Supplemental Material can be found at: http://www.jbc.org/cgi/content/full/M702951200/DC1 THE JOURNAL OF BIOLOGICAL CHEMISTRY VOL. 282, NO. 38, pp. 28285–28295, September 21, 2007 © 2007 by The American Society for Biochemistry and Molecular Biology, Inc. Printed in the U.S.A.
HtrA2 Regulates -Amyloid Precursor Protein (APP) Metabolism through Endoplasmic Reticulum-associated Degradation*□ S
Received for publication, April 6, 2007, and in revised form, July 31, 2007 Published, JBC Papers in Press, August 6, 2007, DOI 10.1074/jbc.M702951200
Alzheimer disease-associated -amyloid peptide is generated from its precursor protein APP. By using the yeast two-hybrid assay, here we identified HtrA2/Omi, a stress-responsive chaperone-protease as a protein binding to the N-terminal cysteinerich region of APP. HtrA2 coimmunoprecipitates exclusively with immature APP from cell lysates as well as mouse brain extracts and degrades APP in vitro. A subpopulation of HtrA2 localizes to the cytosolic side of the endoplasmic reticulum (ER) membrane where it contributes to ER-associated degradation of APP together with the proteasome. Inhibition of the proteasome results in accumulation of retrotranslocated forms of APP and increased association of APP with HtrA2 and Derlin-1 in microsomal membranes. In cells lacking HtrA2, APP holoprotein is stabilized and accumulates in the early secretory pathway correlating with elevated levels of APP C-terminal fragments and increased A secretion. Inhibition of ER-associated degradation (either HtrA2 or proteasome) promotes binding of APP to the COPII protein Sec23 suggesting enhanced trafficking of APP out of the ER. Based on these results we suggest a novel function for HtrA2 as a regulator of APP metabolism through ER-associated degradation.
A major neuropathological hallmark of Alzheimer disease (AD)3 is the accumulation of amyloid -peptide (A) in senile plaques (1). A is generated from -amyloid precursor protein (APP) by sequential proteolytic cleavages mediated by - and ␥-secretases (2). An alternative nonamyloidogenic ␣-secretase cleavage cuts APP in the middle of the A region (3). APP is a ubiquitous type I transmembrane glycoprotein with many
* This work was supported in part by grants from the NINDS, National Institutes of Health (to D. M. K.) and the Helsingin Sanomat Centennial Foundation and Maud Kuistila Memorial Foundation (to H. J. H.). The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked “advertisement” in accordance with 18 U.S.C. Section 1734 solely to indicate this fact. □ S The on-line version of this article (available at http://www.jbc.org) contains supplemental Figs. S1–S3. 1 These authors contributed equally to this work. 2 To whom correspondence should be addressed: Neurobiology of Disease Laboratory, Massachusetts General Hospital, Harvard Medical School, 114 16th St., Charlestown, MA 02129. Tel.: 617-726-3668; Fax: 617-724-1823; E-mail:
[email protected]. 3 The abbreviations used are: AD, Alzheimer Disease; ER, endoplasmic reticulum; APP, -amyloid precursor protein; A, amyloid -peptide; PBS, phosphate-buffered saline; PDI, protein-disulfide isomerase; ERAD, ER-associated degradation; KPI, Kunitz-type protease inhibitor.
SEPTEMBER 21, 2007 • VOLUME 282 • NUMBER 38
putative functions related to cell adhesion and migration. Like most plasma membrane proteins, APP is synthesized and N-glycosylated in the endoplasmic reticulum (ER) and transported to the Golgi complex for maturation before transport to the cell surface. Several molecular chaperones that interact with APP have been identified including BiP/GRP78 (4) and calreticulin (5). Genetic evidence shows that duplication of the APP gene locus is sufficient to cause early-onset AD (6). APP gene dosage is doubled in Down syndrome (DS), and all adults over the age of 40 years develop AD (7). Furthermore, analysis of the human genome suggests that copy number variations play a significant role in the etiology of complex diseases such as AD (8) highlighting the importance of cellular regulatory mechanisms. Although proteolytic events resulting in the generation of A from APP are well characterized, the regulation of APP protein levels in cells remains poorly understood. Altered maturation, processing, and degradation of APP holoprotein may regulate the availability of APP for A generation or affect the ratio of A42 to A40, both of which appear to be important in the pathogenesis of AD. Several recent reports have suggested that events in the early secretory pathway strongly affect APP metabolism and A generation (9 –11). HtrA2, a novel APP-interacting chaperone protease, was recently reported to cleave APP in the mitochondria (12). HtrA proteins are oligomeric, ATP-independent serine proteases widely found from bacteria to mammals with important roles in protein quality control (13). In general, HtrA proteins contain a protease domain and one or two regulatory PDZ domains that recognize partially folded or misfolded proteins. Of the four human HtrA family members HtrA2 is the only one with an intracellular localization (13), and there is strong evidence showing that HtrA2 plays a role in the regulation of apoptosis (14 –16). However, the neurodegenerative phenotype of the HtrA2 knock-out mice and increased susceptibility of HtrA2⫺/⫺ cells to ER stress suggest that HtrA2 might play an important role in protein quality control (17). HtrA2 has been shown to bind through its PDZ domain to both A (18) and the C termini of the presenilins (PS1 and PS2), key components of the ␥-secretase complex (19). Our current results suggest that HtrA2 has a more general role in the regulation of APP metabolism. Partial localization of HtrA2 to the cytosolic side of ER membranes together with the finding that HtrA2 exclusively binds to the immature form of JOURNAL OF BIOLOGICAL CHEMISTRY
28285
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
Henri J. Huttunen‡§1, Suzanne Y. Gue´nette§1, Camilla Peach‡§, Christopher Greco‡§, Weiming Xia¶, Doo Yeon Kim‡§, Cory Barren‡§, Rudolph E. Tanzi§, and Dora M. Kovacs‡§2 From the ‡Neurobiology of Disease Laboratory and the §Genetics and Aging Research Unit, Massachusetts General Institute for Neurodegenerative Disease (MIND), Massachusetts General Hospital, Harvard Medical School, Charlestown, Massachusetts 02129 and the ¶Center for Neurologic Diseases, Brigham and Women’s Hospital and Harvard Medical School, Boston, Massachusetts 02115
HtrA2 Regulates APP Metabolism through ERAD APP indicate that the HtrA2-APP interaction occurs in the early secretory pathway. Lack of HtrA2 in cells results in stabilization of APP holoprotein, its accumulation in microsomes as well as increased association of immature APP with the COPII protein Sec23. Furthermore, we show that APP is retrotranslocated from the ER to the cytosol and is a substrate for the ERassociated degradation (ERAD) pathway. Based on these data, we propose that HtrA2 collaborates with the proteasome in ERAD to regulate cellular levels of APP.
