PML Regulates Apoptosis at Endoplasmic Reticulum by Modulating Calcium Release

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Science  26 Nov 2010:
Vol. 330, Issue 6008, pp. 1247-1251
DOI: 10.1126/science.1189157


The promyelocytic leukemia (PML) tumor suppressor is a pleiotropic modulator of apoptosis. However, the molecular basis for such a diverse proapoptotic role is currently unknown. We show that extranuclear Pml was specifically enriched at the endoplasmic reticulum (ER) and at the mitochondria-associated membranes, signaling domains involved in ER-to-mitochondria calcium ion (Ca2+) transport and in induction of apoptosis. We found Pml in complexes of large molecular size with the inositol 1,4,5-trisphosphate receptor (IP3R), protein kinase Akt, and protein phosphatase 2a (PP2a). Pml was essential for Akt- and PP2a-dependent modulation of IP3R phosphorylation and in turn for IP3R-mediated Ca2+ release from ER. Our findings provide a mechanistic explanation for the pleiotropic role of Pml in apoptosis and identify a pharmacological target for the modulation of Ca2+ signals.

The promyelocytic leukemia gene (PML) was originally identified at the breakpoint of the t(15;17) translocation of acute promyelocytic leukemia (APL), and function of the PML protein is frequently lost or aberrant in human solid tumors and hematopoietic malignancies (1, 2). PML is a nuclear protein and an essential component of subnuclear structures termed nuclear bodies (NBs) (3). However, many, if not all, PML isoforms have shown both cytoplasmic and nuclear localization (4, 5). Pml−/− mice and primary cells are protected from apoptosis triggered by a number of diverse stimuli (6).

To determine how PML could regulate such broadly diverse apoptotic responses, we analyzed its intracellular localization by cell fractionation (7, 8). We fractionated homogenates of primary mouse embryonic fibroblasts (MEFs) by ultracentrifugation, focusing on the mitochondria, endoplasmic reticulum (ER), and mitochondria-associated membranes (MAMs), the structures that contain sites where the ER contacts mitochondria. Pml localized both to the nucleus and the cytosol and appeared to localize also to the ER, MAM, and crude mitochondrial fractions but not to “pure” mitochondrial fraction free of ER and nuclear markers (Fig. 1A). These results were confirmed by immunogold labeling of ultrathin cryosections showing that Pml associates with the surface of the ER (Fig. 1B, a and b) and in the proximity of the mitochondrial membrane at contact sites between the ER and mitochondria (Fig. 1B, d to g).

Fig. 1

Identification of Pml at ER and MAM regions and Ca2+-mediated Pml-dependent cell death. (A) Detection of Pml by immunoblotting in Pml+/+ MEFs fractionation. IP3R, tubulin, proliferating cell nuclear antigen (PCNA), and voltage-dependent anion channel (VDAC) are used as markers. H: homogenate; Mc: crude mitochondria; Mp: pure mitochondria; ER; MAM; C: cytosol; N: nucleus. (B) Immunogold labeling of Pml near the rough ER (r), mitochondria (m), and MAM (arrowheads) in Pml+/+ MEFs. Gold particles (15 nm) are mostly associated with the surface of the ER (7.07 gold particles/μm2) and more occasionally with mitochondrial membranes (3.08 gold particles/μm2) (a and b). Specificity of the antibodies is demonstrated by labeling of nuclear bodies (n) (c). Morphologically identified MAM often demonstrated labeling at contacts between ER and mitochondria [(d) to (g), and arrowheads in insets therein]. Insets correspond to boxed areas. Bar: (a) 360 nm; (b) 340 nm; (c) 370 nm; (d) 188 nm, inset 120 nm; (e) 260 nm, inset 190 nm; (f) 340 nm, inset 180 nm; (g) 280 nm, inset 210 nm. (C) Apoptosis induced by 1 mM H2O2, 15 μM menadione (MEN), 6 μM tunicamycin (TN), 2 μM thapsigargin (TG), or 50 μM etoposide (ETO) in Pml+/+ or Pml−/− MEFs treated for 12 hours. Data represent the mean SD of five independent experiments.

