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J. Biol. Chem., Vol. 278, Issue 35, 32784-32793, August 29, 2003
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¶
From the
Basic Research Laboratory and the
Basic Research Program, Science Applications
International Corporation Frederick, NCI, National Institutes of Health,
Frederick, Maryland 21702
Received for publication, April 14, 2003
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ABSTRACT |
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 TOP ABSTRACT INTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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INTRODUCTION |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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250-amino acid ATPase domain contains the consensus Walker A and B
motifs, which are responsible for ATP binding and ATP hydrolysis,
respectively, and a second region of homology, which distinguishes the AAA
family from other Walker-type ATPases. In addition to sequence homology, the
family members almost always form a ring-shaped oligomeric structure. The
contrast between the functional diversity and the high sequence and structural
similarities suggests that AAA proteins play a common and fundamental role in
cells, and the ring-shaped oligomeric structure is essential for such a
role.
As other AAA proteins, VCP plays an important role in numerous seemingly unrelated cell activities, including membrane fusion (8–10), cell cycle regulation, stress response, programmed cell death, B and T cell activation, endoplasmic reticulum (ER)-associated degradation, and protein degradation (reviewed in Refs. 2–7). Interestingly, all these activities have been shown to be regulated, directly or indirectly, by the ubiquitin-proteasome degradation pathway. This notion suggests that VCP may play a fundamental role in the degradation pathway that underlies all these seemingly unrelated functions. Indeed, we and others (11–16) showed that VCP is genetically and functionally involved in the ubiquitin-proteasome degradation pathway. We further showed (11) that VCP physically associates with the ubiquitinated proteins, through a direct binding to the multiubiquitin chains, thus targeting the substrates to the proteasome for degradation. Recently, several groups (17–22) demonstrated that p97/VCP/Cdc48 along with its partners Ufd1 and Npl4 are required for ER-associated degradation. VCP likely acts as a molecular chaperone that extracts the ubiquitinated proteins from the ER membrane, modifies the conformation of the substrate proteins, and then targets the proteins to the 26 S proteasome for degradation. Moreover, VCP has also been proposed to work as a chaperone with cofactors, such as p47, SVIP, and VCIP135, to mediate membrane fusion in Golgi, ER, and nuclear membrane assembly (23–25). The chaperone activity is powered by the energy generated from the ATP hydrolysis catalyzed by VCP. The conformational change of VCP during the ATPase cycle likely exerts mechanical force on the substrates and possibly the cofactors to accomplish the chaperone actions.
VCP molecule is composed of an N-terminal domain (N), two ATPase domains (D1 and D2), and a C-terminal domain (C). We previously showed that the entire VCP molecule is required for mediating the in vitro degradation of cyclin E (11). The N domain binds to the multiubiquitin chain and thus is responsible for substrate recognition (11), and both D1 and D2 are required for providing the chaperone activity (26). Whether the two ATPase domains function equally and how they coordinate with each other is not understood. Previous reports have shown that the two ATPase domains of type II AAA proteins are different from each other with respect to sequence and function. Frequently, only one of them is a bona fide AAA domain, whereas the other exhibits lower similarity to the AAA consensus sequence. In NSF (27, 28) and Hsp104 (29), D1 is responsible for the major ATPase activity, whereas D2 mediates hexamerization. In bacterial ClpA and trypanosome TClpB, the functions of the respective AAA domains are reversed (30–32). Interestingly, D1 and D2 of VCP share high sequence similarities with each other and with those identified to mediate the ATPase activity. Thus, it is of particular interest to identify the specific functions of D1 and D2 in VCP. Indeed, we recently found that D1 and D2 are not enzymatically equal. Although D2 is responsible for the major ATPase activity at physiological temperature, D1 mediates a heat-enhanced ATPase activity (26).