28286 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 38 • SEPTEMBER 21, 2007
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
EXPERIMENTAL PROCEDURES Yeast Two-hybrid Assay—Identification of APP N-terminal domain-binding proteins was performed as described previously for the APP cytoplasmic domain (20). Briefly, the N-terminal cysteine-rich region (38 –187 amino acids) of human APP was cloned in-frame in the LexA plasmid. The yeast strain EGY48 that contained LexAop-LEU2, LexAop-LacZ, and LexA-APP (38 –187) was transformed with DNA from a galactose-inducible activation domain-cDNA fusion library constructed from 22-week-old human fetal brain (a gift from Dimitri Krainc, Massachusetts General Hospital, Boston). We identified and confirmed 63 independent positives from this screen. Southern blot analysis of the cDNA inserts showed that 61 of these clones were highly conserved sequences from six classes of overlapping cDNA clones. A full-length 458 amino acid open reading frame for the newly identified human gene was assembled from the two hybrid library clone containing the longest cDNA insert, a human adult brain lambda ZAP cDNA library (B616), a human kidney lambda phage cDNA library (ClonTech) and a human cosmid library (a gift from Marcy Macdonald, Massachusetts General Hospital, Boston). Cell Culture and Transfection—Parental CHO, H4, CHOAPP751, H4APP751, and mouse embryonic fibroblasts (MEF; wild-type or HtrA2⫺/⫺ (17)) were grown in Dulbecco’s modified Eagle’s medium supplemented with 10% (v/v) fetal bovine serum (Atlanta Biologicals), 2 mM L-glutamine (Lonza), 100 units/ml penicillin, and 100 g/ml streptomycin (Lonza). Stable cell lines were selected and maintained in G418 (Calbiochem). Cells were cultured at 37 °C in a water-saturated air/5% CO2 atmosphere. MEF cells were transiently transfected using the Amaxa Nucleofector system according to the manufacturer’s instructions (Amaxa Biosystems). Antibodies, Peptides, and Recombinant Proteins—Recombinant human HtrA2 (rec-HtrA2), His-tagged recombinant BACE1 and HtrA2 antibody were from R&D Systems. The following APP antibodies were used: 22C11 (N-terminal; Chemicon), A8717 (C-terminal; Sigma), 6E10 (A 1–17, Signet) and NAB228 (A 1–11, Covance). C-66 is an affinity-purified rabbit polyclonal antibody raised to the C-terminal 20 amino acids of human APP (751–770) by the same protocol (BioSource) that was used for the widely used C7 antibody (21). Calreticulin and Smac/Diablo antibodies were from Calbiochem, V5 from Invitrogen, His from Amersham Biosciences, BiP/GRP78 from Affinity BioReagents, GAPDH from Chemicon, protein-disulfide isomerase (PDI) and ubiquitin from Stressgen, Sec23 from Bethyl Laboratories, Derlin-1 from Novus Biologicals, GM130, EEA-1, cytochrome c, and syntaxin-6 from BD Biosciences. To construct C-terminally V5/His-tagged proteins,
APP751, APP695, and nectin-1 cDNAs were subcloned into the pcDNA3.1-V5/His vector (Invitrogen). These constructs were stably transfected to CHO cells and V5/His-tagged proteins purified from detergent lysates using nickel-nitrilotriacetic acid (Ni-NTA)-agarose columns (Qiagen). Immunoprecipitation, Western, and Lectin Blotting—Cells were extracted on ice in a Triton-Nonidet P-40 buffer containing 10 mM Tris-HCl, pH 6.8, 1 mM EDTA, 150 mM NaCl, 0.25% Nonidet P-40, 1% Triton X-100, and a protease inhibitor mixture (Roche Applied Science). Nuclei and unbroken cells were removed by centrifugation at 16,000 ⫻ g. The protein concentrations were determined using the BCA protein assay kit (Pierce). For Western blots, 20 –75 g of total protein was resolved in 4 –12% gradient Bis-Tris gels (Novex/Invitrogen) under reducing conditions. For immunoprecipitation, 250 – 1000 g of total protein was diluted to 1 mg/ml with extraction buffer and precleared with protein A or protein G-conjugated agarose beads (Pierce). The precleared samples were incubated overnight with excess amount of specific antibodies or nonimmune IgG (Jackson Laboratories). Immunocomplexes were captured with Protein A/G agarose beads, washed five times with the extraction buffer and heated for 10 min at 70 °C in 1⫻ LDS gel-loading buffer (Invitrogen) containing -mercaptoethanol. When needed, 20 M UCF-101 (an HtrA2 inhibitor, Calbiochem) was included in the immunoprecipitation mixes. Band intensities on Western blot images were quantitated by using Quantity One software (Bio-Rad) and normalized as indicated in figure legends. Subcellular Fractionation—Cells were harvested in ice-cold 10 mM Hepes, pH 7.4, 0.25 M sucrose, 1 mM EDTA, and homogenized using a metal Dounce homogenizer. Postnuclear supernatants (1,000 ⫻ g, S1) were centrifuged at 3,000 ⫻ g for 10 min (heavy mitochondria, P2), 12,000 ⫻ g for 10 min (light mitochondria, P3) and 100,000 ⫻ g for 45 min (microsomes, P4). Each pellet was washed once before proceeding to the next step. A portion of resuspended microsomal pellet (P4) was washed with 100 mM Na2CO3, pH 11.5 for 30 min on ice and centrifuged for 45 min at 100,000 ⫻ g. The pellet (P5) was the carbonate washed microsomal membrane fraction whereas the supernatant (S5) consisted mostly of proteins peripherally associated with microsomal membranes. Post-mitochondrial supernatants of CHOAPP751 or parental CHO cells were fractionated on a 7.5–30% continuous iodixanol gradients (OptiPrep; Axis-Shield) as described previously (22). Lipid rafts were isolated as described previously (23) using 0.5% Lubrol WX (Lubrol 17A17; Serva) as a detergent. Because of variation in distribution of proteins between the two lipid raft fractions within a given gradient, combined APP signal from fractions 3 and 4 was normalized to the sum of flotillin-1 signal from the same fractions. Confocal Fluorescence Microscopy—CHO cells were grown on coverslips coated with poly-D-lysine/laminin mixture. The cells were fixed with 3% paraformaldehyde/PBS, permeabilized with 0.1% Triton X-100/PBS for 10 min and blocked first with 10 mM NH4Cl/PBS and then with 2% BSA/PBS. Endogenous HtrA2, PDI, syntaxin-6, and APP (rabbit C-terminal (Chemicon) or 6E10 mAb (Signet)) were detected with corresponding antibodies and Alexa Fluor-conjugated secondary antibodies
HtrA2 Regulates APP Metabolism through ERAD
SEPTEMBER 21, 2007 • VOLUME 282 • NUMBER 38
FIGURE 1. HtrA2/Omi interacts with the ectodomain of immature APP. A, schematic diagram of APP751 domains and the yeast two-hybrid construct used in this study. The yeast two-hybrid construct was generated by fusing the cysteine-rich region of APP-(38 –187) to LexA. SP, signal peptide; KPI, Kunitz-type protease inhibitor; TM, transmembrane; IC, intracellular domain. B, detergent extracts of CHO (750 g) and CHOAPP751 (250 g) cells were immunoprecipitated with HtrA2 or C-terminal APP antibodies. Nonimmune rabbit IgG and plain protein G beads were used as specificity controls. A representative Western blot of triplicate immunoprecipitations is shown for both cell lines. C, reciprocal coimmunoprecipitation of detergent-extracted mouse brain hemispheres with HtrA2 or APP C-terminal antibodies.
Statistical Methods—Statistical comparisons were done using unpaired t tests or analysis of variance with significance placed at p ⬍ 0.05. Data are expressed as mean ⫾ S.D.