In view of the localization of Pml at the ER and MAM, we investigated its requirement in apoptosis induced by ER stress (9). Matched wild-type (Pml+/+) and Pml−/− MEFs were treated with ER stress inducers: H2O2 and menadione (MEN), two oxidizing agents that induce ER Ca2+ release; tunicamycin (TN) or an inhibitor of protein N-glycosylation; and thapsigargin (TG), an inhibitor of the sarcoplasmic/ER Ca2+-ATPase (adenosine triphosphatase). After 12 hours of treatment, the percentage of apoptotic cells in Pml−/− MEFs was much lower than that observed in Pml+/+ MEFs under all treatment conditions (Fig. 1C and fig. S1).

MAMs are specialized domains selectively enriched in critical Ca2+ signaling elements, which mediate Ca2+ transfer between ER and mitochondria (10, 11), such as the inositol 1,4,5-trisphosphate receptor (IP3R) (12). Ca2+ signaling has a major role in the regulation of cell death (13, 14). Release of the ER Ca2+ pool through the type 3 IP3R (IP3R3) appears to induce a sensitization of cells to apoptotic stimuli (15, 16).

To investigate the role of Pml in Ca2+ homeostasis, we used recombinant Ca2+-sensitive bioluminescent protein aequorin (17). In Pml+/+ MEFs, the Ca2+ concentration ([Ca2+]) in the lumen of the ER ([Ca2+]ER) at steady state was ~450 μM, whereas in Pml−/− MEFs it was lower. When the cells were stimulated with adenosine 5′-triphosphate (ATP), the P2Y receptor agonist that causes release of Ca2+ from the ER, the decreases in the [Ca2+]ER observed in Pml+/+ MEFs in quantitative and kinetic terms were larger and faster than in Pml−/− MEFs, reflecting a more rapid flow of Ca2+ through the IP3R (Fig. 2A). In turn, the [Ca2+] increases evoked by stimulation with ATP in the cytosol ([Ca2+]c) and mitochondria ([Ca2+]m) were smaller in Pml−/− than in Pml+/+ MEFs (Fig. 2, B and C, and fig. S2). A mitochondrial Ca2+ deregulation was observed also in human-derived cells in which PML was depleted (fig. S3) and in different cellular models of APL (fig. S4).

Fig. 2

Intracellular Ca2+ homeostasis in Pml+/+ and Pml−/− MEFs. (A to C) ER (A), cytosolic (B), and mitochondrial (C) Ca2+ homeostasis measurements with aequorins. Where indicated, cells were treated with 100 μM ATP. Pml+/+: [Ca2+]ER peak 448 ± 32 μM; [Ca2+]c peak 3.3 ± 0.16 μM; [Ca2+]m peak 138 ± 14 μM. Pml−/−: [Ca2+]ER peak 386 ± 42 μM; [Ca2+]c peak 2.65 ± 0.23 μM; [Ca2+]m peak 78 ± 10 μM. n = 15 samples from five independent experiments, P < 0.01. (D) MEFs loaded with calcium-sensitive fluorescent dye fura-2 were stimulated with menadione (MEN) or H2O2. The kinetic behavior of the [Ca2+]c response is presented as the ratio of fluorescence at 340 nm/380 nm. In these, and other fura-2 experiments, the traces are representative of at least 10 single-cell responses from three independent experiments. (E) Analysis of [Ca2+]m during oxidative stress. Where indicated, cells were stimulated with 30 μM MEN or 2 mM H2O2. n = 10 samples from three independent experiments.

We then investigated whether the absence of Pml could alter the increases in [Ca2+]c and [Ca2+]m induced by apoptotic stimuli. In Pml−/− MEFs, the increases in [Ca2+]c and [Ca2+]m, evoked by the oxidative apoptotic stimuli, such as MEN and H2O2 that trigger both a progressive release of Ca2+ from the ER and an activation of the capacitative Ca2+ influx (18), were smaller as mentioned above (Fig. 2, D and E).

