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In addition to its well-known glycolytic activity, GAPDH displays multiple functions, such as nuclear RNA export, DNA replication and repair, and apoptotic cell death. This functional diversity depends on its intracellular localization. In this study, we explored the signal transduction pathways involved in the nuclear translocation of GAPDH using confocal laser scanning microscopy of immunostained human diploid fibroblasts (HDFs). GAPDH was present mainly in the cytoplasm when cultured with 10% FBS. Serum depletion by culturing cells in a serum-free medium (SFM) led to a gradual accumulation of GAPDH in the nucleus, and this nuclear accumulation was reversed by the re-addition of serum or growth factors, such as PDGF and lysophosphatidic acid. The nuclear export induced by the re-addition of serum or growth factors was prevented by LY 294002 and SH-5, inhibitors of phosphoinositide 3-kinase (PI3K) and Akt/protein kinase B, respectively, suggesting an involvement of the PI3K signaling pathway in the nuclear export of GAPDH. In addition, 5-aminoimidazole-4-carboxamide-1-β-D-ribofuranoside (AICAR), an activator of AMP-activated protein kinase (AMPK), stimulated the nuclear translocation of GAPDH and prevented serum- and growth factor-induced GAPDH export. AMPK inhibition by compound C or AMPK depletion by siRNA treatment partially prevented SFM- and AICAR-induced nuclear translocation of GAPDH. Our data suggest that the nuclear translocation of GAPDH might be regulated by the PI3K signaling pathway acting mainly as a nuclear export signal and the AMPK signaling pathway acting as a nuclear import signal.
GAPDH (E.C. 18.104.22.168) functions as a glycolytic enzyme working within the cytoplasm. GAPDH forms a tetramer to be active and catalyzes the oxidative phosphorylation of glyceraldehyde 3-phosphate, producing 1,3-bisphosphoglycerate. Cysteine and histidine are located in the active site. Besides its role in glycolysis, GAPDH is also involved in several biological functions, including the organization of the cytoskeleton and regulation of endocytosis, binding and transport of tRNA, and regulation of translation, transcription, replication, DNA repair, cell proliferation, and apoptosis (Sirover, 2005; Harada et al., 2007). Its diverse activities appear to be regulated according to its oligomeric structure and subcellular localization to the nucleus and other subcellular organelles such as mitochondria and the cytoskeleton (Barbini et al., 2007). The nuclear translocation of GAPDH upon apoptosis (Sawa et al., 1997; Shashidharan et al., 1999; Du et al., 2007), serum deprivation (Schmitz, 2001; Schmitz et al., 2003), oxidative stresses (Dastoor and Dreyer, 2001), and genotoxic stresses (Brown et al., 2004) has been reported.
Analysis of the growth factor signaling pathway with specific inhibitors has revealed that the nuclear export of GAPDH is prevented by LY 294002, an inhibitor of phosphoinositide 3-kinase (PI3K) (Schmitz, 2001). Because PI3K links the growth factor signaling pathway with cell death via the repression of an apoptotic inducer, they have suggested that the nuclear accumulation of GAPDH upon growth factor depletion might be reversed by PI3K-induced survival signals (Schmitz, 2001). Activated PI3K produces phosphatidyl inositol 3,4,5-triphosphate (PIP3), which interacts with a variety of molecules, such as Akt kinase (also called PKB) via pleckstrin homology (PH) domains of these downstream targets (Cooray, 2004). The interaction of PIP3 with Akt allows the phosphorylation of Akt by PDK1/2 at two key regulatory sites, Thr308 and Ser473 near the C-terminus, and the subsequent activation of Akt (Rameh and Cantley, 1999). Akt is a serine/threonine kinase that phosphorylates many different target proteins including GSK-3β, Bad, caspase-9, forkhead transcription factors and NF-kB (Cooray, 2004).