RESULTS HtrA2 Binds and Degrades Immature APP—To identify proteins that interact with the cysteine-rich, N-terminal domain of APP, we performed a yeast two-hybrid assay with the APP cysteine-rich domain as a bait sequence (depicted in Fig. 1A). The smallest APP-interacting cDNA contained 162 C-terminal amino acids of HtrA2/Omi chaperone-protease including the active site motif, GNSGG, and the PDZ domain (data not shown). Furthermore, the HtrA2 two-hybrid fusion proteins failed to induce lacZ expression when the APLP2 cysteine-rich region (56 –203 amino acids) was used in the yeast two-hybrid assay, indicating that HtrA2 binding is specific for the APP Cys-rich region. Next, we performed reciprocal immunoprecipitations with HtrA2 and APP antibodies to verify the yeast two-hybrid findings. As shown in Fig. 1B, only immature form of APP interacts JOURNAL OF BIOLOGICAL CHEMISTRY
28287
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
(Molecular Probes/Invitrogen). Mitochondria were stained MitoTracker Red and nuclei with Hoechst 33342 (Molecular Probes/Invitrogen). Confocal fluorescence images were obtained using a Olympus DSU/IX70 spinning disc confocal microscope and processed using IPLab software (Scanalytics/BD Biosciences). In Vitro Cleavage Assay—Rec-HtrA2 was incubated with purified recombinant APP751, APP695, nectin-1 or BACE1 in a reaction buffer containing 50 mM Tris-HCl, pH 7.0, 0.5 mM EDTA, 1 mM dithiothreitol. Depending on the assay, duration and temperature of incubation varied between 15 and 90 min and 37– 42 °C. Reaction was stopped by adding 1⫻ LDS gelloading buffer (Invitrogen) and heating for 10 min at 70 °C. Occasionally, the 15 amino acid peptide corresponding to the presenilin-1 C terminus was included in the reaction mixture at 10 –100 M (19). Alternatively, microsomal membranes rehomogenized in 10 mM Hepes, pH 7.4, 0.25 M sucrose, 1 mM EDTA with or without 1% Triton X-100 were used as substrate material. Retrotranslocation Assay—Retrotranslocation of proteins to the cytosol was analyzed as described previously (24). Briefly, cells in monolayer were detached from tissue culture plates with PBS containing 5 mM EDTA. After centrifugation at 1,000 ⫻ g for 5 min, the cell pellet was resuspended in 100 l of DPB buffer (0.04% digitonin (Sigma), 50 mM Hepes, pH 7.5, 150 mM NaCl, 2 mM CaCl2, protease inhibitor mixture (Roche Applied Sciences)), incubated on ice for 10 min and centrifuged at 16,000 ⫻ g for 10 min at 4 °C. The supernatant was removed (cytosol), and the membrane pellet was washed with 500 l of cold PBS and extracted in 150 l of DEB buffer (1% digitonin, 25 mM Tris-HCl, pH 7.4, 150 mM NaCl, 5 mM MgCl2, 1 mM phenylmethylsulfonyl fluoride, protease inhibitor mixture). Alternatively, the membrane pellet was homogenized in 10 mM Hepes, pH 7.4, 0.25 M sucrose, 1 mM EDTA with a glass-teflon homogenizer. Postnuclear supernatant was centrifuged at 16,000 ⫻ g and carbonate washed as described above for microsomes. Where indicated, cells were treated with 1 M epoxomicin (Biomol) for 5 h. Pulse Chase—Nearly confluent cells grown on 100-mm plates were first preincubated in methionine/cysteine-free medium for 1 h. 100 Ci of [35S]methionine/cysteine (MP Biomedicals) was then added per plate for 15 min (pulse). Then, cells were incubated in the presence of excess amounts of cold methionine/cysteine (MP Biomedicals) and harvested at 20-min intervals (chase). The cells were then washed, lysed in Triton-Nonidet P-40 buffer, and APP was immunoprecipitated (A8717 antibody, Sigma). Fixed and dried gels were exposed to a phosphorimaging screen (Bio-Rad). Images were read and quantitated using a Personal Molecular Imager FX and Quantity One software (Bio-Rad). A ELISA—For A determination, conditioned media was collected and cleared from debris. Secreted A was immunoprecipitated with excess 6E10 antibody and quantitated by standard sandwich ELISA (A ELISA Core Facility, Center for Neurological Diseases, Harvard Institutes of Medicine, Harvard Medical School).
HtrA2 Regulates APP Metabolism through ERAD
28288 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 38 • SEPTEMBER 21, 2007
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
nM HtrA2 produced N-terminally truncated versions optimally at pH 7.0 (open arrowheads in Fig. 2B). While this report was in preparation, Park et al. (12) identified an HtrA2 cleavage site in the APP ectodomain (at Val590/Asn591 according to APP751 numbering) generating a major cleavage product APP-C161. Accordingly, we found a prominent APP C-terminal fragment of ⬃25–27 kDa (V5/His-tag increases molecular weight) generated maximally at neutral pH that likely is APP-C161 (closed arrowhead in Fig. 2B). The 751-amino acid splicing variant of APP contains a Kunitz-type protease inhibitor (KPI) domain whose function is poorly understood (28). Given that the 56-amino acid KPI is located close to the cysteine-rich region, we next incubated FIGURE 2. Proteolytic cleavage of APP by HtrA2. Purified recombinant APP751-V5/His (A–C), APP695-V5/His both APP 751 (containing the KPI (C), nectin-1-V5/His (D), or BACE1-His (D) was incubated with rec-HtrA2 in different conditions: (A) increasing domain) and APP695 (lacking the concentrations of HtrA2 at 42 °C (15 or 45 min), (B) 132 nM HtrA2 at 37 °C (60 min) in a series of increasing buffer pH, (C) APP751-V5/His or APP695-V5/His were incubated with HtrA2 at 37 °C, pH 7.0 (60 min). D, 0.5 g of KPI domain) with HtrA2 at 37 °C. nectin-1-V5/His or BACE1-His were incubated with increasing concentrations of HtrA2 at 37 °C (60 min). Western blots were stained with APP C-terminal antibodies, V5 or His antibodies and subjected to densitometric After a 45-min incubation with 500 analysis. The results are displayed as percentage of remaining APP holoprotein compared with the control nM HtrA2, roughly 15% of both samples containing no HtrA2. APP751 and APP695 had been degraded by HtrA2 (Fig. 2C). Howwith HtrA2 in naı¨ve and APP751-overexpressing CHO cells. A ever, the resulting 25-kDa C-terminal fragment (presumably similar interaction of HtrA2 with immature APP was found in APP-C161) was present in the APP751 but not in APP695 samboth parental H4 human neuroglioma cells and H4 cells over- ples suggesting that the presence of the KPI domain somehow expressing APP751 (data not shown). To confirm that the HtrA2 affects the degree of completion to which HtrA2 degrades APP. interaction with APP occurs in vivo we immunoprecipitated Recombinant V5/His-tagged nectin-1, a type 1 transmembrane HtrA2 and APP from mouse brain extracts. Similar to our find- protein (29), and His-tagged ectodomain of BACE1 (30) were ings in cultured cells, the immature form of APP immunopre- used to control for specificity of HtrA2 proteolytic activity. As cipitated with HtrA2 from detergent extracts of mouse brains shown in Fig. 2D, HtrA2 was not able to cleave either nectin-1 (Fig. 1C). or BACE1 in these assay conditions suggesting that APP is a Although HtrA family proteases do not display strict cleav- specific substrate for the HtrA2 protease. age site requirements in general, optimal substrate cleavage In addition to APP, HtrA2 has been reported to interact with sites for HtrA2 have been reported (25). Sequence analysis of presenilin-1 (PS1) and presenilin-2 (PS2), both implicated in APP suggests that there are several potential HtrA2 cleavage Alzheimer disease. PS1 is a critical component of the ␥-secresites in the APP ectodomain (data not shown). To analyze deg- tase complex that generates A from APP (31) and the C terradation of APP by HtrA2 in vitro, we incubated purified minus of PS1 interacts with the regulatory PDZ domain of V5/His-tagged APP with rec-HtrA2. By homology to its bacte- HtrA2 activating the protease (19). Thus, we tested whether a rial relative DegS, HtrA2 is considered to be a heat-responsive 15-amino acid C-terminal peptide of PS1 could regulate HtrA2 protease whose proteolytic activity is regulated