Physiological levels of ATP Negatively Regulate Proteasome Function

Abstract

Intracellular protein degradation by the ubiquitin-proteasome system is ATP-dependent and the optimal ATP concentration to activate proteasome function in vitro is ~100 μM. Intracellular ATP levels are generally in the low millimolar range but ATP at a level within this range was shown to inhibit proteasome peptidase activities in vitro. Here we report new evidence that supports a hypothesis that intracellular ATP at the physiological levels bidirectionally regulates 26S proteasome proteolytic function in the cell. First, we confirmed that ATP exerted bidirectional regulation on the 26S proteasome in vitro, with the optimal ATP concentration (between 50–100 μM) stimulating proteasome chymotrypsin-like activities. Second, we found that manipulating intracellular ATP levels also led to bidirectional changes in the levels of proteasome-specific protein substrates in cultured cells. Finally, measures to increase intracellular ATP enhanced, while decreasing intracellular ATP attenuated, the ability of proteasome inhibition to induce cell death. These data strongly suggest that endogenous ATP within the physiological concentration range can exert a negative impact on proteasome activities, allowing the cell to rapidly up-regulate proteasome activity upon ATP reduction under stress conditions.

Introduction

Intracellular protein degradation is mainly carried out by the autophagy-lysosome pathway and the ubiquitin-proteasome system (UPS) which is ATP-dependent [1–3]. The UPS is responsible for specific degradation of most intracellular normal and abnormal proteins. In general, UPS-mediated proteolysis includes two steps: ubiquitination of targeted protein molecules and degradation of the ubiquitinated proteins by the 26S proteasome. The 26S proteasome is assembled by the association of the 19S regulatory particle with the 20S proteolytic core particle in an ATP-dependent manner [4, 5]. Besides promoting 26S assembly [5], ATP is also essential to both the ubiquitination reaction and the functioning of 19S proteasome which deubiquitinates, unfolds, and channels the target protein into the proteolytic chamber of the 20S core [6]. Additionally, the 20S proteasome core seems to be able to degrade certain protein targets, such as ornithine decarboxylase (ODC) and oxidized proteins, in an ATP-and ubiquitin- independent fashion [7, 8]. In the past several decades, exciting progress has been made in understanding the general ubiquitination process and how the proteasome works in general [4, 9]. It is emerging that posttranslational modifications of proteasome subunits may have significant impacts on proteasome function [10]. However, our understanding on how the proteasome activity is regulated timely to meet the dynamic demand of cell functions and to harmonize with energy metabolism in the cell remains quite rudimentary.

Intracellular ATP levels are generally in the low millimolar range [11–14], but ATP at a level within this range was shown to suppress proteasome peptidase activities in vitro [15,16]. Proteasome activities in cells facing energy challenge tend to elevate [17, 18]. These observations prompted us to hypothesize that proteasome activities in the cell are geared in a relatively lower state under physiological ATP conditions. Hence, we carried out a series of experiments to test this hypothesis. Our results strongly support this hypothesis, revealing a previously underappreciated mechanism by which the cell reserves its proteasome function at the baseline and rapidly mobilizes the reserve upon a moderate reduction of ATP. This mechanism not only could readily explain a wide variety of (patho)physiological processes but also may potentially be captivated to develop novel strategies to treat life threatening diseases by altering ATP levels in the cell to manipulate proteasome function.

Results

ATP exerts bidirectional regulations on 26S proteasome activities in vitro

The homeostatic level of intracellular ATP ranges generally from 0.5 mM to 5 mM, depending on cell types [11–14]. To test the direct effect of the physiological level of ATP on proteasome function, we first examined the in vitro peptidase activities of purified 26S proteasomes in buffers containing various concentrations of ATP. We found that ATP at a concentration lower than 50 μM stimulated the chymotrypsin (CT)-like activity of purified 26S proteasomes; however, at a concentration higher than ~100 μM, additional ATP did not further stimulate the proteasome but rather showed a dose-dependent suppression on the proteasome activity (Figure 1). This is consistent with previous reports using the crude protein extract of heart tissue as the proteasome donor and purified 26S proteasomes [15, 16]. These in vitro results suggest that ATP at a physiological concentration beyond a minimum level required for 26S proteasome assembly and function may very likely yield an inhibitory effect on proteasome proteolytic activity in the cell and, therefore, decreasing ATP within a physiologically tolerable range will release the inhibition and thereby rapidly increase proteasome proteolytic activities. Our further experimentation as shown below demonstrates that this is indeed the case in the cell.

Figure 1.