AMP-activated protein kinase (AMPK) is a heterotrimeric serine/threonine protein kinase consisting of a catalytic α subunit and regulatory β and γ subunit. AMPK activity can be regulated by a low energy state (increases in the AMP/ATP ratio), phosphorylation of Thr172 and Ser485/491 of the α subunit, and stresses such as reactive oxygen species (ROS), hypoxia, and genotoxic drugs (Stein et al., 2000; Hawley et al., 2003; Hurley et al., 2006). AMPK has various cellular functions, including the regulation of cellular metabolism, ion channels, and gene expression (Hardie, 2004), activation of glucose transport during hypoxia and ischemia via eNOS phosphorylation (Li et al., 2004), cell cycle arrest via p53 phosphorylation (Jones et al., 2005), differentiation of endothelial progenitor cells via eNOS activation (Li et al., 2008), inhibition of protein synthesis via TSC1/2, induction of aortic vasorelaxation in mice (Goirand et al., 2007), and regulation of apoptotic cell death signals (Cao et al., 2008; Kim et al., 2008; Lee et al., 2009).
Since both PI3K/Akt and AMPK are responsive to serum and growth factors, and an AMPK activator, 5-aminoimidazole-4-carboxamide-1-β-D-ribofuranoside (AICAR), has been shown to inhibit the PI3K signaling pathway (Jhun et al., 2004), we postulated that the PI3K and AMPK signal transduction pathways might contribute to GAPDH translocation. Following serum depletion (by culturing in serum-free medium, SFM) and the re-addition of serum (by culturing in FBS), PDGF, and lysophosphatidic acid (LPA), we examined the intracellular distribution of GAPDH by confocal laser scanning microscopy of immunostained human diploid fibroblasts (HDFs). The involvement of the PI3K signaling pathway was examined using inhibitors of PI3K and Akt, LY 294002 and SH-5, respectively. The role of AMPK was examined using an inhibitor of AMPK (compound C), an activator of AMPK (AICAR), and siRNAs of AMPK. In addition, we examined the involvement of NOS and p53 in GAPDH nuclear localization using NOS inhibitors, N-nitro-L-arginine methyl ester (L-NAME) and N-monomethyl-L-arginine (L-NMMA), and p53-null cells, MEF-p53-/- and HCT116-p53-/-.
Because serum depletion had no influence on the total GAPDH expression level, we investigated the intracellular distribution of GAPDH by confocal laser scanning microscopy of immunostained HDFs (Figures 1A and 1B). Cells in which green FITC fluorescence was present in the cytosol, but absent or weak in the nuclear fraction, were counted as cells with cytosolic GAPDH. Cells with dense bright green fluorescence only in the nucleus were counted as cells with nuclear GAPDH. Cells containing green fluorescence evenly in both the nuclear and cytosolic fractions were counted as cells with cytosolic and nuclear GAPDH (Figure 1B). To compare the distribution of GAPDH between the cytosol and nucleus, the percent distributions of cells with cytosolic GAPDH (cytosol: black bar) or nuclear GAPDH alone (nuclear: white bar), and cells with both cytosolic and nuclear GAPDH (cytosol + nuclear: gray bar) were plotted in Figure 1C.
Almost all GAPDH was present in the cytosol of HDFs with a population doubling of less than 25 (designated as young HDFs in other reports) when they were cultured in DMEM containing 10% FBS for 2 days (Figure 1A, 10% FBS and Figure 1C, FBS). Serum withdrawal from young HDFs for 1 day initiated an accumulation of GAPDH in the nucleus, and its nuclear accumulation increased gradually until 5 days (Figure 1A, 10% FBS/SFM-5d). The number of cells with cytosolic GAPDH alone decreased such that the number of cells with nuclear GAPDH increased gradually to over 90% in young cells with serum depletion for 4-5 days (Figure 1C, SFM).
Nuclear export of GAPDH to the cytosol was observed upon the addition of serum to HDFs that had been serum-deprived for 5 days (Figure 2A, SFM-5d/10% FBS). After 2 days of incubation with 10% FBS, over 90% of the GAPDH had been released back to the cytosol (Figures 2A and 2B). Our data suggest that GAPDH nuclear translocation is a reversible process in HDFs. A portion (~60%) of the nuclear GAPDH in serum-deprived cells was also exported by treatment with 100 ng/ml PDGF for 24-48 h (Figure 2C) or 30 µM LPA for 48 h (Figure 2D).