by the open/ proteolytic activity toward APP. In the presence of 100 M PS1 close conformation of its regulatory PDZ-domain (13, 26, 27). C-terminal peptide, HtrA2 activity is roughly doubled and only Therefore, we first tested whether APP is cleaved by increasing 31% of full-length APP remains in the reaction mixture as comconcentrations of HtrA2 at the activating temperature 42 °C. pared with 66% in the control reaction without the PS1 peptide As shown in Fig. 2A, increasing HtrA2 concentration resulted (supplemental Fig. S1). Altogether, the in vitro cleavage data in gradually increasing degradation of full-length APP. At 150 suggest that HtrA2 is capable of specifically degrading APP, and nM HtrA2 concentration, more than 90% of APP had been that the degree of APP degradation is controlled by conditions degraded by HtrA2 after 45 min at 42 °C. To optimize the con- that affect the regulatory PDZ domain of HtrA2 as well as the ditions for HtrA2-mediated in vitro cleavage of APP751-V5/His, presence of a protease inhibitor domain in the substrate. HtrA2 Localizes to Mitochondria, ER, and Cytosol—Original we determined the pH optimum for this proteolytic reaction. At 37 °C where HtrA2 displays partial proteolytic activity, 132 reports described mammalian HtrA2 as an ER- and nucleus-
HtrA2 Regulates APP Metabolism through ERAD
localized protease (32, 33). However, it has become evident that the majority of cellular HtrA2 is localized to mitochondria (14, 15). Because of these contradictory reports, we used both subcellular fractionation and confocal immunofluorescence imaging to study subcellular localization of HtrA2. Crude cell fractionation by differential centrifugation confirmed that the majority of HtrA2 was localized to the mitochondrial fractions. However, a significant amount of HtrA2 was also found in the microsomal fraction and a small amount in the cytosolic fraction under normal growth conditions (Fig. 3A). To analyze the microsomal fraction in detail, we resolved the postmitochondrial supernatant in an OptiPrep density gradient. Clearly, most of the extramitochondrial HtrA2 colocalized with the ER-chaperone BiP/GRP78 (Fig. 3B). Interestingly, an alkali carbonate extraction of both microsomal (Fig. 3A) and pooled ER fractions (data not shown) washed out most if not all HtrA2 but none of the integral membrane proteins (APP and calreticulin in fractions P5 and S5 in Fig. 3A) or ER lumenal proteins (GRP78/BiP, data not shown). This suggests that HtrA2 associates peripherally to the cytosolic side of the microsomal/ER vesicles. Confocal microscopy of CHO cells stained with HtrA2 antibodies together with MitoTracker Red, PDI or syntaxin-6 confirmed that HtrA2 mainly colocalized with the mitochondrial marker (Fig. 3C). However, less frequent but still significant colocalization of HtrA2 with the ER marker PDI was detected (Fig. 3D). No colocalization was observed with the Golgi SEPTEMBER 21, 2007 • VOLUME 282 • NUMBER 38
marker, syntaxin-6 (Fig. 3E). Costaining of HtrA2 and APP showed colocalization of the two proteins in ER-like structures (Fig. 3F). Given a couple of recent reports indicating mitochondrial localization of APP (12, 34), it should be noted that in these experiments we could not detect any colocalization of APP with mitochondrial markers in our cell lines (Fig. 3G). Taken together, our subcellular localization data suggest that HtrA2 interacts with immature APP in the early secretory pathway. APP Can Be Retrotranslocated and Degraded by the Proteasome and HtrA2—Several studies have implied that a degradation pathway associated with the ER participates in the regulation of APP metabolism (4, 35–37). Because of the localization of extramitochondrial HtrA2 to the cytosolic side of the ER/microsomal membranes, access of HtrA2 to its binding sites in the extracellular/lumenal domain of APP would require dislocation of APP from the ER to the cytosol. To assess whether APP is retrotranslocated from the ER, we used a retrotranslocation assay (24) to collect cytosols from semipermeabilized cells. Treatment of CHOAPP751 cells with epoxomicin, a selective and irreversible proteasome inhibitor (38), resulted in cytosolic accumulation of immature APP and a smaller, ⬃95-kDa form of APP (Fig. 4A). Neither form of APP was ubiquitinated suggesting that the cytosolic forms of APP are degraded by the proteasome in a ubiquitin-independent manner. Interestingly, the 95-kDa form of APP appeared to be N-terminally truncated as C-terminal (A8717, NAB228) but not N-terminal (22C11) APP antibodies recognized it in Western blots (Fig. 4B). JOURNAL OF BIOLOGICAL CHEMISTRY
28289
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
FIGURE 3. Extramitochondrial HtrA2 colocalizes with APP and ER markers in CHO cells. A, crude fractionation of CHOAPP751 cells by differential centrifugation. Heavy mitochondrial (P2), light mitochondria (P3), microsomal (P4), and cytosolic (S4) fractions were analyzed together with carbonate-washed microsomes. The fractions were separated on an SDS-PAGE gel and Western blots were probed with HtrA2, APP, and organelle marker antibodies. B, postmitochondrial supernatant of CHOAPP751 cells (fraction S3 from A) was fractionated on a 7.5–30% iodixanol gradient. CHO cells immunostained with HtrA2 antibodies (C–F) together with subcellular organelle markers MitoTracker (C), ER-marker PDI (D), trans-Golgi marker syntaxin-6 (E), and APP (F). In addition, immunostaining of APP together with MitoTracker is shown (G). Nuclei in all samples were counterstained with Hoechst 33342 (blue). Bar, 10 m.
HtrA2 Regulates APP Metabolism through ERAD
28290 JOURNAL OF BIOLOGICAL CHEMISTRY
VOLUME 282 • NUMBER 38 • SEPTEMBER 21, 2007
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
Derlin-1 is involved in retrotranslocation of APP. Together with the ability of HtrA2 to N-terminally trim APP in vitro (Fig. 2B), these data suggest that HtrA2 may serve as a shuttling factor delivering and preparing ERAD substrates for proteasomal degradation. Inhibition of the proteasome by epoxomicin caused a 29% increase in the microsome-associated HtrA2 (supplemental Fig. S2A). Interestingly, when microsomal membranes isolated from epoxomicintreated cells were incubated with rec-HtrA2, HtrA2 not only cleaved APP (data not shown) but also decreased the amount of total polyubiquitinated proteins by about 25% (supplemental Fig. S2B). This suggests that when proteasomal activity is compromised, HtrA2 may be recruited to the ER membrane to assist in the disposal of accumulating proteasome substrates. APP Metabolism Is Altered in FIGURE 4. Proteasome inhibition induces accumulation of a cytosolic APP fragment. A, CHOAPP751 cells were treated with 1 M epoxomicin or vehicle (Me2SO) for 5 h and semipermeabilized with 0.04% digitonin. Cells Lacking HtrA2—To better Cytosols were harvested, and the rest of the cells extracted in 1% Triton X-100/0.25% Nonidet P-40 (membranes). Fractions were resolved in Western blots and stained with APP (A8718), ubiquitin, and marker anti- understand the physiological relabodies. B, total lysates from A were resolved in Western blots and stained with different APP antibodies tionship between HtrA2 and APP, (epitopes (APP751 numbering): 22C11 (66 – 81 amino acids), A8717 (732–751 amino acids), and NAB228 (653– we next analyzed metabolism of 663 amino acids; A 1–11 amino acids)). C, B104 neuroblastoma cells were treated with 1 M epoxomicin or vehicle (Me2SO) for 16 h, and cytosols were harvested as in Fig. 4A. Membranes were homogenized without endogenous APP in fibroblasts detergent and washed with alkaline carbonate buffer. Western blots were stained with APP and transferrin derived from HtrA2⫺/⫺ mouse receptor antibodies. D, cytosols from A were incubated with rec-HtrA2 (0 or 2.0 M) for 90 min at 37 °C. E, detergent-extracted microsomal membranes from vehicle- and epoxomicin-treated cells were immu- embryos (17). As compared with noprecipitated with