ATP bidirectionally modulates in vitro 26S proteasome peptidase activities. Purified 26S proteasomes were treated with ATP at the indicated doses in a Tris reaction system (pH7.4). The chymotrypsin-like (CT-like) peptidase activity was measured using specific synthetic fluorogenic substrates.

Bidirectional regulations of proteasome proteolysis by ATP in vivo

To test whether ATP has the bidirectional effects on 26S proteasomes in vivo, we performed experiments in cultured cells in which ATP production was manipulated and proteasome proteolytic function assessed. Cellular ATP mainly comes from oxidative phosphorylation and glycolysis. Therefore, oligomycin, a specific inhibitor of oxidative phosphorylation was utilized to block ATP production from substrate aerobic oxidation and glucose withdrawal or 2-deoxyglucose (2DG) was employed to reduce glycolysis-dependent ATP production. In K562 and P388 leukemic cells cultured in the D-glucose containing media, oligomycin moderately decreased the levels of intracellular ATP (Figure 2A, 2E) but significantly reduced poly-ubiquitinated proteins and other proteasome substrates including p27 and I-κBα in a dose-dependent manner (Figure 2B, 2F). While in the glucose-free medium or the L-glucose-containing medium (L-glucose cannot be used to generate ATP), oligomycin quickly depleted intracellular ATP (Figure 2A and 2E) and dose-dependently increased the levels of poly-ubiquitinated proteins, p27 and I-κBα (Figure 2B, 2F). When cultured in glucose-free medium for 2 hr, the ATP concentration in K562 cells dropped by approximately 50%, compared with those cultured in the medium containing 2 g/L D-glucose (Figure 2C). Addition of D-glucose to glucose-free medium efficiently increased both the levels of cellular ATP (Figure 2C) and the poly-ubiquitinated proteins (Figure 2D). Similar results were also observed in cultured P388 cells (Figure 2G and 2H). These results suggest that altering intracellular ATP levels seem to produce bidirectional effects on proteasome proteolytic function in the cell, consistent with the in vitro results (Figure 1).

Figure 2.

Severe and moderate reduction of intracellular ATP induces bidirectional changes of proteasome substrates in cultured cells. (A, B) Oligomycin (Oli) induced changes in the ATP levels (A, mean+SD) and changes in the protein levels of ubiquitinated proteins (Ub-prs.), p27 and I-κBα (B) in K562 cells that were cultured in D-glucose (D-Glu)-containing and D-Glu-free media. The ATP levels were measured with the cell lysates collected at 6 h after oli treatment at the indicated doses ( μg/ml). ATP levels in the equal number of cells are presented. The protein levels (B) were analyzed using Western blotting with the cell lysates collected at 24 h after Oli treatment (B). The same membrane was re-probed for GAPDH (GA) as loading controls. Representative images are shown. (C, D) Relative ATP levels (C, Mean+SD) and representative images of Western blotting analysis for Ub-prs in K562 cells that were treated with D-Glu at the indicated doses (g/L) for 2 h (C) and 6 h (D), respectively. (E, F) Relative ATP levels (E) and representative Western blotting images of Ub-prs (F) in P388 cells that were cultured the 1640 RPMI medium and treated with indicated doses of Oli for 2 h (E) and 6 h (F), respectively. D-Glu (+) stands for D-glucose (2 g/L); D-Glu (−) stands for D-glucose-free. (G, H) Relative ATP levels (G) and representative images of Western blotting analysis for Ub-prs (H) in P388 cells that were treated with D-glucose at the indicated doses for 2 h (G) and 6 h (H), respectively.

To further demonstrate that the observed regulation of intracellular ATP levels on proteasome proteolytic function has a functional consequence on the degradation of a proteasome-specific full length protein substrate, we created clonal SH-SY5Y cells stably expressing a degron CL1 fused green fluorescence protein (GFPu), referred to as GFPu-5Y cells. The degradation of GFPu depends on the UPS [19, 20]. This is further verified by the ability of proteasome inhibition to increase GFPu protein levels in the GFPu stably transfected cells (Figure 3A). With 2.5 μg/ml oligomycin treatment, the ATP levels in GFPu-5Y cells were time-dependently decreased (Figure 3B). Western blotting analyses revealed that GFPu protein levels in these cells were significantly decreased at 1 h and 3 h, returned to the control level at 6 h, and became significantly increased at 12 h after oligomycin treatment (Figure 3C). The bidirectional nature of the temporal changes in GFPu protein levels after oligomycin treatment corroborates very well with the in vitro bidirectional effects of ATP on the proteasome peptidase activity.