The cell number with nuclear GAPDH alone was combined with that including both nuclear and cytosolic GAPDH to illustrate the effects of inhibitors and activators (nuclear +/- cytosol in Figures 3--55 and and77--9).9). An inhibitor of PI3K, LY 294002, induced the nuclear accumulation of GAPDH significantly (P < 0.001) at concentrations of 10-50 µM, even when cultured in 10% FBS for 2 days (Figure 3A). After serum depletion for 5 days, the medium was replaced with 10% FBS, 100 ng/ml PDGF, or 30 µM LPA in the presence and absence of 50 µM LY 294002. As shown in Figure 3B, the nuclear export induced by the re-addition of 10% FBS, PDGF, or LPA was (P < 0.001) prevented completely by the PI3K inhibitor, LY 294002.
SH-5, an inhibitor of PI3K-downstream kinase Akt, also induced the nuclear translocation of GAPDH significantly (P < 0.01) at a concentration of 20 µM when cultured in 10% FBS (Figure 3C). This concentration of SH-5 reduced partially but significantly (P < 0.001) the serum-induced GAPDH export (Figure 3D). Because the effect of SH-5 was less than that of LY 294002, we used Western blot analysis to compare the efficacy of LY 294002 and SH-5 on the phosphorylation of downstream substrates such as Akt, GSK3β, and Bad. As shown in Figure 3E, Ly 294002 completely inhibited Akt phosphorylation but only partially inhibited GSK3β phosphorylation. Similarly, SH-5 only partially inhibited the phosphorylation of GSK3β and Bad, two downstream signaling proteins of Akt. Although the reason why the Akt inhibitor is less effective remains elusive, our data suggest that the PI3K/Akt signaling pathway is involved in the nuclear export of GAPDH in HDFs.
To examine the involvement of AMPK in GAPDH translocation, we first examined the effect of AICAR, a specific AMPK activator, on GAPDH nuclear localization. HDFs were grown in culture medium containing 10% FBS for 2 days and then grown further in fresh culture medium with 0.5-2 mM AICAR for 1-4 days. AICAR by itself stimulated the nuclear translocation of GAPDH in a dose- and time-dependent manner (Figures 4A and 4B, respectively). About 60% of the cytosolic GAPDH was translocated to the nucleus after 4 days of treatment with 0.5 mM AICAR (P < 0.001) and its translocation increased to over 90% by 2 mM AICAR treatment for 4 days (Figures 4A and 4B). After GAPDH had localized to the nucleus by serum depletion for 4 days, the effect of AICAR on the nuclear export of GAPDH by FBS was also examined. In the presence of 0.5-2 mM AICAR, nuclear GAPDH was not exported to the cytosol upon serum re-addition (Figure 4C).
To work as a specific activator of AMPK, AICAR should be internalized and become phosphorylated by adenosine kinase to form AICAR-monophosphate (AICA ribotide, ZMP) (Vincent et al., 1996). ZMP mimics the effects of AMP on AMPK (Corton et al., 1995). Therefore, we first examined whether the AICAR-induced nuclear accumulation of GAPDH depends on AICAR uptake and subsequent phosphorylation to ZMP using an adenosine kinase inhibitor, 5'-iodotubercidin (5'-ITC). Within the concentration range of 0.1-1 µM, 5'-ITC increased a low but significant (P < 0.001) nuclear export of GAPDH in a dose-dependent manner, while at higher concentrations, such as 2 µM, it enhanced the level of nuclear GAPDH slightly (Figure 5A). After serum depletion for 4 days, FBS-induced GAPDH export was also examined in the presence of 5'-ITC. The lower concentrations of 5'-ITC did not affect FBS-induced GAPDH export, but 5'-ITC concentrations as high as 2 µM resulted in about 70% nuclear GAPDH (Figure 5B). The AICAR-induced nuclear accumulation was partially but significantly (P < 0.001) reduced in the presence of various doses of 5'-ITC, compared to the level observed in the presence of 2 mM AICAR only (Figure 5C). Over 90% of the cytosolic GAPDH was translocated to the nucleus after 4 days of treatment with SFM, and then most GAPDH was released by the addition of 10% FBS. We also observed that 2 mM AICAR blocked FBS-induced release, and this AICAR effect was reduced significantly (P < 0.001) in the presence of lower concentrations (0.1-0.5 µM) of 5'-ITC (Figure 5D). Our data indicate that the AMPK activation via ZMP production from AICAR may contribute to the AICAR-induced nuclear GAPDH accumulation. Because the nuclear GAPDH increased at the higher concentrations (1-2 µM) of 5'-ITC under most conditions, these 5'-ITC concentrations may exert a cellular toxic effect, resulting in nuclear GAPDH accumulation.