HtrA2 or APP C-terminal antibodies. Western blots were stained with APP, HtrA2, and fibroblasts derived from wild-type Derlin-1 antibodies. embryos, HtrA2⫺/⫺ cells had only slightly elevated total levels of APP To rule out the possibility that only overexpressed APP is holoprotein (by ⬃10%; Fig. 5A). However, the APP C-terminal retrotranslocated, we used naı¨ve B104 neuroblastoma cells in fragment levels were more significantly increased in HtrA2⫺/⫺ the retrotranslocation assay. Although free cytosolic, endoge- cells. After normalization to APP holoprotein levels, HtrA2⫺/⫺ nous APP forms could not be detected in epoxomicin-treated cells harbored 218% higher levels of APP-C99 and 171% higher B104 cells, we noticed an abundant pool of peripherally associ- levels of APP-C83 than the HtrA2⫹/⫹ cells (Fig. 5, A and B). The ated APP molecules that could be detached from microsomal elevated APP-C99 level correlated with a 41% increase in the membranes with an alkali carbonate buffer (Fig. 4C). These amount of A in the conditioned media from HtrA2⫺/⫺ cells as data show that endogenous APP can be retrotranslocated from compared with wild-type cells (Fig. 5C). the ER but remains associated with the cytosolic side of ER As HtrA1, a secreted HtrA-family member, was previously membranes. suggested to be an APP-CTF degrading protease (39) and Next, we tested whether HtrA2 could degrade the retrotrans- HtrA2 has been shown to bind to A and APP-C99 (18), we located, cytosolic APP. When cytosols collected from epoxomi- tested whether HtrA2 could also be an APP-CTF degrading cin-treated CHOAPP751 cells were incubated with rec-HtrA2, protease. However, HtrA2 was unable to directly degrade APPAPP was efficiently degraded (Fig. 4D). This suggests that C99 in vitro (supplemental Fig. S3) suggesting that even though HtrA2 may collaborate with the proteasome to degrade retro- both HtrA2 and HtrA1 are capable of binding APP they may translocated APP. Remarkably, when microsomal membranes exhibit different cleavage site specificities. Therefore, the isolated from epoxomicin-treated cells were immunopre- increased levels of APP-CTFs in HtrA2⫺/⫺ cells are more likely cipitated with HtrA2, a dramatic increase in the association explained by reduced degradation of APP holoprotein rather of both immature and 95-kDa forms of APP with HtrA2 was than altered degradation of the C-terminal fragments. To furobserved (Fig. 4E). Microsomal APP-immunoprecipitates from ther investigate this, we performed pulse-chase assays with epoxomicin-treated cells also contained more retrotransloca- [35S]methionine/cysteine in wild-type and HtrA2⫺/⫺ fibrotion protein Derlin-1 than the controls (Fig. 4E) suggesting that blasts. As shown in Fig. 5, D and E, the lack of HtrA2 increases
HtrA2 Regulates APP Metabolism through ERAD
SEPTEMBER 21, 2007 • VOLUME 282 • NUMBER 38
JOURNAL OF BIOLOGICAL CHEMISTRY
28291
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
APP holoprotein levels were significantly increased in microsomes prepared from HtrA2⫺/⫺ cells (Fig. 6A). We could not detect accumulation of immature or 95-kDa APP forms in the cytosols prepared from HtrA2⫺/⫺ or HtrA2⫹/⫹ cells in the retrotranslocation assay. However, similarly to B104 cells, microsomes prepared from HtrA2⫺/⫺ cells contained a pool of peripherally associated APP molecules that was detached from microsomal membranes with an alkali carbonate buffer (Fig. 6A). A transmembrane ER chaperone calreticulin did not dissociate from the microsomes, whereas a significant fraction of Sec23, a peripherally associated COPII transport protein, shifted to the wash fraction. Importantly, the carbonate wash had little effect on microsomal APP in HtrA2⫹/⫹ cells showing that retrotranslocated APP accumulates in HtrA2⫺/⫺ cells and remains peripherally associated with the microsomal membranes. Thus, lack of HtrA2 in fibroblasts results in accumulation of immature APP in the early secretory pathway further suggesting that HtrA2 FIGURE 5. Proteolytic processing of APP is altered in HtrA2ⴚ/ⴚ cells. A, expression levels of endogenous ⫺/⫺ HtrA2 and various APP forms in mouse embryonic fibroblasts (MEF) derived from HtrA2 and wild-type plays a role in ERAD of APP. Recently, Kincaid et al. (40) (HtrA2⫹/⫹) embryos. B, APP C-terminal fragments were quantitated from Western blots, normalized to GAPDH and then to the immature APP holoprotein. C, total secreted A quantitated from the conditioned media by A showed that ERAD and ER exit ⫺/⫺ ELISA and normalized to total protein content of the cell extracts. D, wild-type and HtrA2 MEFs were metabolically labeled with [35S]Met/Cys for 15 min and chased in the presence of excess amounts of cold pathways compete for substrates methionine/cysteine for 0, 20, 40, 60, and 80 min. Total protein lysates (500 g) were immunoprecipitated with that have ER exit signals. Therefore, an APP C-terminal antibody (A8717) and exposed to a phosphorimaging screen. E, quantitation of replicate lowered ERAD capacity may result pulse-chase experiments. Half-lives of immature and mature APP were calculated by logarithmic fitting of background-corrected band intensities at different time points. F, wild-type and HtrA2⫺/⫺ MEFs were tran- in increased ER exit of (misfolded) siently transfected with FLAG-tagged mouse HtrA2 or empty vector. APP processing was analyzed 24 h later. secretory proteins such as APP. G, APP C-terminal fragments were quantitated from Western blots, normalized to GAPDH and then to the Altered ER exit dynamics could be immature APP holoprotein. *, p ⬍ 0.05; **, p ⬍ 0.01; ***, p ⬍ 0.001. indicated by differential binding of APP to COPII cargo selection comthe half-life of APP holoprotein by ⬃175% (from 27.1 ⫾ 2.7 to plex Sec23/Sec24 (41, 42). Supporting this idea, immunopre47.5 ⫾ 2.3 min for immature APP and from 27.3 ⫾ 5.0 to 47.4 ⫾ cipitation of Sec23 pulled down a significantly higher amount 0.9 min for mature APP). of immature APP from HtrA2⫺/⫺ cells as compared with the Next, we tested if retransfection of HtrA2 back to the wild-type cells (Fig. 6B). Similarly, epoxomicin treatment of HtrA2⫺/⫺ cells could reverse the alterations in APP metabo- H4 cells resulted in increased binding of immature APP to lism. FLAG-tagged mouse HtrA2 was transfected by electropo- Sec23 (Fig. 6C) suggesting that suppression of HtrA2 or proration into the wild-type and HtrA2⫺/⫺ fibroblasts. In wild- teasome activities have similar accelerating effects on ER exit type MEFs, overexpression of HtrA2 had no significant effect of APP molecules. on the levels of APP holoprotein or APP-CTFs whereas trans- and ␥-secretase activities are known to be concentrated in fection of mHtrA2/FLAG into the HtrA2⫺/⫺ MEFs signifi- lipid rafts, cholesterol-enriched membrane microdomains cantly reduced APP-CTF levels (Fig. 5F). Mature APP holopro- implicated in protein trafficking, proteolytic processing, and tein was also reduced but to a lesser extent. Quantitation of signal transduction (23, 43). As most of the secreted A is repeated rescue experiments showed that the APP-CTF: thought to be generated in lipid rafts in post-Golgi compartAPP-FL ratio returned to wild-type levels in transfected ments, we tested whether APP association with lipid rafts is HtrA2⫺/⫺ cells (Fig. 5G) confirming that HtrA2 proteolytic altered in HtrA2⫺/⫺ cells. As shown in Fig. 6D, more APP holoactivity is directly coupled to metabolism of endogenous APP. protein is associated with flotillin-positive lipid raft fractions
HtrA2 Regulates APP Metabolism through ERAD
(fractions 3 and 4) HtrA2⫺/⫺ cells. Quantitation of replicate experiments revealed a significant 1.7-fold increase in lipid raftassociated APP holoprotein in HtrA2⫺/⫺ cells as compared with the wild-type cells (Fig. 6E). Thus, elevated APP-CTF and A levels in HtrA2⫺/⫺ cells may be explained by increased availability of APP holoprotein for amyloidogenic processing due to facilitated trafficking of newly synthesized APP out of the ER.