Figure 3.

Changing intracellular ATP bidirectionally alters the stability of GFPu and GFPdgn in cultured cells. (A) MG132 accumulates GFPu in GFPu-5Y cells (a clonal SH-SY5Y cell line stably transfected with GFPu, a surrogate UPS substrate). DM: DMSO. (B) The time course of oligomycin (Oli, 2.5 μg/ml) induced decreases of ATP levels in GFPu-5Y cells cultured in the glucose-containing medium. (C) Temporal monitoring dose-response of Oli treatment on the GFPu protein levels in GFPu-5Y cells cultured in the glucose-containing medium. (D) Representative Western blotting images showing that MG132 increases GFPdgn but not RFP protein levels in the GFPdgn/RFP stably transfected HEK293 cells. (E, F) Temporal changes in GFPdgn and RFP in the GFPdgn/RFP double-stably transfected HEK293 cells treated with Oli (1.0 μg/ml) in the glucose-free culture medium. A representative set of images of Western blotting for GFPdgn and RFP (E) and a summary of GFPdgn/RFP ratios derived from 6 independent repeats (F) are presented. *P<0.05, ***P<0.001 vs. the same time point vehicle control (DMSO) treatment group.

Reduction of ATP may inhibit protein synthesis, which can also cause a decrease in GFPu protein levels. To further demonstrate that changes in UPS-mediated protein degradation accounts for the observed GFPu changes, we next created clonal HEK293 cell lines with stable double-transfection of GFPdgn and a red fluorescence protein (RFP). Derived from GFPu, GFPdgn is also a validated substrate for the UPS [21]. The RFP is not a specific substrate for the UPS and this is verified by the absence of a change in RFP levels in the face of a marked accumulation of GFPdgn in the GFPdgn/RFP stable cells upon proteasome inhibition (Figure 3D). The RFP expression vector was constructed similarly to that of GFPdgn so that any potential changes in general transcription and translation induced by an ATP manipulation would have a similar effect on both GFPdgn and RFP in the GFPdgn/RFP stable cell lines. Therefore, the use of the GFPdgn/RFP protein ratio to monitor UPS function is more accurate than GFPdgn as the impact from potential changes in protein synthesis on GFPdgn protein levels is now controlled for. As expected, in the absence of D-glucose in the culture medium, oligomycin treatment exerted a typical bidirectional influence on the GFPdgn/RFP ratio. The GFPdgn/RFP ratio was significantly decreased at 1 h and 2 h, returned to nearly the control level at 3 h, and significantly increased at 6 h after the oligomycin treatment (1 μM, Figure 3E, 3F).

Taken together, the findings from the cell culture experiments recapitulate nicely the in vitro findings described earlier (Figure 1) and previously reported by others [15, 16], strongly supporting a bidirectional regulation of ATP over proteasome function in the cell. In the activation arm, a below-a-threshold ATP concentration is positively correlated with proteasome function; in the inhibition arm, however, a beyond-the-threshold ATP concentration is negatively correlated with proteasome function. The threshold was roughly 50~100 μM under the in vitro condition used in the present study (Figure 1). The threshold in intact cells is not exactly defined at this time but our data clearly reveal that it is substantially lower than the normal ATP level in the cell. The activation arm is consistent with what is already known [5, 6, 22], while the inhibition arm had not been well demonstrated in the cell although it had been recently implicated by a few studies [15,16].

ATP levels determine the efficacy of proteasome inhibition to cause cell death

It is well known that proteasome inhibition can induce apoptosis and/or necrosis. Based on the parabolic feature of the dose-response curve of ATP modulating the 26S proteasome activity, we hypothesize that a higher intracellular ATP level within “the inhibition arm” would make proteasome inhibitors more effective in inducing cell death. ATP concentration of cells cultured in the D-glucose-containing medium is considered within the physiological range because this medium provides the optimal condition for cell culture. Several ATP states were modeled and then cell death induced by the proteasome inhibitors MG132 or MG262 was temporally assessed.

First, as shown in Figure 2A and 2C, the ATP level in K562 cells cultured in the glucose-free medium was about 50% of that in the D-glucose medium. Annexin V-propidium iodide (PI) double-staining followed by flow cytometry revealed that MG262 (62.5 nM ~ 1.0 μM, Figure 4A, 4B) or MG132 (1 ~ 20 μM, Figure 4C) in a range of doses induced significant more cell death in the D-glucose containing medium than in the glucose-free medium. This is further demonstrated by imaging the membrane permeability of living cells in PI-containing culture medium (Figure 4D).