To confirm that SFM- and AICAR-induced GAPDH nuclear translocation was mediated through AMPK activation, we examined the effect of an AMPK inhibitor, compound C, on the GAPDH distribution. Compound C in the culture medium with 10% FBS induced GAPDH translocation to the nucleus significantly (P < 0.001) in a dose- and time-dependent manner (Figures 6A and 6B, respectively). Moreover, compound C prevented SFM- and AICAR-induced GAPDH translocation (Figures 6C and 6D, respectively).
Because the inhibition of SFM- and AICAR-induced GAPDH translocation by 10 µM compound C was significant (P < 0.001) but only partial (about 60%), we examined the effect of compound C on SFM- and AICAR-induced AMPK activation by measuring the phosphorylation status of AMPK and its target substrate (acetyl-CoA carboxylase: ACC) through Western blot analysis. A partial inhibitory effect of 10 µM compound C on SFM-induced phosphorylation of AMPK and ACC was observed (Figure 7A). In addition, the same amount of compound C partially prevented the AICAR-induced phosphorylation of AMPK and ACC during a short-term (0.5-2 h), as well as a long-term incubation period (2 days) (Figures 7B and 7C, respectively). These findings indicate that the partial inhibitory effect of compound C might be due to a partial inhibition of AMPK activity.
We also applied an siRNA approach, specific for AMPK, to abolish the expression of AMPK proteins. AMPKα1 and AMPKα2 are the major isoforms of the AMPKα catalytic subunit in HDFs. Therefore, we utilized a mixture of siRNAs to block the expressions of both AMPKα1 and AMPKα2. As depicted in Figure 8A, treatment with AMPKα1/α2 siRNAs for 2 days reduced the total AMPK protein expression and AMPK phosphorylation induced by SFM and AICAR. AMPK depletion by siRNA treatment significantly (P < 0.001) prevented SFM- and AICAR-induced nuclear translocation of GAPDH compared to the mock control group (Figures 8B and 8C, respectively). Our data indicate that AMPK is involved in SFM- and AICAR-induced GAPDH translocation in HDFs.
Previous studies have suggested that S-nitrosylation of GAPDH is required for its nuclear translocation in apoptotic cancer cells (Hara et al., 2005; Hara and Snyder, 2006; Du et al., 2007). However, whether S-nitrosylation is necessary for GAPDH nuclear translocation in all cell types with various stimuli is not known. Therefore, the involvement of S-nitrosylation in SFM- and AICAR-induced GAPDH nuclear localization in HDF cells was examined using the NOS inhibitors L-NMMA and L-NAME. We found that GAPDH translocation by SFM and AICAR in cells treated with NOS inhibitors was similar to that observed in the untreated control cells (Figures 9A and 9B, respectively), indicating that NOS activation is not necessary for SFM- and AICAR-induced GAPDH translocation.