To determine whether the effects of Pml on regulation of Ca2+ homeostasis depend on its localization to the ER and MAMs, we generated a chimeric protein containing the entire PML protein that was targeted to the outer surface of the ER (19). This chimera, designated erPML, localized to the ER and MAMs in Pml−/− MEFs, as revealed by immunocytochemical staining, immunogold labeling, and subfractionation (Fig. 3A and fig. S5). The introduction of erPML in Pml−/− MEFs restored Ca2+ signals evoked by either agonist (Fig. 3B and fig. S6) or apoptotic stimuli (MEN or H2O2) (Fig. 3C) to values comparable to those in Pml+/+ MEFs (Fig. 2, C and D). This effect was associated with a reestablished sensitivity to apoptosis induced by ER stress but did not restore the sensitivity to etoposide (ETO) (Fig. 3D and fig. S7A), a DNA-damaging agent that triggers apoptotic death by a Ca2+-independent process (fig. S7B). Overall, these experiments indicate that the absence of Pml causes a reduction in the amplitude of Ca2+ signals induced by ATP, other agents, or apoptotic stimuli, and that forcing PML to the ER rescues these defects. A PML protein targeted to the nucleus restored the formation of NBs, but did not restore the Ca2+ responses and the sensitivity to ER stress–dependent cell death, although it restored response to other apoptotic stimuli such as ETO (fig. S8).

Fig. 3

erPML chimera reestablishes the [Ca2+]m and apoptotic responses in Pml−/− MEFs. (A) Schematic map of the erPML chimera and immunofluorescence image, stained with the antibody to PML, of Pml−/− MEFs expressing erPML. (B) erPML reestablishes the agonist-dependent [Ca2+]m response in Pml−/− MEFs ([Ca2+]m peak 135 ± 12 μM) to values comparable to those of Pml+/+ MEFs. (C) Pml−/− and Pml−/− MEFs expressing erPML previously incubated with fura-2 were stimulated with menadione (MEN) or H2O2. (D) Representative microscopic fields of Pml−/− MEFs and Pml−/− expressing erPML before and after treatment with 1 mM H2O2, 15 μM MEN, or 50 μM etoposide (ETO) for 16 hours.

To investigate the mechanism underlying these activities of Pml, we tested whether Pml could functionally and physically interact with the IP3R3. Immunoprecipitation of IP3R3 led to the coprecipitation of Pml (Fig. 4A and fig. S9) and vice versa (fig. S10). Amounts of phosphorylated-IP3R3 (p-IP3R3) were higher in Pml−/− than in Pml+/+ MEFs (Fig. 4A and fig. S11).

Fig. 4

Modulation of [Ca2+]m and apoptotic responses by Pml through Akt- and PP2a-dependent phosphorylation of IP3R3. (A) Coimmunoprecipitation of IP3R3 with Pml, Akt, and PP2a in Pml+/+ MEFs. In the same blot, the levels of p-IP3R3 and pAkt are shown. (B) Localization of Pml (green) and PP2a (red) at ER and MAM sites in Pml+/+ MEFs analyzed by immunofluorescence. FACL [long-chain fatty acid–CoA (coenzyme A) ligase type 4, blue] was used as MAM marker. (C) Pml+/+ MEFs subcellular fractionation and identification of PP2a and Akt at ER and MAM fractions by immunoblot. (D) Effects of okadaic acid (OA, 1 μM for 1 hour) and LY294002 (5 μM for 30 min) on agonist-dependent [Ca2+]m responses in Pml+/+, Pml−/−, and Pml−/− MEFs expressing erPML. [Ca2+]m is represented as a percentage of the peak value of control cells. Representative traces are shown in fig. S15. (E) Quantification of cell survival of Pml+/+, Pml−/−, and Pml−/− MEFs expressing erPML, control (CTR, untreated) and treated first with OA (1 μM for 1 hour) or LY294002 (5 μM for 30 min) and then H2O2 or menadione (MEN) for 16 hours. The data show the percentage of living cells in the whole-cell population negative for annexin-V–fluorescein isothiocyanate and propidium iodide staining, analyzed by flow cytometry. Data show the means SD from three independent experiments.

