experiments imply that NDRG2 might act as some kind of chaperone molecule that is involved in regulating protein stability in different cell physiological contexts. However, the currently available bioinformatics analysis does not indicate any known motif or domain in NDRG2 [
40], and, to the best of our knowledge, there is no published literature indicating that NDRG2 is an E3 ubiquitin ligase. Mass spectrometric analysis could be used to screen for the ubiquitin-related proteins that interact with both NDRG2 and GLUT1. However, this hypothesis must be determined directly in future studies.
Competing interests
The authors declare that they have no competing interests.
Authors’ contributions
All authors conceived of the study and participated in its design. JM, WCL and HG performed most of the experiments. SLi performed xenograft experiments. WC participated in all statistical analyses. XD and SLei provided formalin-fixed, paraffin-embedded, archived patient materials and conducted pathologic reviews and clinical data evaluations. WH performed immunostaining and quantitative analyses. NL and YL interpreted the data and drafted the manuscript. JM, WCL, HG, SLi, WC, XD, SLei, WH, LX and LY revised the manuscript critically. All authors read and approved the final manuscript.