DISCUSSION Mammalian cells have evolved sophisticated mechanisms for recognition, retrotranslocation, and degradation of misfolded or unassembled ER and secretory proteins (44, 45). Several studies have suggested that a degradation pathway associated with ER participates in the regulation of APP metabolism (4, 35–37). Early events in the maturation of amyloid precursor protein (APP) seem to determine its entry into one of several alternative processing pathways, one involving proteasomal degradation in the cytosol. We have characterized an interaction between the stress-responsive chaperone protease HtrA2 and APP in the early secretory pathway. The present results are summarized in Fig. 7 and suggest that ERAD plays a role in the regulation of APP metabolism, and that by increasing the amount of APP available for - and ␥-secretase cleavages defective or impaired ERAD pathways could contribute to pathogenesis of AD. A prerequisite for HtrA2-APP interaction is retrotranslocation of APP from the ER membrane. Several studies have shown that APP holoprotein is degraded by the proteasome under var-
28292 JOURNAL OF BIOLOGICAL CHEMISTRY
ious conditions: proteasomal degradation of APP is enhanced by interrupted N-glycosylation of APP (36) and overexpression of modifier of cell adhesion (MOCA, Dock3) (35) whereas overexpression of peroxisome proliferator-activated receptor-␥ (PPAR␥) induces accumulation of polyubiquitinated APP (46). On the other hand, induction of ER stress results in retention of APP in the early secretory pathway and decreases generation of A (47). Our results showing that (1) immature APP as well as an N-terminally truncated form of APP are retrotranslocated to the cytosol, and (2) both retrotranslocated forms of APP can be degraded by the proteasome and HtrA2, provide a mechanistic explanation for the previously reported findings and identify APP as a novel substrate for ERAD. Although we noticed retrotranslocated immature APP peripherally associated with microsomal membranes in HtrA2⫺/⫺ cells, we were unable to detect the N-terminally truncated form of APP suggesting that it may be generated by HtrA2 during the retrotranslocation process. This is supported by the in vitro cleavage data where HtrA2 truncated APP N-terminally. Most retrotranslocated ERAD substrates carry polyubiquitin chains that are trimmed by shuttling factors such as ataxin-3 to facilitate proteasomal degradation (48). As retrotranslocated APP appears to be degraded in a ubiquitin-independent manner, it is tempting to speculate that HtrA2 could serve as a shuttling chaperone between retrotranslocation machinery and proteasome using its proteolytic activity to trim the core protein of nonubiquitinated ERAD substrates before proteasomal degradation. The finding that cells lacking HtrA2 are more VOLUME 282 • NUMBER 38 • SEPTEMBER 21, 2007
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
FIGURE 6. APP metabolism in the early secretory pathway is altered in HtrA2ⴚ/ⴚ cells. A, APP levels in microsomes and cytosols of HtrA2⫺/⫺ and wild-type MEF cells. Microsomes were washed in an alkali carbonate buffer to wash out peripherally bound proteins. Calreticulin (transmembrane ER protein) and Sec23 (peripherally bound to ER membranes and vesicles) were used as loading controls. B, coimmunoprecipitation of APP with Sec23 from HtrA2⫹/⫹ and HtrA2⫺/⫺ MEF cells. C, coimmunoprecipitation of APP with Sec23 from vehicle- and epoxomicin-treated H4 cells. D, APP levels in lipid raft fractions in HtrA2⫺/⫺ and wild-type MEF cells. The presence of flotillin-1 identifies fractions 3 and 4 as lipid raft fractions. E, APP holoprotein was quantitated from Western blots (the sum of APP signal in fractions 3 and 4) and normalized to flotillin-1 (the sum of flotillin-1 signal in fractions 3 and 4). *, p ⬍ 0.05.
HtrA2 Regulates APP Metabolism through ERAD
SEPTEMBER 21, 2007 • VOLUME 282 • NUMBER 38
JOURNAL OF BIOLOGICAL CHEMISTRY
28293
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
cells further support our conclusion that the lack of HtrA2 increases A production (1) by stabilizing APP in the early secretory pathway, and (2) by promoting trafficking of APP to - and ␥-secretase-containing cellular compartments. In general, this kind of mechanism involving a fine balance between ERAD and ER exit may also partially explain some recent functional findings regarding ubiquilin (9), a cytosolic protein containing ubiquitin-like (UBL) and ubiquitin-associated (UBA) domains, that has a strong genetic linkage in late-onset AD (49). The current view of mostly mitochondrial localization of HtrA2 (13, 50) argues against HtrA2 being a part of the protein quality control/ degradation machinery of the ER. However, our localization studies by FIGURE 7. HtrA2 collaborates with the proteasome in degradation of APP in the early secretory pathway. both subcellular fractionation and A schematic model summarizing our hypothesis based on the findings of this study. A, in normal cells, most confocal microscopy are supported newly synthesized APP molecules fold correctly and are exported from the ER in COPII vesicles after correct by two previous studies (32, 33) and folding. Occasional misfolded APP molecules are retained in the ER, engaged with the ERAD machinery, and retrotranslocated to the cytosol for degradation by the proteasome and HtrA2. B, in HtrA2⫺/⫺ cells, shuttling of suggest that although the majority ERAD substrates from the retrotranslocation machinery to the proteasome is impaired, resulting in accumula- of HtrA2 is localized to the mitotion of retrotranslocated immature APP on the ER membrane. C, in cells treated with a proteasome inhibitor, chondrial intermembrane space, ERAD substrates are retrotranslocated and shuttled to proteasome but fail to be degraded and accumulate in the cytosol. More HtrA2 is recruited to the ER membrane to compensate for the lost ERAD capacity. Similar to there is a fraction of cellular HtrA2 HtrA2⫺/⫺ cells, reduced ERAD capacity results in increased flow of APP from the ER to Golgi as reflected by that associates peripherally with ER increased association of APP with Sec23. The size of the red arrows reflects the number of molecules passing membranes and colocalizes with through each pathway. APP. It should be noted that our susceptible to ER stress (17) strongly supports our current results do not exclude the possibility that in addition to the ER, results and may be partially explained by accumulation of HtrA2 could interact with APP when localized to mitochondria ERAD substrates in the ER. Inhibition of proteasomal function (12, 34). However, in our cell lines we could not detect APP in induced association of HtrA2 with APP as well as Derlin-1, a the mitochondria suggesting that this may be cell type dependputative retrotranslocation channel forming ER protein. This ent. We also noticed a residual amount of HtrA2 in the cytosol suggests that Derlin-1 is involved in retrotranslocation of APP of normal, nonapoptic cells under standard cell culture condiand that HtrA2 may get recruited to Derlin-1 containing retro- tions. It is possible that to prevent induction of apoptosis, translocation complexes to assist in ERAD. Interestingly, exog- HtrA2 is recruited from the cytosol to ER by HtrA2-interacting enously added HtrA2 is able to degrade ubiquitinated proteins proteins such as presenilins (19). Presenilins are abundant in in proteasome-inhibited microsomes suggesting a more gen- the ER and have been suggested to have ␥-secretase independeral role for HtrA2 in ERAD. ent functions in trafficking and unfolded protein response Recently, it was reported that ERAD competes with ER-exit (UPR) in the early secretory pathway (51–53). Thus, it is temptpathways for substrates that have ER exit signals (40). Thus, ing to speculate that presenilin C termini could regulate the inhibition of ERAD in cells may result in increased ER exit of association of HtrA2 with the ER membranes. This could also (misfolded) secretory proteins (as depicted in Fig. 7). Immature be relevant regarding the role of cytosolic HtrA2 in apoptosis, APP holoprotein is clearly stabilized in HtrA2⫺/⫺ cells, and this especially in light of the antiapoptotic roles attributed to presemay result in increased ER exit of APP. Accordingly, we found nilin C-terminal fragments (54). Interestingly, proteolytic increased binding of immature APP to Sec23, a COPII cargo- activity of HtrA2 can be regulated through phosphorylation at loading protein, in both HtrA2⫺/⫺ cells and proteasome inhib- S212 by Akt kinase, a member of a key antiapoptotic pathway, itor-treated cells supporting the idea of altered ER exit dynam- adding another layer of complexity to HtrA2 biology (55). Although there are no reported genetic associations of ics. This also suggests that increased generation of APP C-terminal fragments and A in HtrA2⫺/⫺ cells could be HtrA2 with AD, mice with targeted deletion of the HtrA2 gene explained by accelerated trafficking of APP out of ER. suffer from a loss of striatal neurons and display a neurodegenIncreased levels of lipid raft-associated APP in HtrA2⫺/⫺ erative phenotype with Parkinsonian features (17). A careful
HtrA2 Regulates APP Metabolism through ERAD
Acknowledgments—The MEF cells from HtrA2⫺/⫺ mice and the mouse HtrA2 cDNA were kind gifts from Dr. Julian Downward (Cancer Research UK, London) and Dr. Emad Alnemri (Thomas Jefferson University, Philadelphia), respectively. We thank Dr. Dennis Selkoe (Brigham and Women’s Hospital, Boston) for the CHOAPP-C99 cell line.
