Abstract
Aims:
25-Hydroxyvitamin D [25(OH)VD] deficiency/inadequacy is a major public health issue affecting more than 1 billion people worldwide. A convincing association exists between low levels of circulating 25(OH)VD and the poor health outcomes associated with chronic diseases. However, high supraphysiological doses of VD are needed to achieve the required 25(OH)VD levels in the blood, because many subjects respond poorly to supplementation.
Results:
This study reports a link between 25(OH)VD deficiency and a reduction in glutathione (GSH) in obese adolescents. The improvement in GSH status that results from cosupplementation with VD and
Innovation:
These studies demonstrate a previously undiscovered mechanism by which GSH status positively upregulates the bioavailability of 25(OH)VD.
Conclusion:
Supplementation with a combination of VD and LC or GSH precursor, rather than supplementation with VD alone, is beneficial and helps achieve more successful VD supplementation. Antioxid. Redox Signal. 00, 000–000.
Introduction
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The status of 25-hydroxyvitamin D [25(OH)VD] plays a crucial role in preventing disease and maintaining optimal health. These studies demonstrate a previously undiscovered mechanism by which increasing glutathione (GSH) status positively influences the bioavailability of 25(OH)VD. The improvement in GSH caused by supplementation with vitamin D (VD) combined with
Risk factors for 25(OH)VD deficiencies include race (darker pigmented skin tones), higher body mass index (BMI), winter season, higher geographic latitudes, and diet. Circulating 25(OH)VD is considered to be a comprehensive and stable metabolite, levels of which can be used to diagnose 25(OH)VD deficiency and monitor VD consumption (8). The metabolic factors responsible for the limited success of VD supplementation studies, despite the convincing association between low 25(OH)VD levels and poor health, remain unknown.
VD or cholecalciferol in the human body is derived mostly from either diet or from skin exposure to ultraviolet B from sunlight (39, 45, 49, 59). Most people require dietary supplementation with VD to achieve the recommended blood levels of 25(OH)VD. The liver is the principal site where cholecalciferol is converted to 25(OH)VD by VD-25-hydroxylase (cytochrome p450 enzymes [CYP], CYP2R1, CYP27A1) (9, 14, 45, 56). 25(OH)VD is bound to vitamin D binding protein (VDBP) and transported into the circulation. VDBP is primarily synthesized and secreted by the liver (14, 55). (CYP27B1), which converts 25(OH)VD to its active metabolite [1alpha,25-dihydroxyvitamin D3, 1,25(OH)2VD], is present in both renal (major site) and nonrenal tissues (1). Even though renal tissue is considered to be a major site for 1,25(OH)VD formation, recent studies demonstrate expression of (CYP27B1) in nonrenal cells and tissues, indicating localized 1,25(OH)2VD formation and its tissue-specific paracrine function in different tissues (1).
(CYP24A1) is involved in the catabolic inactivation of 1,25(OH)2D3 and its inhibition is thought to limit 1,25(OH)2D3 signaling (39). Genetic variations in VDBP/(CYP2R1) are known to influence 25(OH)VD blood levels in response to VD supplementation (13, 19, 23, 29, 30, 52). Most cells have receptors for VD known as vitamin D receptor (VDR) (60). The biological actions of 1,25(OH)2VD are directly related to the VDR content of target tissues. Muscle is a major site of glucose metabolism and maintenance of glucose homeostasis (12). Therefore, biosynthesis and metabolism of VD are under the control of VD regulatory genes (GC/VDBP/VD-25-hydroxylase) in the liver, while the downstream actions of the active 1,25(OH)2VD in muscle are mediated by glucose metabolism genes (VDR/peroxisome proliferator-activated receptor gamma coactivator 1-alpha [PGC-1α]/glucose transporter type 4 [GLUT-4]).
Glutathione (GSH) is a major antioxidant and its depletion increases oxidative stress and extensive carbonylation of proteins (10, 11, 16
–18). Oxidative modification or carbonylation covalently modifies endogenous enzymes and proteins, which can result in the loss of protein function, insulin resistance (IR), and impaired cell function, and play a significant role in the etiology of several human diseases (2, 5, 6, 15, 37, 46, 47). Oral supplementation with GSH or
This article discusses our investigation of the dual roles of GSH in increasing circulating 25(OH)VD and augmenting the actions of active VD metabolites in one of the target tissues (skeletal muscle), which is a major site for glucose metabolism.