p53 has been demonstrated to be phosphorylated and activated by AMPK (Jones et al., 2005). The treatment of cells with AICAR caused cell cycle arrest in S-phase accompanied with increased expression of p21, p27, and p53 proteins (Rattan et al., 2005). In addition, p53 could be activated by GAPDH nuclear translocation via the formation of a GAPDH-Siah1 complex and subsequent activation of p300/CBP in the presence of apoptotic stimuli (Sen et al., 2008). To determine whether p53 might contribute to GAPDH localization, we performed experiments using p53-null (p53-/-) MEF and HCT116 cancer cells. SFM and AICAR could induce GAPDH nuclear accumulation in both normal and p53-null MEF cells (Figures 10A and 10B, respectively). The effects of SFM and AICAR on GAPDH nuclear accumulation were significantly (P < 0.001) higher in p53-null MEF cells than in normal MEF cells. However, p53-null HCT116 cells exhibited little reduction (P < 0.05 at day 2, P < 0.001 at day 4) in SFM-induced GAPDH nuclear localization compared to normal HCT116 cells (Figure 10C). We observed no changes in AICAR-induced GAPDH nuclear localization between normal and p53-null HCT116 cells (Figure 10D). Our data suggest that p53 activation may not be necessary for SFM- and AICAR-induced GAPDH translocation in both MEF cells and HCT116 cancer cells. The activation of p53 might play an inhibitory role in GAPDH nuclear localization at least in the MEF cell system.
Recently, the CRM1(chromosome region maintenance 1, also called exportin1/Xpo1)-dependent nuclear export system has been demonstrated to operate in determining GAPDH localization (Brown et al., 2004). Because the CRM1-dependent nuclear export can be inhibited by leptomycin B (LMB), we examined the effect of different LMB concentrations (1-20 ng/ml) in the culture medium with 10% FBS for 2 days (Figure 11A) as well as the effect of 10 ng/ml LMB treatment for 1-4 days (Figure 11B). LMB induced the nuclear accumulation of GAPDH at a dose as low as 1 ng/ml within 1 day. The nuclear fraction increased to about 50% after 2 days of treatment with 10 ng/ml LMB. The LMB-induced nuclear accumulation of GAPDH reached a plateau at 50%, even after longer treatment periods or in the presence of higher concentrations of LMB. We also tested the effect of LMB on GAPDH export by the re-addition of 10% FBS for 2 days following complete serum depletion for 4 days. LMB completely prevented FBS-induced GAPDH export at a dose as low as 1 ng/ml (Figure 11C). These data suggest that GAPDH translocation by serum and growth factors can be regulated via the CRM1-dependent nuclear export system.
GAPDH contains a novel CRM1-dependent nuclear export signal (NES) comprising 13 amino acids (KKVVKQASEGPLK) in the C-terminal domain, and truncation or mutation of this NES abrogated the binding of CRM1 and caused the nuclear accumulation of GAPDH (Brown et al., 2004). Because treatment of cells with the inhibitor LMB did not influence the cytoplasmic localization of GFP-GAPDH in NIH3T3 fibroblasts (Schmitz et al., 2003), the involvement of CRM1 in GAPDH export remains controversial. In our experiment, we found that LMB completely prevented FBS-induced GAPDH export after serum depletion for 4 days. This finding supports a positive role of CRM1 in serum- and growth factor-induced GAPDH nuclear export in HDF cells.
It has been suggested that the nuclear export of estradiol receptor alpha (ERα) depends on CRM1 as well as PI3K/Akt activation (Lombardi et al., 2008). Akt-dependent phosphorylation of a forkhead protein Foxo1 (FKHR) drives its association with ERα, thereby triggering the complex export from the nucleus. In this study, we found that a PI3K inhibitor, LY 29004, inhibited serum- or growth factor-induced GAPDH nuclear export in HDF cells, which is in agreement with previous findings (Schmitz, 2001). Therefore, we suggested PI3K as a candidate that regulates GAPDH nuclear export in HDF cells but its regulation mechanism is not yet clear. A similar forkhead family protein might also be associated with GAPDH, and perhaps Akt-dependent phosphorylation of these forkhead proteins could play a role in GAPDH export. This should be verified further.