Figure 4.

Intracellular ATP concentration determines the efficacy of proteasome inhibition to induce cell death. (A) Cell viability assays by flow cytometry. K562 cells were cultured in the 1640 RPMI glucose-free medium with or without the addition of D-glucose (D-Glu, 2 g/L). After treated with MG262 at the indicate doses for 36 h, the cells were collected and subjected to Annexin V-FITC/propidium iodide (PI) double staining for flow cytometry. The lower right quadrant (Annexin V-FITC+/PI-) was considered as early stage apoptotic cells, the upper right quadrant (Annexin V-FITC+/PI+) was considered late stage apoptotic cells, and the upper left quadrant (Annexin V-FITC-/PI+) was considered as necrotic cells. (B) Summaries of changes in the percentage of viable cells (i.e., percentage of cells in the lower left quadrant) as assessed in the experiments shown in panel A. (C) Removal of glucose from the culture medium increases the resistance of K562 cells to MG132-induced cell death. K562 cells were treated with MG132 at the indicated doses for 24 h in the presence or absence of D-glucose (2 g/L) in the 1640 RPMI medium. Cell viability was assayed by flow cytometry as described for in panel A. (D) Representative micrographs of live cultured cells with in situ staining for cell death. K562 cells were treated with MG132 (10 μM) or MG262 (1 μM) for 24 h in the absence or presence of D-glucose in the culture medium. PI was added to the medium and 15 min later, the cells on the culture dish were directly imaged for both PI-positive staining (red) and the phase contrast using an inverted fluorescence microscope. The merge images between red fluorescence and the phase-contrast images are shown. Scale bar=50 μm. (E) K562 cells were treated with MG132 (5 μM) or MG262 (0.5 μM) for 12 h in the 1640 RPMI D-glucose medium in the absence or presence of oligomycin (Oli, 0.5 μg/ml), followed by Annexin V-PI double staining for cell death assay via flow cytometry. A representative image of each group from three independent repeats is shown. (F) A summary of the incidence of the early and late apoptosis in the groups treated with MG132 as shown in (E). Oli co-treatment delayed the induction of apoptosis by MG132. Mean+SD, n=3. (G) A summary of percentage viable cells treated by MG262 as shown in (E). Mean+SD, n=3. *P<0.01, vs. DM control; ^#P<0.01, vs. MG262 treatment.

Second, oligomycin decreased ATP content by ~20% in K562 cells cultured in normal D-glucose (2 g/L) containing medium (Figure 2A). Under this condition, oligomycin significantly attenuated the ability of MG262 to induce cell death (Figure 4E, 4G) and markedly shifted MG-132 induced apoptosis from the late stage to the early stage (Figure 4E, 4F). To further compare the effects of three different levels of intracellular ATP on proteasome inhibition-induced cell death, the ATP concentration was set at approximately 100%, 80%, or 50% of the normal level, respectively, by culturing the cells in the D-glucose medium, the D-glucose+oligomycin medium, or the glucose-free medium. By temporally monitoring PI-positive nuclear staining of live cells cultured in these conditions, we confirmed that the effectiveness of MG132 (5 μM) to induce cell death is time-dependent but the effectiveness decreased dose-dependently as the ATP was forced to decrease from 100% to 80% and 50% of the normal level (Figure 5).

Figure 5.

Temporal monitoring cell death induced by proteasome inhibition in live cells cultured under various ATP states using propidium iodide (PI) staining and an inverted fluorescence microscope. In this setting, dead or dying cells stain red by PI. Representative fluorescence micrographs of PI-stained living K562 cells taken at the indicated time points after MG132 (5 μM) treatment are shown. The relative intracellular ATP concentrations were set at approximately 100%, ~80%, and ~50% of the normal level respectively by culturing the cells in the D-glucose medium, the D-glucose +oligomycin medium, and the glucose-free medium. As the ATP decreased, the effectiveness of MG132 to induce cell death decreased. As the time of treatment went on, MG132 induced cell death increased in all the three ATP states.

Unlike D-glucose, L-glucose can not be utilized by the cell to produce ATP. To control for the potential non-ATP increasing effects of D-glucose, the impact of D-glucose and L-glucose on proteasome inhibition-induced cell death was compared in K562 cells. D-glucose but not L-glucose at the equivalent dose significantly enhanced MG262- or MG132-induced cell death as revealed by the cell death assay using the flow cytometry after the Annexin V-PI double staining (Figure 6A~6C) as well as the detection of LDH release from the cell to the culture medium (Figure 6D). The cell death data were also confirmed by additional morphological analyses for chromosome condensation and nuclear fragmentation (Figure 6E, 6F), and characteristic cell shape changes (Figure 6G). These additional control experiments confirm that the enhancing effect of D-glucose on the induction of cell death by proteasome inhibition is only attributable to the increase of ATP production.