REFERENCES 1. 2. 3. 4. 5. 6.
7. 8.
9.
10. 11.
12. 13.
Selkoe, D. J. (2001) Physiol. Rev. 81, 741–766 Haass, C. (2004) EMBO J. 23, 483– 488 Kojro, E., and Fahrenholz, F. (2005) Subcell. Biochem. 38, 105–127 Yang, Y., Turner, R. S., and Gaut, J. R. (1998) J. Biol. Chem. 273, 25552–25555 Johnson, R. J., Xiao, G., Shanmugaratnam, J., and Fine, R. E. (2001) Neurobiol. Aging 22, 387–395 Rovelet-Lecrux, A., Hannequin, D., Raux, G., Le Meur, N., Laquerriere, A., Vital, A., Dumanchin, C., Feuillette, S., Brice, A., Vercelletto, M., Dubas, F., Frebourg, T., and Campion, D. (2006) Nat. Genet. 38, 24 –26 Lott, I. T., and Head, E. (2005) Neurobiol. Aging 26, 383–389 Redon, R., Ishikawa, S., Fitch, K. R., Feuk, L., Perry, G. H., Andrews, T. D., Fiegler, H., Shapero, M. H., Carson, A. R., Chen, W., Cho, E. K., Dallaire, S., Freeman, J. L., Gonzalez, J. R., Gratacos, M., Huang, J., Kalaitzopoulos, D., Komura, D., MacDonald, J. R., Marshall, C. R., Mei, R., Montgomery, L., Nishimura, K., Okamura, K., Shen, F., Somerville, M. J., Tchinda, J., Valsesia, A., Woodwark, C., Yang, F., Zhang, J., Zerjal, T., Zhang, J., Armengol, L., Conrad, D. F., Estivill, X., Tyler-Smith, C., Carter, N. P., Aburatani, H., Lee, C., Jones, K. W., Scherer, S. W., and Hurles, M. E. (2006) Nature 444, 444 – 454 Hiltunen, M., Lu, A., Thomas, A. V., Romano, D. M., Kim, M., Jones, P. B., Xie, Z., Kounnas, M. Z., Wagner, S. L., Berezovska, O., Hyman, B. T., Tesco, G., Bertram, L., and Tanzi, R. E. (2006) J. Biol. Chem. 281, 32240 –32253 Rechards, M., Xia, W., Oorschot, V., van Dijk, S., Annaert, W., Selkoe, D. J., and Klumperman, J. (2006) Traffic 7, 354 –364 Vetrivel, K. S., Gong, P., Bowen, J. W., Cheng, H., Chen, Y., Carter, M., Nguyen, P. D., Placanica, L., Wieland, F. T., Li, Y. M., Kounnas, M. Z., and Thinakaran, G. (2007) Mol. Neurodegener. 2, 4 Park, H. J., Kim, S. S., Seong, Y. M., Kim, K. H., Goo, H. G., Yoon, E. J., Min do, S., Kang, S., and Rhim, H. (2006) J. Biol. Chem. 281, 34277–34287 Clausen, T., Southan, C., and Ehrmann, M. (2002) Mol. Cell 10, 443– 455
28294 JOURNAL OF BIOLOGICAL CHEMISTRY
14. Suzuki, Y., Imai, Y., Nakayama, H., Takahashi, K., Takio, K., and Takahashi, R. (2001) Mol. Cell 8, 613– 621 15. Hegde, R., Srinivasula, S. M., Zhang, Z., Wassell, R., Mukattash, R., Cilenti, L., DuBois, G., Lazebnik, Y., Zervos, A. S., Fernandes-Alnemri, T., and Alnemri, E. S. (2002) J. Biol. Chem. 277, 432– 438 16. Yang, Q. H., Church-Hajduk, R., Ren, J., Newton, M. L., and Du, C. (2003) Genes Dev. 17, 1487–1496 17. Martins, L. M., Morrison, A., Klupsch, K., Fedele, V., Moisoi, N., Teismann, P., Abuin, A., Grau, E., Geppert, M., Livi, G. P., Creasy, C. L., Martin, A., Hargreaves, I., Heales, S. J., Okada, H., Brandner, S., Schulz, J. B., Mak, T., and Downward, J. (2004) Mol. Cell. Biol. 24, 9848 –9862 18. Park, H. J., Seong, Y. M., Choi, J. Y., Kang, S., and Rhim, H. (2004) Neurosci. Lett. 357, 63– 67 19. Gupta, S., Singh, R., Datta, P., Zhang, Z., Orr, C., Lu, Z., Dubois, G., Zervos, A. S., Meisler, M. H., Srinivasula, S. M., Fernandes-Alnemri, T., and Alnemri, E. S. (2004) J. Biol. Chem. 279, 45844 – 45854 20. Gue´nette, S. Y., Chen, J., Jondro, P. D., and Tanzi, R. E. (1996) Proc. Natl. Acad. Sci. U. S. A. 93, 10832–10837 21. Podlisny, M. B., Tolan, D. R., and Selkoe, D. J. (1991) Am. J. Pathol. 138, 1423–1435 22. Puglielli, L., Konopka, G., Pack-Chung, E., Ingano, L. A., Berezovska, O., Hyman, B. T., Chang, T. Y., Tanzi, R. E., and Kovacs, D. M. (2001) Nat. Cell Biol. 3, 905–912 23. Vetrivel, K. S., Cheng, H., Lin, W., Sakurai, T., Li, T., Nukina, N., Wong, P. C., Xu, H., and Thinakaran, G. (2004) J. Biol. Chem. 279, 44945– 44954 24. Forster, M. L., Sivick, K., Park, Y. N., Arvan, P., Lencer, W. I., and Tsai, B. (2006) J. Cell Biol. 173, 853– 859 25. Martins, L. M., Turk, B. E., Cowling, V., Borg, A., Jarrell, E. T., Cantley, L. C., and Downward, J. (2003) J. Biol. Chem. 278, 49417– 49427 26. Wilken, C., Kitzing, K., Kurzbauer, R., Ehrmann, M., and Clausen, T. (2004) Cell 117, 483– 494 27. Li, W., Srinivasula, S. M., Chai, J., Li, P., Wu, J. W., Zhang, Z., Alnemri, E. S., and Shi, Y. (2002) Nat. Struct. Biol. 9, 436 – 441 28. Tanzi, R. E., McClatchey, A. I., Lamperti, E. D., Villa-Komaroff, L., Gusella, J. F., and Neve, R. L. (1988) Nature 331, 528 –530 29. Kim, D. Y., Ingano, L. A., and Kovacs, D. M. (2002) J. Biol. Chem. 277, 49976 – 49981 30. Vassar, R., Bennett, B. D., Babu-Khan, S., Kahn, S., Mendiaz, E. A., Denis, P., Teplow, D. B., Ross, S., Amarante, P., Loeloff, R., Luo, Y., Fisher, S., Fuller, J., Edenson, S., Lile, J., Jarosinski, M. A., Biere, A. L., Curran, E., Burgess, T., Louis, J. C., Collins, F., Treanor, J., Rogers, G., and Citron, M. (1999) Science 286, 735–741 31. De Strooper, B. (2003) Neuron 38, 9 –12 32. Faccio, L., Fusco, C., Chen, A., Martinotti, S., Bonventre, J. V., and Zervos, A. S. (2000) J. Biol. Chem. 275, 2581–2588 33. Gray, C. W., Ward, R. V., Karran, E., Turconi, S., Rowles, A., Viglienghi, D., Southan, C., Barton, A., Fantom, K. G., West, A., Savopoulos, J., Hassan, N. J., Clinkenbeard, H., Hanning, C., Amegadzie, B., Davis, J. B., Dingwall, C., Livi, G. P., and Creasy, C. L. (2000) Eur. J. Biochem. 