Electron microscopy (EM) study indicated that VCP has a barrel-like homo-hexameric structure that comprises two-stacked hexameric rings made of the respective AAA modules (33). Although a crystallography study of an ADP-bound N-D1 domain provided significant structural details of the D1 ring (34), very little was known about the D2 ring and the conformation of respective rings during the ATPase cycle. We have taken biochemical approaches to characterize the conformation of VCP, either unbound or bound to ATP/ADP, with the goal of depicting the conformational changes accompanying ATP hydrolysis. We report that hexamer formation in VCP does not depend on the presence of nucleotide. An intact D1 and down-stream linker region is required for the nucleotide-independent oligomerization. In addition, ATP/ADP binding induces dramatic conformational changes in D2. Both intrinsic Trp fluorescence and limited digestion studies suggest that D2 exhibits a relatively relaxed structure in the absence of nucleotide but forms a compact hexameric ring in the presence of ATP/ADP. While this report was being prepared, Rouiller et al. (33) and Beuron et al. (35) reported cryo-EM studies that characterized the different conformations of VCP during the ATPase cycle. In general agreement with their findings, our study, using an independent, biochemical approach, provides additional molecular insights to the conformations of VCP during ATPase cycle.
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MATERIALS AND METHODS |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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All mutations were confirmed by DNA sequencing. All VCP variants were cloned into a His fusion expression vector, pQE60, and expressed as His fusion protein (through the C terminus of VCP) in Escherichia coli strain M15 [pREP4] (QIAexpress system, Qiagen). His-tagged wild type and mutant VCP proteins were purified as previously described (26, 36).
Gel Filtration Chromatography—Affinity-purified His-tagged VCP and variants were centrifuged at 100,000 x g for 30 min before they were loaded onto a Superose 6 column (Amersham Biosciences) equilibrated with buffer containing 20 mM HEPES (pH 7.0), 150 mM NaCl, 4 mM MgCl2, 5 mM DTT, and 1% glycerol. Proteins were eluted at a flow rate of 0.5 ml/min and collected in 16 fractions (0.5 ml/each). An aliquot of 20 µl from each fraction was analyzed by SDS-PAGE and immunoblotting with antibody against the C terminus of VCP (15).
HPLC Analysis of Nucleotides—To detect the nucleotide bound to the purified VCP, samples (0.2 ml of 4 µM) suspended in dialysis buffer (50 mM Tris-HCl, pH 7.5, 80 mM NaCl, 0.1 mM EDTA, and 1 mM DTT) were boiled for 5 min and then passed through a 30,000 MWCO filter (Millipore, Ultra-free MC) as described previously (37). The filtrate was resolved by high-pressure liquid chromatography (HPLC) (Waters model 626) with a Waters Xterra MS C18 column (4.6 mm x 5 cm) equilibrated in 50 mM triethylammonium acetate (pH 7.0). The nucleotide was eluted with a linear gradient of CH3CN from 0 to 98% at a flow rate of 1 ml/min and detected at 254 nm with a 996 PDA detector. For reassembled samples, wild type VCP was dissociated with 6 M urea and reassembled in the presence or absence of ATP for2has previously described (36). The reassembled VCP was passed through a Sephadex G-50 column to remove the unincorporated ATP and then boiled and analyzed by HPLC. For controls, ATP and ADP (0.2 ml of 2.5 µM) were also analyzed.
Native Gel Electrophoresis—In addition to gel filtration chromatography, the oligomeric status of VCP was examined by native polyacrylamide gel electrophoresis (36). The reaction mixture was loaded onto 8% Tris/glycine mini gel (Invitrogen) and electrophoresed at 20 mA for 2hat4 °C. The running buffer contains 25 mM Tris, 195 mM glycine, pH 8–9. The oligomeric status was also verified by analyzing the same samples with gel filtration chromatography.
Fluorescence Spectroscopy—Fluorescence spectra of tryptophan were recorded with a PerkinElmer Life Sciences LS 50 luminescence spectrometer with the use of a 1.0-mm cell at approximately 24 °C. The excitation wavelength was set at 295 nm so as to monitor tryptophan emission between 305 and 450 nm with bandwidths of 5 nm. The protein concentration used was approximately 100 µg/ml. The experiments were carried out in the dialysis buffer plus 10 mM MgCl2 and either with or without 4 mM nucleotides.