Figure 6.

Comparison of the effects of L- and D- glucose (Glu) on proteasome inhibition-induced cell death in cultured K562 cells. K562 cells were treated with MG262 (0.5 μM) or MG132 (5 μM) for 9 h or 18 h in the 1640 RPMI medium with L-Glu (not usable by the cell to produce ATP) or D-Glu. Cell death was detected by Annexin V/PI double staining and flow cytometry. (A, B) Representative flow cytometric dot plots of the K562 cells undergone the indicated treatment for 9 h (A) or 18 h (B). (C) A summary of cell viability data derived from experiments shown in (A) and (B). (D) LDH activity in the culture medium derived from the experiments shown in (B). (E) Nuclear morphology of K562 cells treated with M132 (5 μM) in L-Glu or D-Glu containing medium for 12 h. The nuclei of fixed cells stained blue by Hoechst. Phase contrast and blue fluorescence were imaged with epi-fluorescence microscopy. Chromatin condensation is more prevalent in the D-Glu group than the L-Glu group. (F) Representative transmission electronic microscopy (EM) micrographs of cells treated as described in (A). Nuclear fragmentation and chromatin condensation are evident only in the D-Glu group. (G) As described in (A), K562 cells were treated with MG132 (5 μM), followed by recording the temporal morphological changes at 6 h, 9 h and 12 h. Representative phase-contrast images were shown. Cell disintegration and apoptotic bodies emerged much earlier and more frequently in the D-Glu group, compared with the L-Glu group after MG132 treatment.

Since glycolysis plays a major role in ATP generation, we next used 2DG in K562 cells to inhibit glycolysis as an alternative way to decrease ATP production and investigated its effect on proteasome inhibition-induced cell death. As shown in Figure 7A, 2DG significantly decreased ATP concentration and, as expected, significantly attenuated MG132-induced cell death (Figure 7B, 7C). Essentially the same results were also obtained when a similar experiment was performed using a human lung cancer cell line (H460), in which a moderate inhibition of ATP generation by 2DG significantly attenuated MG132-induced LDH release and cell death (Figure 7D~7F).

Figure 7.

Inhibition of glycolysis by 2DG decreases intracellular ATP and rescues MG132 induced cell death in K562 and H460 cells. (A) ATP levels in the lysate of K562 cells that were treated with 2DG (5 mM) or DMSO (DM) in the D-glucose 1640 RPMI medium for 3 h and 12 h, were assayed using HPLC. (B) For cell death assay, cells were treated by MG132 (10 μM) for 12 h in the presence of 2DG (2.5 mM, 5 mM) in the RPMI 1640 medium. Cells were collected and labeled by Annexin V and PI for flow cytometry assessment of cell death. Representative images are shown. (C) A statistical summary of the data were illustrated. *P<0.01, compared with control treatment; ^#P<0.01, compared with MG132 treatment alone (D) H460 cells were treated with MG132 (5 μM) or DMSO in the absence or presence of 2DG (5 mM) for 12 h, followed by Annexin V-PI staining for cell death assay. Representative images of cell death analyses by flow cytometry were shown. (E) Bar graph summarizing the cell death data illustrated in panel (D). (F) LDH activities in the culture medium derived from the experiments illustrated by panel (D).

Notably, the increased resistance to proteasome inhibitor-induced cell death by a moderate reduction of intracellular ATP is time-dependent. It was only observed in the initial period of the time after the administration of a proteasome inhibitor. Comparable cell death occurred eventually in all groups treated with the proteasome inhibitor when they were observed for sufficiently long time (data not shown). In other words, the reduction of ATP only significantly delayed proteasome inhibition-induced cell death.

All the results reported in this manuscript support a conclusion that a decrease of intracellular ATP concentration in the inhibition arm attenuates proteasome inhibition-induced cell death at these early time points tested. These results therefore lend additional support to the hypothesis that physiological levels of ATP negatively regulate proteasome function.