GAPDH has been reported to undergo autophosphorylation (Kawamoto and Caswell, 1986) as well as phosphorylation via phosphatidylserine-dependent PKCs (Reiss et al., 1996). Although GAPDH export was not altered upon inhibition of PKC by a general PKC inhibitor bisindolylmaleimide II in NIH3T3 cells (Schmitz, 2001), we could not exclude the possibility that the atypical PKC family PKCι/λ could be involved in GAPDH nuclear translocation. The atypical PKCs are activated by the lipid second messenger PIP3 produced by PI3K. PI3K could be activated by EGF- or PDGF-receptor tyrosine kinases. In our study, we observed that a PI3K inhibitor, LY 294002, provided a dramatic inhibition of GAPDH nuclear export. Moreover, GAPDH has been shown to be phosphorylated by PKCι/λ and influence microtubule dynamics in the early secretory pathway (Tisdale, 2002, 2003; Tisdale et al., 2004). Src-dependent PKCι/λ tyrosine phosphorylation is required for PKCι/λ association with Rab2 and GAPDH on pre-Golgi intermediates (Tisdale and Artalejo, 2006). Therefore, it is possible that PIP3-induced atypical PKCι/λ might be involved in GAPDH nuclear translocation.
Because GAPDH also possesses a region homologous to a nuclear localization sequence motif (NLS) between amino acids 259 and 263 (KKVVK), its nuclear transport could occur via this NLS (Sirover, 1999). However, possible regulatory proteins and signaling pathways have not been elucidated. In the current study, we found that a well-known AMPK activator AICAR induced GAPDH nuclear translocation and an adenosine kinase inhibitor 5'-ITC abrogated this change. In the presence of AMPK inhibitors and siRNAs for the inhibition of AMPK activity and blockage of AMPK expression, respectively, we also observed an inhibition of GAPDH translocation. These data suggest that AMPK activation via ZMP production from AICAR may play a role in the nuclear accumulation of GAPDH. Because AICAR inhibits the PI3K/Akt signaling pathway in an AMPK-dependent (Peairs et al., 2009) or AMPK-independent manner (Jhun et al., 2004), a part of AICAR effect on GAPDH nuclear accumulation might be explained by the negative effect on the PI3K/Akt signaling pathway.
AMPK directly phosphorylates and activates p53 (Jones et al., 2005) and AICAR increases p53 expression (Rattan et al., 2005). In addition, p53 could be activated by GAPDH nuclear translocation via the formation of GAPDH-Siah1 complexes (Sen et al., 2008). In our experiments, SFM and AICAR induced GAPDH nuclear accumulation in both normal (p53+/+) and p53-null (p53-/-) MEF and HCT116 cells. Therefore, we suggest that p53 activation may not be necessary for SFM- and AICAR-induced GAPDH translocation in MEF and HCT116 cells.
Because AMPK phosphorylates endothelial NOS on Ser633 and control NO bioavailability in vascular endothelial cells (ECs) (Chen et al., 2009), and S-nitrosylated GAPDH can be translocated to the nucleus under diverse apoptotic stimuli (Hara et al., 2005; Hara and Snyder, 2006; Du et al., 2007), we investigated the involvement of NOS in SFM- and AICAR-induced GAPDH nuclear localization using NOS inhibitors. We observed no effects of NOS inhibitors, such as L-NMMA and L-NAME, on the nuclear translocation of GAPDH, suggesting that S-nitrosylation of GAPDH may not be necessary for SFM- and AICAR-induced nuclear translocation in this cell system.
Based on the current findings, we propose signal transduction pathways involved in the nuclear translocation of GAPDH (Figure 12). GAPDH exists mainly in the cytoplasm in the presence of serum and growth factors. When cells are serum-depleted by SFM or treated with AICAR, GAPDH moves to the nucleus. The re-addition of serum or growth factors to serum-depleted cells causes an export of nuclear GAPDH, which requires the PI3K/Akt signal transduction pathway. The inhibition of PI3K and Akt by LY 294002 and SH-5, respectively, prevents GAPDH export and causes GAPDH accumulation in the nucleus. In contrast, the depletion of serum or growth factors, or treatment with AICAR results in AMPK activation, which may play a role in the nuclear translocation of GAPDH.