267, 5699 –5710 34. Anandatheerthavarada, H. K., Biswas, G., Robin, M. A., and Avadhani, N. G. (2003) J. Cell Biol. 161, 41–54 35. Chen, Q., Kimura, H., and Schubert, D. (2002) J. Cell Biol. 158, 79 – 89 36. Hare, J. F. (2006) Arch. Biochem. Biophys. 451, 79 –90 37. Bunnell, W. L., Pham, H. V., and Glabe, C. G. (1998) J. Biol. Chem. 273, 31947–31955 38. Meng, L., Mohan, R., Kwok, B. H., Elofsson, M., Sin, N., and Crews, C. M. (1999) Proc. Natl. Acad. Sci. U. S. A. 96, 10403–10408 39. Grau, S., Baldi, A., Bussani, R., Tian, X., Stefanescu, R., Przybylski, M., Richards, P., Jones, S. A., Shridhar, V., Clausen, T., and Ehrmann, M. (2005) Proc. Natl. Acad. Sci. U. S. A. 102, 6021– 6026 40. Kincaid, M. M., and Cooper, A. A. (2007) Mol. Biol. Cell 18, 455– 463 41. Wang, X., Matteson, J., An, Y., Moyer, B., Yoo, J. S., Bannykh, S., Wilson, I. A., Riordan, J. R., and Balch, W. E. (2004) J. Cell Biol. 167, 65–74 42. Kim, J., Hamamoto, S., Ravazzola, M., Orci, L., and Schekman, R. (2005) J. Biol. Chem. 280, 7758 –7768 43. Riddell, D. R., Christie, G., Hussain, I., and Dingwall, C. (2001) Curr. Biol. 11, 1288 –1293
VOLUME 282 • NUMBER 38 • SEPTEMBER 21, 2007
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
analysis of these HtrA2⫺/⫺ mice resulted in a conclusion that despite of the suggested role of HtrA2 as a mitochondrial regulator of apoptosis, mammalian HtrA2 is likely involved in protection against cell stresses that involve protein misfolding. Notably, loss of function mutations in HtrA2 gene result in neurodegenerative phenotype with Parkinsonian features in both humans and in mice. Furthermore, S276C loss of function mutation in HtrA2 is responsible for the neurodegenerative phenotype in mnd2 (motor neuron degeneration 2) mice (56). Recently, two mutations in HtrA2 gene (G399S and A141S) were reported in German Parkinson disease (PD) patients (57). Both mutations resulted in defective induction of the proteolytic activity of HtrA2. In this regard, our findings identify yet another PD-associated protein as a component of the protein quality control and proteasome-related disposal machinery. Our results raise interesting new questions on the neuronal roles of HtrA2, especially in the light of the neurodegenerative phenotypes of mnd2 and HtrA2 knock-out mice. Being a part of protein quality control systems in both mitochondria and ER puts HtrA2 in a central position in terms of pathophysiology of neurodegeneration.
HtrA2 Regulates APP Metabolism through ERAD
SEPTEMBER 21, 2007 • VOLUME 282 • NUMBER 38
52.
53.
54. 55. 56.
57.
D. E., Hollister, R. D., Hallmark, O. G., Mancini, R., Felsenstein, K. M., Hyman, B. T., Tanzi, R. E., and Wasco, W. (1996) Nat. Med. 2, 224 –229 Naruse, S., Thinakaran, G., Luo, J. J., Kusiak, J. W., Tomita, T., Iwatsubo, T., Qian, X., Ginty, D. D., Price, D. L., Borchelt, D. R., Wong, P. C., and Sisodia, S. S. (1998) Neuron 21, 1213–1221 Katayama, T., Imaizumi, K., Sato, N., Miyoshi, K., Kudo, T., Hitomi, J., Morihara, T., Yoneda, T., Gomi, F., Mori, Y., Nakano, Y., Takeda, J., Tsuda, T., Itoyama, Y., Murayama, O., Takashima, A., St George-Hyslop, P., Takeda, M., and Tohyama, M. (1999) Nat. Cell Biol. 1, 479 – 485 McCarthy, J. V. (2005) Biochem. Soc. Trans. 33, 568 –572 Yang, L., Sun, M., Sun, X. M., Cheng, G. Z., Nicosia, S. V., and Cheng, J. Q. (2007) J. Biol. Chem. 282, 10981–10987 Jones, J. M., Datta, P., Srinivasula, S. M., Ji, W., Gupta, S., Zhang, Z., Davies, E., Hajnoczky, G., Saunders, T. L., Van Keuren, M. L., Fernandes-Alnemri, T., Meisler, M. H., and Alnemri, E. S. (2003) Nature 425, 721–727 Strauss, K. M., Martins, L. M., Plun-Favreau, H., Marx, F. P., Kautzmann, S., Berg, D., Gasser, T., Wszolek, Z., Muller, T., Bornemann, A., Wolburg, H., Downward, J., Riess, O., Schulz, J. B., and Kruger, R. (2005) Hum. Mol. Genet. 14, 2099 –2111
JOURNAL OF BIOLOGICAL CHEMISTRY
28295
Downloaded from www.jbc.org at Massachusetts General Hospital Treadwell Library on September 21, 2007
44. Tsai, B., Ye, Y., and Rapoport, T. A. (2002) Nat. Rev. Mol. Cell. Biol. 3, 246 –255 45. Meusser, B., Hirsch, C., Jarosch, E., and Sommer, T. (2005) Nat. Cell Biol. 7, 766 –772 46. d’Abramo, C., Massone, S., Zingg, J. M., Pizzuti, A., Marambaud, P., Dalla Piccola, B., Azzi, A., Marinari, U. M., Pronzato, M. A., and Ricciarelli, R. (2005) Biochem. J. 391, 693– 698 47. Kudo, T., Okumura, M., Imaizumi, K., Araki, W., Morihara, T., Tanimukai, H., Kamagata, E., Tabuchi, N., Kimura, R., Kanayama, D., Fukumori, A., Tagami, S., Okochi, M., Kubo, M., Tanii, H., Tohyama, M., Tabira, T., and Takeda, M. (2006) Biochem. Biophys. Res. Commun. 344, 525–530 48. Wang, Q., Li, L., and Ye, Y. (2006) J. Cell Biol. 174, 963–971 49. Bertram, L., Hiltunen, M., Parkinson, M., Ingelsson, M., Lange, C., Ramasamy, K., Mullin, K., Menon, R., Sampson, A. J., Hsiao, M. Y., Elliott, K. J., Velicelebi, G., Moscarillo, T., Hyman, B. T., Wagner, S. L., Becker, K. D., Blacker, D., and Tanzi, R. E. (2005) N. Engl. J. Med. 352, 884 – 894 50. Vaux, D. L., and Silke, J. (2003) Biochem. Biophys. Res. Commun. 304, 499 –504 51. Kovacs, D. M., Fausett, H. J., Page, K. J., Kim, T. W., Moir, R. D., Merriam,