Results
Association between GSH and 25(OH)VD blood levels in adolescents
Blood levels of GSH and 25(OH)VD were significantly lower in obese compared with lean or overweight adolescents (Fig. 1a, c). VDBP levels were significantly lower in obese children compared with both lean and overweight (Fig. 1d). Blood levels of carbonyl protein were significantly elevated in obese adolescents compared with lean and overweight, suggesting elevated oxidative stress level in obese subjects (Fig. 1b). Tumor necrosis factor alpha (TNF-α) levels and homeostatic model assessment (HOMA)-IR were significantly higher in obese compared with lean or overweight subjects (Fig. 1e, f). Figure 1g shows a significant positive correlation between 25(OH)VD and GSH (r = 0.38, p = 0.03, n = 72).
Supplementary Table S1 (Supplementary Data are available online at
This suggests that lower VDBP can contribute to decreased circulating 25(OH)VD levels in obese adolescents. A positive association exists between blood levels of GSH and those of 25(OH)VD and has been previously shown in adult diabetic patients (3, 25, 27). The present finding of a positive association between circulating 25(OH)VD and GSH status is unique and interesting because in contrast to adults, the adolescent population has a narrow age range (14–17 years) and does not have any of the confounding variables such as medications or clinical disorder. This led us to search whether GSH regulates VD regulatory genes and 25(OH)VD status, and additionally whether GSH deficiency increases TNF-α levels and downregulates PGC-1α/VDR/GLUT-4 signaling of glucose metabolism.
Effect of high-fat diet feeding on GSH, 25(OH)VD, and carbonyl protein levels in blood, and GSH metabolism genes and VD regulatory genes in liver and muscle in mice
Male C57BL/6J mice (5 weeks old) were purchased from The Jackson Laboratory (Bar Harbor, ME). The animals were fed either a standard chow diet (Control: Harlan TD.08485, providing 5.2% calories as fat) or a high-fat diet (HFD) for 16 weeks (36). Composition of normal and HFD is given previously (36). Data given in Figure 2 show that the HFD-fed mice exhibited significantly lower levels of GSH (Fig. 2a) and 25(OH)VD (Fig. 2c) and higher levels of carbonyl protein (Fig. 2b), TNF-α (Fig. 2e), and IR (Fig. 2f) similar to the obese adolescent subjects' data. VDBP levels were not significantly different between HFD- versus control diet-fed group. Body weight (BW), food intake, parathyroid hormone (PTH), calcium, and blood count levels in the blood of mice fed normal diet and HFD mice groups were similar (Supplementary Table S2).
Figure 3 shows the mRNA and protein expression of genes GCLC (glutamate-cystein ligase catalytic subunit)/GCLM (glutamate-cysteine ligase regulatory subunit)/GSS/NRF2 (nuclear factor erythroid-2-related factor) involved in GSH synthesis (Fig. 3a–c), and genes VDBP/CYP2R1/CYP27B1/VDR, which determine bioavailability of 25(OH)VD, were significantly downregulated (Fig. 3d–f) in livers of HFD-fed mice compared with normal diet-fed mice. Interestingly, mRNA and protein expression levels of CYP24A1 that degrade 25(OH)VD are upregulated in the liver of mice fed HFD in comparison with mice fed normal diet.
Figure 4 shows a significant decrease in total GSH and increased oxidative stress markers (Fig. 4j) in muscle. GSH (GCLC/GCLM/NRF2) and VD regulatory genes (VDBP/CYP2R1/CYP27B1) are downregulated significantly (Fig. 4a–f) in HFD-fed mice muscle. Figure 4g–i shows that mRNA and protein expression of genes that regulate glucose metabolism (VDR/PGC-1α/GLUT-4) is significantly downregulated and TNF-α increased in the muscle of mice fed HFD compared with normal diet-fed mice group.
There was a significant increase in lipid peroxidation and protein oxidation with decreased GSH levels in skeletal muscle (Fig. 4j) of HFD-fed compared with normal diet-fed mice. A similar trend was observed in liver tissue (Fig. 3g). Protein-bound carbonyls are relatively more stable than lipid peroxidation products (10, 11). This demonstrates that HFD consumption increases cellular oxidative stress levels.