Discussion

It is well known that the 26S proteasome is an ATP-dependent multimeric protease in the cell. Through both in vitro and cell culture experiments, the present study has demonstrated that intracellular ATP levels beyond a threshold but well within the homeostatic range are negatively correlated to proteasome proteolytic activities and intracellular ATP below a threshold is positively associated with proteasome activities. This helps unveil that ATP is a critical small molecule that may regulate proteasome function in the cell in two opposing directions, depending on its levels. This contention challenges the traditional dogma on ATP-mediated regulation of the proteasome function. As elaborated below, this new revelation of the effect of changing ATP levels on proteasome function is of potentially high significance and may potentially be exploited to design new therapeutic strategies to combat a variety of diseases, including some of the life-threatening ones.

First, the findings of our study help expand current understanding on the regulation of proteasome by intracellular ATP. The traditional view has been that ATP is required for and stimulates the assembly and functioning of the 26S proteasome. Our study shows that this view is still true but represents only the half of the picture, only the activation arm. We provide additional evidence here helping reveal the other half of the picture, the inhibition arm, in which ATP at a level beyond a threshold appears to negatively impact on proteasome function in the cell. The threshold is likely the minimum ATP concentration required for 26S proteasome assembly and the UPS to function in the cell. According to in vitro assessments (Figure 1), the threshold is likely in the tens to one hundred μM range which is at least one order of magnitude lower than the normal intracellular ATP level which is usually in the low mM range [11–14]. Therefore, the basal level of ATP exerts constitutively a negative regulatory effect on proteasome function in the cell, serving likely as a layer of safeguard for the proteasome reserve. The existence of the inhibition arm of ATP-mediated regulation over the proteasome conceivably allows the cell to rapidly up-regulate its proteasome activities upon ATP-reduction which often accompanies cellular stress. Indeed, gentle decreases of intracellular ATP by multiple means, such as the administration of oligomycin or of 2DG and glucose withdrawal, were all able to significantly increase proteasome proteolytic function in the cell (Figures 2 and 3). The precise mechanism underlying the bidirectional regulation of ATP over proteasome activities remains to be futher explored. Both direct and indirect effects from ATP may be invovled.

In many pathological conditions, this suggested regulation appears to be in play as well. It was reported that proteasome peptidase activities were significantly increased in the heart under pressure overload, during which myocardial ATP levels were lower than normal [23]. Interestingly, pharmacological proteasome inhibition markedly suppressed pressure overload cardiac hypertrophy [23]. Muscle wasting by proteasome activation has been confirmed in chronic occlusive pulmonary disease (COPD) both in vitro and in vivo [17, 24, 25]. Severe acute hypoxia is seen in the acute respiratory distress syndrome (ARDS). Administration of proteasome inhibitors was shown to abrogate the hypoxia-induced severe pulmonary distress [26], suggesting that proteasome activation plays a pathogenic role in ARDS and decreased ATP production may be responsible as well. Another example is ischemia where decreases in ATP are common and again the proteasome is often activated during the early stage of ischemia and proteasome inhibition often ameliorate ischemic injury [27]. These examples seemly share the sequela that decreases in intracellular ATP under the stress conditions are accompanied by proteasome activation and the use of proteasome inhibitors is often beneficial in managing the stress. It was recently reported that prolonged glucose infusion in vivo could inhibit the proteasome function and decreases myofibrillar protein degradation [28]. It was further confirmed that glucose infusion, even at a relatively low rate, suppresses muscle protein breakdown in the early postoperative period via suppression of the UPS [29]. Direct ATP infusion increases liver energy status and slowed down weight loss in advanced lung cancer patients [30].

Second, the new contention strengthened by the present study may unveil a new mechanism by which the cell mobilizes its proteolytic capability in response to starvation. It is well documented that macroautophagy is activated upon starvation to allow the cell to self-digest a portion of the cytoplasm for survival [31, 32]. Starvation inevitably decreases intracellular ATP; therefore, according to our new findings, proteasome-based proteolytic activity will also be increased at least at the initial stage of starvation when the ATP level is only moderately decreased. This is directly demonstrated by our data that glucose withdrawal decreases the level of proteasome substrates in cultured cells (Figures 2 and 3) and slows down cell death induced by proteasome inhibitors (Figure 4).

Third, the inhibition arm of the bidirectional regulation of ATP over the 26S proteasome provides a rationale for manipulating intracellular ATP concentrations to alter proteasome function in the cell. The latter has tremendous therapeutic implications because, for instance, modulating proteasome proteolytic function has been shown experimentally and/or clinically to be remarkably effective in mitigating a variety of pathological processes that are essential to the genesis and progression of a large set of life-threatening diseases, such as cell proliferative diseases. To this end, we have demonstrated that increasing ATP production can synergize with pharmacological proteasome inhibitors to induce cell death of cultured cancer cells while decreasing ATP production antagonizes proteasome inhibition induction of cell death (Figures 4~7).