Taken together, we conclude that serum-dependent signaling pathways may regulate any import or export processes of GAPDH. The PI3K/Akt signaling pathway regulates the GAPDH nuclear export signal positively or the nuclear import signal negatively. The AMPK signaling pathway, however, works in the opposite way, regulating the GAPDH nuclear import signal positively and its export signal negatively. The involvement of other signaling pathways should be investigated further to explain the molecular mechanism of reversible GAPDH nuclear translocation.
The followings are the reagents used in this study and their sources: PDGF-BB, LPA, LMB, FITC-conjugated goat antimouse secondary antibody, and mouse anti-β-actin monoclonal antibody from Sigma-Aldrich (St. Louis, MO); DMEM, FBS, penicillin, and streptomycin from Gibco/BRL Life Technologies, Inc (Carlsbad, CA); PI3K inhibitor LY 294002, anti-rabbit monoclonal antibodies against phospho-AMPKα (Thr172) and GSK-3β (Ser9), anti-mouse monoclonal antibodies against phospho-Bad (Ser136) and phospho-Akt (Ser473), and anti-rabbit polyclonal antibodies against AMPK-α, Akt, and GSK-3β from Cell Signaling Technology (Denver, MA); compound C, AICAR, SH-5, L-NAME, and L-NMMA from Calbiochem (San Diego, CA); mouse anti-GAPDH monoclonal antibody from Chemicon (Bedford, MA); anti-rabbit monoclonal antibodies against ACC1 and phospho-ACC1 (Ser79) from Upstate (Waltham, MA); horseradish peroxidase (HRP)-conjugated anti-rabbit and anti-mouse secondary antibodies from Vector Laboratories (Burlingame, CA); Lipofectamine™ RNAiMAX and mounting solution including DAPI from Invitrogen Life Technologies (Carlsbad, CA); protein assay kit from Bio-Rad Laboratories (Hercules, CA); enhanced chemiluminescence (ECL) system and Amersham hyperfilm™ ECL from GE Healthcare (Buckinghamshire, UK); sense and complement strands of human AMPK-α1 and α2 siRNAs, siCONTROL complete kit, and 5 × siRNA buffer from Dharmacon Inc. (Lafayette, CO); 5'-ITC from Biomol Research Labs (Plymouth Meeting, PA).
Foreskin human fibroblasts were isolated from newborn foreskins as described previously (Boyce and Ham, 1983). Fibroblasts were maintained in 100-mm tissue culture dishes in DMEM supplemented with 10% FBS and 100 U/ml penicillin and 100 µg/ml streptomycin, and maintained in 5% CO2 in a humidified incubator at 37. Cells from the early stage of culture (population doubling of less than 25) were utilized for this experiment. Prior to serum withdrawal, cells were grown for 2 days to 60-70% sub-confluence in the culture medium with 10% FBS in DMEM, and then serum-depleted by incubation with serum-free DMEM containing 0.1% bovine serum albumin (SFM) for 1-5 days. To examine the effect of serum and growth factors on GAPDH export from the nucleus, cells were cultured for 2 days in 10% FBS in DMEM, then serum-starved for 4-5 days, and then 10% FBS or agonists (PDGF or LPA) were added for the times indicated. For immunofluorescence staining, cells were cultured on coverslips in 6-well culture plates.
Protein expression levels were examined by Western blot analysis, as described previously (Yeo et al., 2000). Total cell lysates were prepared in a lysis buffer containing 50 mM Tris-HCl (pH 7.5), 150 mM NaCl, 2 mM EDTA, 1 mM EGTA, 1 mM Na3VO4, 10 mM NaF, 1 mM DTT, 1 mM PMSF, 25 µg/ml leupeptin, 25 µg/ml aprotinin, 5 mM benzamidine, and 1% Ingepal CA630. Protein concentrations of the lysates were determined using a Bio-Rad protein assay kit, as described by the manufacturer. Cell lysates containing equal amounts of protein were resolved by SDS-PAGE and transferred onto Immobilon PVDF membranes. Blots were blocked with a solution containing 5% nonfat dried milk or 5% BSA and 0.1% Tween 20, and treated with antibodies in the blocking solution overnight, then washed and further probed with HRP-conjugated anti-rabbit IgG (1:5,000). The immune complexes were visualized using an ECL detection system, as described by the manufacturer.