Overall, HFD feeding resulted in a significant downregulation of genes that synthesize GSH and lower levels of GSH in blood, liver, and muscle. Similarly, there was a significant downregulation of VD regulatory genes in the liver and muscle of mice fed HFD. In addition, there was a significant downregulation of glucose metabolism genes in muscle of mice fed HFD in comparison with normal diet-fed mice group. A decrease in blood and tissue GSH reflects exhaustion or impaired antioxidant pathways and increased oxidative stress in tissues in mice consuming HFD.
Effect of supplementation with VD along with LC on plasma levels of GSH, 25(OH)VD, and IR, and on GSH and VD regulatory genes in liver and on GSH and glucose metabolism genes in muscle
Beginning at 5 weeks of age, male C57BL/6J mice were fed and maintained on a VD-deficient HFD and water ad libitum for 16 weeks (36). Mice were gavaged daily for the last 8 weeks with saline, olive oil (OO), LC (5 mg/kg BW), VD (67 IU/kg BW), or LC+VD to investigate whether cosupplementation with GSH precursor has a better effect on blood levels of 25(OH)VD compared with levels achieved using VD alone. VD was dissolved in OO and one group of mice was also gavaged with OO (vehicle) alone. Details of experimental design are shown in Figure 5.
The effect of VD with and without cosupplementation with LC on blood levels of GSH, carbonyl protein, 25(OH)VD, VDBP, TNF-α, IR, glucose, and HbA1c is shown in Figure 6a–h. VD alone did not show effect on GSH, TNF-α, VDBP, IR, and HbA1c. However, supplementation with combined VD (cholecalciferol)+LC significantly corrected the GSH status and showed a significant decrease in TNF-α, IR, and HbA1c in the blood compared with levels seen in the mice supplemented with OO (vehicle)-control group. In addition, supplementation with combined VD (cholecalciferol)+LC showed a greater increase in 25(OH)VD and decrease in protein carbonylation levels in the blood compared with the OO-supplemented control mice. There were no changes in food intake, RBC indices, or calcium among these groups. There was also no change in blood counts, which indicates that the decrease in HbA1c values seen in the VD+LC group was not due to any effect on cell viability (Supplementary Table S3).
Cosupplementation with VD+LC caused a significantly greater upregulation of mRNA and protein expression of GSH synthesizing genes (GCLC/GSS/NRF2), GSH status, and VD regulatory genes (CYP2R1/CYP27A1/VDBP/VDR) in the liver (Fig. 7a–f). In addition, CYP24A1 showed significantly lower mRNA and protein expression levels in the liver of mice supplemented with VD+LC in comparison with VD-alone mice. This study measured total 25(OH)VD status using an enzyme-linked immunosorbent assay (ELISA) kit. Studies in the literature show that 25(OH)VD analyses using either an ELISA kit or the MC/MS approach show a significant correlation. Similarly, Figure 8 shows that there was a significant upregulation of GCLC/GCLM/NRF2 (Fig. 6a–c) and VD regulatory genes CYP2R1/CYP27A1/VDR (Fig. 8d–f) in the muscle of mice supplemented with VD+LC compared with VD alone.
In addition, there was a significant upregulation of PGC-1α/GLUT-4 (Fig. 8g–i) and GSH status (Fig. 8j) in muscle of mice supplemented with VD+LC in comparison with VD-alone supplemented mice (Fig. 8g–i). In addition, levels of protein oxidation and lipid peroxidation were significantly reduced in the liver (Fig. 7g) and muscle (Fig. 8j) of mice supplemented with VD+LC compared with those in mice supplemented with VD alone. The increase in GSH and reduction of oxidative stress biomarkers in blood and tissues reflect reduction of oxidative stress levels in tissues of mice supplemented with VD+LC compared with tissues of mice supplemented with VD alone.