Hypoxia is commonly found in solid tumors and up-regulates a number of target genes involved in angiogenesis, anaerobic energy metabolism, cell survival, cell invasion and drug resistance, thereby contributing to the progression of a more malignant phenotype and to the increased resistance to radiotherapy and chemotherapy [33]. Based on the bidirectional regulation of ATP over proteasome function, the reduction of ATP associated inevitably with hypoxia should activate the proteasome in the cancer tissue. Indeed, cancer tissue proteasome activities are generally significantly higher than the normal tissue from which the cancer originates. Moreover, it has been shown that administration of a proteasome inhibitor such as bortezomib can sensitize cancer cells to radiotherapy and chemotherapy [34–36]. Administration of these pharmacological inhibitors often unfortunately yields unintended severe adverse effects, such as congestive heart failure [37]. Hence, increasing intracellular ATP may be a safe alternative measure to inhibit proteasomes in cancers and thereby sensitizing the cancer cells to radiotherapy and chemotherapy. Consistent with this postulate, intracellular ATP concentration has proven to be an important determinant for cell death [38–42].

Materials and Methods

Materials

ATP, Hochest 33258 and oligomycin (No. 04876) were purchased from Sigma-Aldrich (St. Louis, MO, USA). 2-Deoxyglucose and L-glucose were purchased from Alfa Aesar (Karlsruhe, Germany), mouse monoclonal antibodies against GFP (clone 2), RFP, ubiquitin (P4D1), p27 (F-8), tubulin and rabbit polyclonal antibodies against GAPDH (FL-335) and I-κBα (C-15) were from Santa Cruz Biotechnology Inc. (Santa Cruz, CA, USA). Enhanced chemiluminescence (ECL) reagents were from Amersham Biosciences (Piscataway, NJ, USA). Annexin V-FITC Apoptosis Detection Kit was from Keygen Company (Nanjing, China).

Cell culture and ATP manipulation

K562, P388, and NCI-H460 cells were purchased from the American Type Culture Collection (ATCC) and cultured in the RPMI1640 medium (GIBCO, USA) supplemented with 10% fetal bovine serum (HyClone, Logan, UT, USA). SH-SY5Y cells and HEK293 cells were purchased from ATCC and cultured in DMEM medium with high glucose supplemented with 10% fetal bovine serum (HyClone, Logan, UT, USA). Oligomycin, a classic inhibitor of F0F1-ATPase, was used to block ATP production from oxidative phosphorylation; withdrawal of D-glucose from the culture media was employed to reduce glucose-dependent ATP production; 2DG was used to block glycolysis-dependent ATP production.

Peptidase activity assays

These were performed as we previously described (43, 44). A 20 μl of Tris-HCl buffer (pH 7.4) containing purified 26S proteasomes (4 nM, Boston Biochem, Cambridge, MA, USA) were added to a total volume of 180 μl Tris-HCl (pH 7.4) reaction buffer containing the synthetic fluorogenic peptide Suc-LLVY-aminomethylcoumarin (AMC) for the chymotrypsin-like activity (final concentration = 25 μM, Calbiochem, USA). The reaction mixture was then incubated at 37°C for 90 min and analyzed for the fluorescence intensity of the free AMC using a luminescence microplate reader (Varioskan Flash 3001, Thermo, USA). The excitation and emission wavelengths for measuring free AMC were 360 nm and 436 nm, respectively.

Creation of SH-SY5Y GFPu stable cell lines

SH-SY5Y cells were purchased originally from ATCC. GFPu, a green fluorescence protein (GFP) modified by carboxyl fusion of degron CL1, was previously proven a specific surrogate substrate for the UPS [19, 20]. A GFPu expressing plasmid was used to transfect the SH-SY5Y cells using a liposome-based transfection kit from Nanjing Keygen (Nanjing, China). The transfected cells were selected for stable transfection using G418 as previously described [42]. The selected stably transfected clones were maintained in growth medium containing G418. These cells are referred to as GFPu-5Y cells in the main text.

Creation of HEK293 GFPdgn/RFP stable cell lines

As previously described for generating the GFPu-2 stable cell lines [20], HEK293 cells from ATCC were co-transfected with pGFPdgn and pDSRed2-C1 plasmids using Lipofectamine 2000 (Invitrogen, Carsbad, CA, USA). Derived from the original GFPu vector [19], the pGFPdgn vector was previously used to generate the GFPdgn transgenic mice and described therein [21]. The pDSRed2-C1 encoding a red fluorescence protein (RFP) was purchased from Clontech (Mountain View, CA, USA).