Target sequences for preparing siRNAs of human AMPK-α1 and α2 were as follows: 5'-AGUGAAGGUUGGCAAACAUTT-3' (sense strand) and 5'-AUGUUUGCCAACCUUCACUTT-3' (complement strand) for human AMPK-α1; 5'-GGAAGGUAGUGAAUGCAUATT-3' (sense strand) and 5'-UAUGCAUUCACUACCUUCCTT-3' (complement strand) for human AMPK-α2. A siCONTROL complete kit was used as a negative mock control. Chemically synthesized RNA oligonucleotides were 2'-deprotected, annealed, and desalted as recommended by the manufacturer. RNA duplexes (100 µM stock) resuspended in 1 × siRNA buffer [6 mM HEPES-KOH (pH 7.5), 20 mM KCl, 0.2 mM MgCl2] were transfected with 2.0 × 104 HDF cells at 30-50% confluence. Transfection with siRNAs was performed using Lipofectamine™ RNAiMAX in a 6-well plate as described by the manufacturer. For this purpose, 120 pmol of siRNA duplex was diluted in 100 µl of Opti-MEM I reduced serum medium, and 2 µl of Lipofectamine™ RNAiMAX reagent in 100 µl of Opti-MEM I reduced serum medium, and the diluted siRNA mix and lipid were combined, mixed gently, and incubated for 20 min at room temperature (RT). The lipid and siRNA mix was added to each well (total volume 1.2 ml, 100 nM siRNA). The medium was replaced with culture medium at 4 h after transfection and the cells were incubated for 24-72 h at 37. Cells were then analyzed for changes in AMPK protein expression by Western blotting.
The cells on coverslips in 6-well culture plates were washed twice with ice-cold PBS and fixed in 4% paraformaldehyde in PBS for 10 min, and then washed once with PBS. Nonspecific protein-binding sites were saturated with blocking solution (2% BSA in TBST: 20 mM Tris, 138 mM NaCl, 0.1% Tween 20, pH 7.4) for 1 h with gentle shaking. The cells were incubated with primary monoclonal antibody against GAPDH (1:1,000 in blocking solution) for 1 h at RT and then washed three times with ice-cold TBST for 10 min each. Cells were incubated with FITC-conjugated goat anti-mouse secondary antibody (1:500) in blocking buffer for 1 h. Cells were washed three times with TBST for 10 min each and dehydrated in three washes of 100% methanol over 1 h. The coverslips were mounted on glass slides with solution including DAPI, which fluorescently (blue) labeled the nuclei. Fluorescence images were then observed by laser scanning confocal microscopy (FV500; Olympus, Tokyo, Japan).
To compare the distribution of GAPDH, both FITC fluorescence (green indicates GAPDH location) and DAPI fluorescence (blue indicates the nuclear region) were examined. After cells were stained for cytosolic GAPDH, nuclear GAPDH, or both cytosolic and nuclear GAPDH, 10-20 different fields of each sample were counted under the microscope at 100 × magnification. The data were combined to give total cell numbers of about 1,000 and were converted to percentage distribution. We repeated this experiment at least three times and statistically analyzed the data.
The Student's t-test for paired variables (Office Excel 2007; Microsoft, Redmond, WA) was used to determine whether the index was significantly different as a result of the treatment. Data are presented as the mean ± standard deviation of at least three experiments. P values of less than 0.05 were considered to be statistically significant.
This work was supported by grants from the National Research Foundation of Korea (NRF) through the Ageing and Apoptosis Research Center at Seoul National University (RII-2002-097-08001-0 and RII-2002-097-08003-0) and from the Korea Basic Science Institute (K-MeP).