Figure 9 shows that GCLC KD resulted in a dose-dependent decrease in GCLC (Fig. 9a) with downregulation of VDBP, CYP27A1, CYP27B1, and VDR and upregulation of CYP24A1 mRNA levels (Fig. 9b–f) in hepatocytes. Figure 9g shows a decrease in the level of GSH and increase in lipid peroxidation and carbonylated protein (Fig. 9h, i) levels in GCLC-KD hepatocytes. The effect of GSH deficiency and of LC supplementation on GSH, malondialdehyde (MDA), and carbonyl protein in GCLC-normal and GCLC-KD hepatocytes is shown in Figure 9j–l. GSH deficiency (8–21%) resulted in significantly increased levels of carbonyl protein (77–277%) and MDA (67–12%) levels, and LC supplementation improved the status of GSH and reduced oxidation of both proteins and lipids in GSH-normal and GSH-deficient hepatocytes. This suggests that improved GSH status has the potential to prevent oxidative stress and mediate the upregulation of VD regulatory gene levels. Details of treatments with GCLC siRNA, LC, and mRNA analyses are given previously (26).
The stimulatory effect of cholecalciferol on VD regulatory genes was higher in LC cosupplemented cells, as shown in Figure 9m–r. GSH deficiency impairs VD regulatory gene expression, whereas cosupplementation with VD and LC can positively modify the status of GSH, CYP24A1, and VD regulatory genes in hepatocytes. These studies show that GSH status positively upregulates the gene expression of CYP27B1 that converts 25(OH)VD to 1,25(OH)2VD. VDR-KD was induced using siRNA and was able to achieve nearly 80% VDR-KD in hepatocytes. VDR-KD caused a simultaneous decrease in VD metabolism genes CYP27A1, VDBP, and VDR, while upregulation of genes by VD+LC was abolished in VDR-KD hepatocytes (Supplementary Fig. S1). Supplementation with LC alone caused upregulation of VDBP but not of the CYP27A1 gene compared with results in control VDR-KD cells (Supplementary Fig. S1). This suggests that VDR mediates the beneficial effect of cholecalciferol on VD metabolism gene upregulation.
Figure 10 shows that GSH deficiency (GCLC-KD) caused a simultaneous increase in TNF-α and decrease in VDR/PGC-1α/GLUT-4 mRNA expression in GCLC-KD C2C12 myotubes (Fig. 10a–f). Stimulation with exogenous TNF-α per se downregulates VDR/PGC-1α/GLUT-4 in myotubes (Fig. 10g–j). Supplementation with LC, which increases GSH levels, caused an increase in mRNA expression of VDR/GLUT-4, and a decrease in TNF-α levels in both GCLC-normal and GCLC-KD myotubes (Fig. 10k–p). This suggests that GSH deficiency caused an increase in TNF-α and decrease in PGC-1α, as well as a decrease in the VDR/GLUT-4 needed for the action of 1,25(OH)2VD in muscle. Deficient GSH levels can result in inflammation, which can be reversed by improving GSH status. Further studies examined the effect of combined LC and 1,25(OH)2VD and of PGC-1α KD on GLUT-4 in myotubes.
Cotreatment with LC and 1,25(OH)2VD (active vitamin D) resulted in significantly greater upregulation of PGC-1α/NRF2/GLUT-4 (Fig. 10q–s) gene expression in comparison with results from treatment with 1,25(OH)2VD alone; however, this was not seen in PGC-1α-KD cells. Thus, a reduction in levels of TNF-α by LC will result in lowered inflammation and improved glucose metabolism and skeletal muscle function. 1,25(OH)2VD was used to understand its efficacy on glucose metabolism genes in muscle cells, whereas cholecalciferol was used with hepatocyte studies to understand 25(OH)VD biosynthesis from cholecalciferol in liver.
Discussion
GSH is a major antioxidant and a cofactor of many enzymes in the human body (16 –18). GSH is readily measured in blood and reflects the in vivo defense against oxidative stress (16, 47, 48, 53). This study demonstrates that a reduction in GSH status is linked to 25(OH)VD deficiencies in obese adolescents and in HFD-fed mice. A decrease in blood GSH and increased oxidative stress reflect exhausted or impaired antioxidant pathways in obese humans and HFD-fed mice. Lower levels of GSH can occur because of nonavailability of LC from food consumption, increased ROS production and oxidative stress from energy-rich diet consumption, and/or increased utilization of GSH relative to its biosynthesis. The depletion or deficiency of GSH can increase oxidative stress and extensive carbonylation of proteins, which can increase inflammatory mediators such as TNF-α and impair normal function of endogenous enzymes and proteins, and IR (10, 11, 16 –18).