ATP content determination

Equal number of cultured cells were collected and centrifuged for 5 min at 3 000×g at 4 °C and the cell pellet was immediately frozen and stored in liquid nitrogen for subsequent ATP analyses. The frozen cells were resuspended in perchloric acid and lysed on ice. The lysates were centrifuged at 12 000 rpm × 10 min at 4 °C. The supernatant was collected for analyzing ATP by using a reversed-phase, C18 HPLC (LC-6AD, Shimadzu, Japan) assay after the pH was adjusted 7.4 [45]. 180 mM of KH₂PO₄ (5% methanol) was used as mobile phase (pH 6.25) running at 0.8 ml/min. The assay was linear from 0.05 to 200 μg/mL for ATP with coefficient of determination (R²) >0.999. Validation coefficients of variation for intra- and inter-day assays were less than 1.5% and 5.1%, respectively.

Western blot analysis

Western blotting was performed as previously described [43]. In brief, an equal amount of total protein extracts from cultured cells were fractionated by 12% SDS-PAGE and electrically transferred onto polyvinylidene difluoride (PVDF) membranes. Mouse, goat or rabbit primary antibodies and horseradish peroxidase (HRP)-conjugated appropriate secondary antibodies were used to detect the designated proteins. The bounded secondary antibodies on the PVDF membrane were reacted to the ECL detection reagents (Amersham Bioscience, Dübendorf, Switzerland) and exposed to X-ray films (Kodak, Japan) or directly imaged and digitalized using a BioRad VersaDoc 4000 imaging system and quantified by the Quantity One software (BioRad, CA, USA). The x-ray film exposure was scanned and digitalized using a high-resolution scanner. The density of desired bands was quantified with the Scion Image Analyzing software. For the quantification of total ubiquitinated proteins, all positive bands with a molecular weight greater than that of free Ub (7.6 kDa) were included.

Cell death assay

This was performed using Annexin V-FITC and propidium iodide (PI) double staining followed by flow cytometry as previously described [43]. In brief, cultured K562 and H460 cells were harvested and washed with cold PBS and resuspended with the binding buffer, followed by Annexin V- FITC incubation for 15 min and PI staining for another 15 min at 4 °C in dark. The stained cells were analyzed with flow cytometry within 30 min.

Lactate dehydrogenase (LDH) activity assay

Release of LDH from the cytoplasm of cultured cells to the culture medium indicates a loss of plasma membrane integrity. Culture medium was collected from individual dishes or wells, and cell debris was removed by centrifugation. LDH activity in the collected medium was measured using the cytotoxicity detection kit (Keygen, Nanjing, China) by the reduction of lactate to pyruvate in the presence of NAD. The resultant NADH reduces tetrazolium to a red formazan product that is detectable at 490 nm. Briefly, 100 μl of reaction reagent were added to each well of a 96-well plate containing 100 μl of optimally titrated culture medium, and the mixture was incubated for 30 min at room temperature. Absorbance of the samples at 490 nm was read on a microplate reader (Sunrise, Tecan, Austria). The reference wavelength was 620 nm. LDH activity was calculated according to the standard curve as μmol/L. Results from at least four separate experiments are presented.

Morphological characterization of cell death

K562 cells were treated as described. To monitor temporal changes in the incidence of cell death in the live culture condition, PI was added to the cell culture medium and at the desired sequential time points the cells in the culture dish were imaged with an inverted fluorescence microscope equipped with a digital camera (Axio Obsever Z1, Zeiss, Germany). PI is not able to enter the normal live cells but the dying or dead cells lose their membrane integrity so that PI can enter their nucleus, bind to double-stranded DNA, and thereby positively stain the dying and dead cells. To observe the nuclear changes, K562 cells were collected, smeared on a slide, and stained with Hochest 33258. The Hochest stained cells were imaged with the inverted epi-fluorescence microscope.

For electron microscopy, the cells were washed and fixed overnight at 4 °C with 2% glutaraldehyde in 0.2 mol/L sodium cacodylate buffer, dehydrated in a graded series of buffers, embedded in resin, and sectioned. The ultrathin sections were post-stained in uranyl acetate and lead citrate and observed with a transmission electron microscope (JEM-100CXII, JEOL, Japan).

Statistical methods

Unless indicated otherwise, Mean+SD are presented where applicable. Unpaired Student’s t-test or one way ANOVA is used where appropriate for determining statistic probabilities. P value less than 0.05 is considered significant.