Reduced cellular sensitivity to apoptotic stimuli was observed in cells with high activity of the protein kinase Akt, as a result of diminished Ca2+ flux from the ER through the IP3R (20, 21). The amount of phosphorylated Akt (pAkt) (that is, the active form of Akt) coprecipitated with IP3R3 (Fig. 4A and fig. S9) was higher in Pml−/− than in Pml+/+ MEFs (fig. S11). Dephosphorylation of Akt at the MAM might occur through Pml-mediated recruitment of the phosphatase PP2a. Indeed, Pml interacts with PP2a in Pml-NBs (22). Further, the amount of PP2a coprecipitated with IP3R3 (Fig. 4A and figs. S9 and S10) was diminished in Pml−/− MEFs (Fig. 4A and fig. S11). Thus, in the absence of Pml, reduced Ca2+ release could be caused by increased phosphorylation and activation of Akt at the ER due to an impaired PP2a activity, which in turn impair Ca2+ flux through the IP3R because of its hyperphosphorylated state (figs. S11 and S12).

To determine whether IP3R3, Pml, Akt, and PP2a interact in a complex, we next performed two-dimensional blue native analysis. We found that Pml, IP3R3, Akt, and PP2a colocalize in high molecular weight complexes, supporting their possible interaction in the native state (fig. S13). Finally, we demonstrated the localization of all these proteins at the ER and MAM through immunocytochemical staining and subfractionation (Fig. 4, B and C, and fig. S14).

We further investigated the correlation among Pml, Akt, and PP2a at the ER and the regulation of the IP3R by a selective inhibition of either Akt or PP2a. Pretreatment of cells with okadaic acid (OA, a PP2a inhibitor) caused a reduction in [Ca2+]m responses to ATP stimulation and a reduced H2O2- or MEN-induced death in Pml+/+ MEFs and in Pml−/− MEFs expressing erPML, but not in Pml−/− MEFs (Fig. 4, D and E, and figs. S15, S16, and S18), in which PP2a activity is impaired. LY294002 (an inhibitor of Akt) had no effect on the agonist-dependent [Ca2+]m transients and on apoptosis in Pml+/+ or Pml−/− MEFs expressing erPML, whereas it increased agonist-dependent [Ca2+]m responses and restored sensitivity to H2O2 or MEN (Fig. 4, D and E, and figs. S15, S17, and S18) in Pml−/− MEFs (in which high levels of pAkt are observed; Fig. 4A and fig. S11). These results were confirmed in experiments in which RNA interference was used to deplete cells of Akt or PP2a proteins (fig. S19, A and B) or a constitutively active form of Akt (m/p Akt) was expressed (fig. S19C).

Our data highlight an extranuclear, transcription-independent function of Pml that regulates cell survival through changes in Ca2+ signaling in the ER, cytosol, and mitochondria (fig. S20). This effect appears to be specific to Ca2+-mediated apoptotic stimuli because alteration in Pml did not influence cell death in cells treated with ETO, which activates the apoptotic pathway in a way largely independent of Ca2+.

This mechanism may explain how Pml can so broadly regulate the early (and transcription independent) apoptotic response. Our findings may have implications in tumorigenesis where the function of Pml is frequently lost, or in other pathophysiological conditions where Pml is accumulated such as cell stress, or infection with viral or bacterial pathogens.

Supporting Online Material

Materials and Methods

Figs. S1 to S20


References and Notes

  1. Materials and methods are available as supporting material on Science Online.
  2. This work was supported in part by grants from the National Cancer Institute (to P.P.P.); by K99 NIH (to I.K.); by AIRC, FISM, Telethon, Ministry of Health, and PRIN (to P.P.); by FP7 “MyoAGE”, NIH, Cariparo Foundation, and AIRC (to R.R.); and by grants from the Ministry of Science and Higher Education in Poland and the Polish Mitochondrial Network (to M.L., J.D., and M.R.W.). We thank S. Missiroli, F. Poletti, and C. Agnoletto for carrying out some experiments, and J. Meldolesi and members of the Pandolfi and Pinton lab for stimulating discussions.
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