This study shows a significant positive correlation between 25(OH)VD and GSH status in adolescents. This led us to examine whether GSH regulates VD regulatory genes and 25(OH)VD status in the blood. Using the mouse model of 25(OH)VD deficiency, we show a significantly greater increase in blood 25(OH)VD levels after cosupplementation with VD (cholecalciferol)+LC (a GSH precursor) compared with results in a group supplemented with VD alone. In addition, supplementation with VD alone does not affect GSH, TNF-α, or IR levels in blood; however, when compared with results in the control group, cosupplementation using VD with LC significantly increases GSH levels and reduces oxidative stress, TNF-α, and IR levels in blood, and increases GSH levels and reduces oxidative stress in liver and muscle. Transfection studies demonstrate that GSH deficiency causes increased oxidative stress, downregulation of VDBP/VD-25-hydroxylase/VDR, and upregulation of CYP24A1 in mouse hepatocytes and downregulation of PGC-1α, VDR, GLUT4 in mouse myotubes, similar to results seen in HFD-fed mice.
Improvement in GSH status by LC prevented the downregulation of VD regulatory genes in hepatocytes and glucose metabolism genes in myotubes. These in vitro and in vivo studies demonstrate the dual roles of GSH in increasing circulating 25(OH)VD and augmenting the actions of active VD metabolites in one of the target tissues (skeletal muscle), which is a major site for glucose metabolism.
Figure 11 outlines the proposed mechanism for role of GSH deficiency in 25(OH)VD deficiency and potential of combined VD and LC supplementation on stimulation of VD regulatory genes and protection from 25(OH)VD deficiency and inflammation. The mechanism potentially responsible for the increased blood levels of 25(OH)VD could be that LC upregulates the synthesis of GSH, thus improving the status of GSH, which reduces oxidative stress and prevents impaired (reduced) levels of VDBP/VD-25-hydroxylase/VDR, thereby helping protect the status of 25(OH)VD levels. VDBP is required for efficient transport and VD-25-hydroxylase is needed for the hydroxylation of cholecalciferol.
Furthermore, upregulation of VDR status in target tissues stimulates the translocation of the VDR/1,25(OH)2VD complex to the nucleus for activation of the VDR/PGC-1α/GLUT-4 pathway responsible for metabolic actions of 1,25(OH)2VD. The PGC-1α is an inducible transcriptional coactivator that upregulates expression of GLUT-4 in skeletal muscle and is a coactivator of the retinoic X receptor (RXRα) (40). PGC-1α functions as a cofactor for NRF2, which is implicated in the biosynthesis of GSH (24). Therefore, upregulation of PGC-1α and GLUT-4 is beneficial in reducing IR and glycemia.
This study provides evidence for a previously undiscovered mechanism that describes how 25(OH)VD deficiency/inadequacy is linked to lower GSH levels and that boosting GSH status beneficially upregulates the genes of VD metabolism and VDR, both of which are needed to increase the bioavailability and blood levels of 25(OH)VD and reduce inflammation levels. GSH provides not only upregulation of VD regulatory genes but also adds to GLUT-4 activation. Thus, increasing GSH status by combined supplementation with LC or a GSH precursor along with VD provides a novel approach to treat widespread 25(OH)VD deficiency/inadequacy in populations worldwide.
Investigation of mRNA expression and protein expression analyses of genes showed some differences between mRNA expression and protein expression levels. This could be due to variances in post-transcription regulation; differences in mRNA and protein turnover rates across the spectrum of genes involved; or differences in the technical precision of the methodology used. This study demonstrates that the improvement in the GSH status exerts measurable and beneficial effects on both mRNA and protein expression levels of VDBP/VD-25-hydroxylase/VDR as well as PGC-1α/GLUT-4 genes. Blood levels of 25(OH)VD are lower in humans with a genetic mutation for VDBP or in VDBP-KD mouse models (19, 30, 52). Blood concentrations of VDBP are positively related to the half-life of circulating 25(OH)VD (30). This suggests that lower circulating 25(OH)VD levels could be a result of the decreased VDBP levels seen in obese adolescents. GSH is formed from LC by the enzymatic action of glutamate-cysteine ligase (GCL) and GSH synthetase (18).
Vitamin D helps the body absorb calcium and maintain bone and muscle health. Evidence in the literature supports the positive link between a high consumption of milk products and leafy vegetables and biomarkers of bone health and 25(OH)VD levels in the blood (50). In fact, milk and leafy vegetables are rich sources of both vitamin D and of GSH and methionine/
These findings focus attention on the fact that the VD supplements widely consumed by the public are unlikely to be efficacious unless the status of the VD metabolism genes is improved by first correcting the status of GSH. This suggests that combined consumption of GSH precursors and VD, rather than solely using high-dose VD, is both novel and a better strategy with which to achieve a more efficacious bioavailability in response to cholecalciferol consumption and to increase blood levels of 25(OH)VD.
Materials and Methods
Enrollment of human subjects
This study was carried out after informed written consent was obtained from all subjects according to the protocol approved by the Louisiana State University Health Sciences Center (LSUHSC) Institutional Review Board (IRB). This study enrolled adolescent boys and girls ages 14–17 years, in good health (other than being overweight or IR), who provided written informed assent and parental consent. Inclusion criteria were children who are not smoking or taking any medicines, food supplements, or antihistamines. All subjects who gave written informed consent were invited to return to have blood drawn after fasting overnight (8 h). The exclusion criterion was that subjects were excluded if pregnant or suspected to be pregnant, applied only to female subjects. Urine was collected from the female subjects for urine pregnancy testing. Subjects were allowed to sit quietly for 10 min after which blood was collected from an easily accessible forearm vein using a butterfly needle and Vacutainer® tube. Ethylenediaminetetraacetic acid (EDTA) blood tubes were brought to the research laboratory. Isolated plasma was stored in different aliquots and frozen immediately at −80°C for analyses of the biochemical parameters.
Animal studies
Male C57BL/6J mice (5 weeks old, 20–24 g) were purchased from The Jackson Laboratory and acclimatized in the institutional animal house for 1 week. Mice were divided into various groups by computer-generated randomization and then housed and labeled in individual cages. They were fasted overnight and then weighed. Blood glucose was assessed by tail prick using an Accu-Chek glucometer (Boehringer Mannheim Corp., Indianapolis, IN). BW and blood glucose were monitored weekly. Control animals were fed a normal diet (lower in fat), while animals in the HFD group were fed HFD for 16 weeks. Flow diagram showing details of diet feeding of mice is given in Supplementary Figure S2. For studies with VD-deficient animals, the mice were maintained on a VD-deficient HFD for 16 weeks. After 8 weeks, the mice were supplemented by oral gavage for another 8 weeks with either 5 mg LC/kg BW daily (LC) or 67 IU VD/kg BW (+VD), or the same doses of cholecalciferol and
In addition, two groups of mice maintained on the VD-deficient HFD were also simultaneously supplemented by oral gavage with either water or the same dose of the vehicle used for dissolving cholecalciferol (OO) (Fig. 5). The animals were maintained under standard housing conditions at 22°C ± 2°C with 12/12-h light/dark cycles. Normal diet, HFD, and VD-deficient HFD were purchased from The Jackson Laboratory and detailed composition of these diets is given in a recent publication (36). The amount of food intake was monitored at 12 and 16 weeks into the treatment period to assess consumption. At the end of 16 weeks, the animals were fasted overnight and then euthanized for analysis by exposure to isoflurane (Webster Veterinary Supply, Inc., Devens, MA). Blood was collected via heart puncture with a 191/2-gauge needle into heparinized Vacutainer tubes. Plasma was isolated after centrifuging the blood in a 4°C centrifuge at 3000 rpm for 10 min. The livers were perfused with cold saline to free them of residual blood. Liver and gastrocnemius muscle were collected immediately, weighed, quickly diced, and frozen in liquid nitrogen at −80°C.
Dose justification for LC and vitamin D
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Cell culture and treatment
FL83B mouse hepatocytes (ATCC®, Manassas, VA) were cultured and maintained in F-12K complete medium. Mouse C2C12 myoblasts were cultured at 37°C in an atmosphere of 5% CO2 in growth medium (GM) consisting of Dulbecco's modified Eagle's medium (DMEM) supplemented with heat-inactivated 10% fetal bovine serum and antibiotics (penicillin and streptomycin). Differentiation of myoblasts into myotubes was induced when the cells had achieved 90–95% confluence by switching the medium from GM to differentiation medium consisting of DMEM supplemented with 2% horse serum (5 days), then treated as described in the figures. siRNAs were purchased from Santa Cruz Biotechnology, Inc. (Dallas, TX), catalog numbers sc-41979 (GCLC), sc-36811 (VDR), and sc-38885 (PGC-1α). The control siRNA, a scrambled nonspecific RNA duplex that shares no sequence homology with any of the genes, was used as a negative control.
Cells were transiently transfected with 0–100 nM siRNA complex using Lipofectamine™2000 transfection reagent (Invitrogen, Carlsbad, CA) following the method described earlier (26, 43). The next day cells were treated with LC (0–300 μM) for 6 h for LC-alone experiments. Pretreatment of the cells, maintained at a concentration of 1 × 106/mL media, was done for 2 h with LC (0–300 μM), followed by treatment for 22 h with cholecalciferol or 25(OH)VD (10 nM). TNF-α (0–250 pg/mL) was exposed for 6 h to differentiated myotubes.
Justification for use of FL83B mouse hepatocytes and mouse C2C12 myoblasts
Liver is a major player in the synthesis and secretion of VDBP and the hydroxylation of cholecalciferol (vitamin D3) to 25-hydroxy-vitamin D. FL83B mouse hepatocytes express VDBP, CYP27A1, CYP27B1, CYP24A1, and VDR, but expression of CYP2R1 is very low and could not be accurately quantitated. However, we got reproducible gene analysis results for expression of VDBP, CYP27A1, CYP27B1, CYP24A1, and VDR genes using FL83B mouse hepatocytes. Liver contains both CYP27A1 and CYP2R1 and participates in the conversion of cholecalciferol (vitamin D3) to 25-hydroxy-vitamin D. The population studies have also shown a link between CYP2R1, GC (VDBP), CYP24A1, and VDR with that of circulating 25(OH)VD concentrations. Recent studies have shown a regulatory role of CYP27A1 gene expression on the blood concentrations of 25(OH)VD (4, 54, 57, 62, 63).
Thus, mouse hepatocytes used in this study have much strength and can be used for investigating the link between GSH-deficiency, oxidative stress, and VD regulatory genes. Muscle is a major site for glucose metabolism. Differentiation of myoblasts into myotubes is very reproducible and these cells express the glucose metabolism genes such as PGC-1α, RXRα, VDR, and GLUT-4. GLUT-4 is a master regulator for the maintenance of glucose metabolism. Thus, mouse C2C12 myoblasts have much strength to investigate the role of GSH deficiency in regulation of glucose metabolism pathways (42).
Analysis of mRNA expression using quantitative polymerase chain reaction
Total RNA was extracted from cells or tissue using the TRIzol reagent (Life Technologies) following the manufacturer's instructions. The quality and quantity of the extracted RNA were determined on a NanoDrop spectrophotometer (Thermo Scientific). First-strand complementary DNA (cDNA) synthesis was performed using a commercially available High Capacity RNA-To-cDNA kit (Life Technologies) in a final reaction volume of 20 μL. Amplification of cDNA was performed on a 7900HT Real Time polymerase chain reaction (PCR) system (Applied Biosystems). PCR conditions were 2 min at 50°C, 10 min at 95°C, 40 cycles of 95°C for 15 s, and then 60°C for 60 s. Details of the TaqMan-FAM-labeled primer/probe used are given in Supplementary Table S4. Glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used as a housekeeping gene to normalize threshold cycle (CT) values.
To exclude nonspecific amplification and/or the formation of primer dimers, control reactions were performed in the absence of target cDNA. All of the experiments were run in triplicate. The relative amounts of mRNAs were calculated using the relative quantification (ΔΔCT) method. Supplementary Table S4 gives details of primer used in our studies.
Western blot analysis
The tissue homogenates were processed for immunoblotting studies. To extract protein from liver and gastrocnemius muscle, ∼100 mg of tissue was homogenized in RIPA buffer on ice using a rotor/stator. RIPA buffer (50 mM Tris pH 8, 150 mM NaCl, 1% NP-40, 0.5% deoxycholic acid, and 0.1% SDS) was supplemented with protease and phosphatase inhibitors (1 mM phenylmethylsulfonyl fluoride, 5 μg/mL leupeptin, 2 μg/mL aprotinin, 1 mM EDTA, 10 mM NaF, and 1 mM NaVO4). Lysates were then centrifuged for 10 min at 10,000 g at 4°C. Supernatants were collected and the protein concentrations were determined using a BCA assay kit (Pierce/Thermo Scientific, Rockford, IL) for Western blot analysis and high performance liquid chromatography (HPLC) assay. Equal amounts (20 μg) of proteins were separated on 10% sodium dodecyl sulfate–polyacrylamide gel electrophoresis (SDS-PAGE) and transferred to a polyvinyl difluoride membrane. Membranes were blocked at room temperature for 2 h in a blocking buffer containing 1% bovine serum albumin to prevent nonspecific binding and then incubated with an appropriate primary antibody at 4°C overnight (26, 43).
The membranes were washed in TBS-T (50 mM Tris–HCl, pH 7.6, 150 mM NaCl, 0.1% Tween 20) for 30 min and incubated with an appropriate Horseradish peroxidase-conjugated secondary antibody (1:5000 dilution) for 2 h at room temperature. The protein bands were detected using ECL detection reagents (Thermo Scientific) and exposed on blue X-ray film (Phenix Research Products, Candler, NC). The technical replicates (n = 2) and biological replicates (n = 4) were done in all our immunoblot experiments. Western blot scans were analyzed using ImageJ software (developed by Wayne Rasband, National Institutes of Health, Bethesda, MD.* Densitometry analyses of Western blots were normalized with respect to β-actin or GAPDH (ratio).
25(OH)VD, 1,25(OH)2VD, VDBP, GSH, TNF-α, PTH, insulin, glucose, protein carbonyl, and MDA assays
Plasma levels of 25(OH) vitamin D were determined using an ELISA kit (Calbiotech, Spring Valley, CA) and 1,25(OH)2vitamin D using another ELISA kit (My BioSource, San Diego, CA). Plasma VDBP quantification was carried out using a kit purchased from ALPCO Diagnostics (Salem, NH). TNF-α was measured using an ELISA kit from R&D Systems (Minneapolis, MN). PTH (1–84) and insulin were determined using ELISA kits from ALPCO Diagnostics, and the HOMA-IR index was calculated (42). VDBP was measured using polyclonal antibodies (DRG Instruments, Springfield, NJ). The kit included polyclonal antibodies that detect total VDBP levels. In the ELISA, control samples were analyzed each time to check the variation from plate to plate on different days of analysis. Protocols as given in the manufacturer's instructions were followed using appropriate controls and standards.
Levels of GSH in plasma, tissues, and cultured cells were determined using HPLC (44). This assay determines total GSH status. Cell viability was determined using the Alamar Blue method (Alamar Biosciences, Sacramento, CA). Oxidative stress was assessed by the quantification of protein carbonyls and MDA using Protein Carbonyl Colorimetric and TBARS Assay Kits, respectively (Cayman Chemical, Ann Arbor, MI). Measurements of HbA1c, Complete Blood Count, glucose, and calcium were done at the clinical chemistry laboratories of LSUHSC-Shreveport. Due to limited amount of blood collected from each mouse, we borrowed diluents from the clinical laboratory and diluted the blood before taking it to the clinical laboratory, which reduced the amount of blood required for clinical tests. All chemicals were purchased from Sigma Chemical Co. (St. Louis, MO) unless otherwise mentioned.
Statistical analysis
Data from clinical, cell culture, and mouse studies were analyzed using regression analyses and ANOVA with Sigma Stat software (SPSS, Chicago, IL). A p-value of ≤0.05 for a statistical test was considered significant.
Data availability
The data supporting the findings are available within the article and the associated Supplementary Data of this study. Any other data are available from the corresponding author on reasonable request.
Footnotes
Acknowledgments
The authors are supported by grants from NIH (R01 AT007442) and the Malcolm Feist Endowed Chair in Diabetes. The authors thank Ms. Morgan for excellent editing. Orcid ID: orcid.org/0000-0002-9574-0436.
Authors' Contributions
S.K.J. designed the research; R.P., A.E.A., and P.K.-M. performed the research; S.K.J., R.P., and A.E.A. analyzed data; and S.K.J. and J.A.B. wrote the article.
Disclosure Statement
No competing financial interests exist.
Abbreviations Used
*
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References
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