Limited Proteolysis—Purified VCP (0.1 mg/ml) was incubated with 5 µg/ml trypsin (Roche Applied Science) at 37 °C for various periods of time in reaction buffer containing 50 mM Tris-HCl (pH 7.5), 5 mM MgCl2, 1 mM DTT and with or without 4 mM ATP. The reactions were terminated by the addition of phenylmethylsulfonyl fluoride (0.5 mM) and SDS-gel sample buffer. The digestion products were separated into two parts. One part was analyzed by SDS-PAGE and stained with a SilverXpress silver staining kit (Invitrogen). The other part was resolved on SDS-gel and immunoblotted with antiserum recognizing either the N or C terminus of VCP (15).
Western Blot Analysis—Western blot analysis was performed as described previously with the following primary antibodies: rabbit anti-VCP C terminus (1:1000), N terminus (1:1000) (15), and mouse anti-His (1:1000) (Qiagen).
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RESULTS |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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Hexamerization of VCP in the Absence of Nucleotide—Our previous study showed that VCP has an unusually high preponderance to form a ring-shaped hexameric structure. Because many AAA proteins assemble into oligomers in the presence of ATP but remain monomeric in the absence of nucleotide, we asked whether this is also true in VCP. Wild type VCP fusion protein was purified (Fig. 1B) and subjected to gel filtration chromatography in the absence of nucleotides. Remarkably, almost all VCP appears in a complex with a molecular size consistent with a hexamer (Fig. 1C). To further confirm this nucleotide independence, an A1A2 double mutant, which harbors a mutation in the ATP-binding site in both D1 and D2 domains (Fig. 1A), was analyzed. The detection of A1A2 as hexamers (Fig. 1D) strongly supported that oligomerization of VCP does not require nucleotide binding.
Although the analyses were performed without the addition of nucleotides, it was formally possible that the purified recombinant VCP already contained a sufficient amount of nucleotides to maintain the hexameric structure. We thus boiled the VCP preparations to release the potentially bound nucleotide and then analyzed the sample by HPLC. Because the control ATP sample exhibits a sharp peak on the chromatogram (Fig. 2A), neither ATP (Fig. 2B) nor ADP (data not shown) was found in the purified wild type and A1A2 preparations. Furthermore, we dissociated VCP to monomers with 6 M urea, reassembled the dissociated VCP in the presence or absence of ATP/ADP (36), removed the unbound nucleotide, and then subjected the samples to HPLC analysis. As we previously reported, although hexameric VCP was efficiently reassembled in both conditions (36), ATP/ADP was only detected in the hexamers reassembled in the presence of added nucleotide (Fig. 2C). This result validated our ability to detect the ATP/ADP bound to hexameric VCP and further supported the nucleotide-independent nature of VCP oligomerization. Taken together, we conclude that nucleotide is not required for forming stable hexameric VCP complexes, an unusual property among AAA proteins.
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D1-linker, but Not N or D2-C, Is Required for Nucleotide-independent Hexamerization—Next, we determined which one or more domains are responsible for the nucleotide-independent hexamerization. Prior crystallography study showed that the N-D1 domain (residues 2–458) of p97 forms a hexameric structure that tightly binds to ADP, and no nucleotide-free hexameric N-D1 was detected (34). This seems to suggest that N-D1 alone is not sufficient for the nucleotide-independent hexamerization. To identify the sequence requirement, we generated a series of deletion mutants with progressive N- or C-terminal truncations (Fig. 3A). The purified VCP variants (Fig. 3B) were subjected to native gel electrophoresis in the absence of ATP. As shown in Fig. 3C (also summarized in Fig. 3A), wild type and variants 1–511, 1–481, and 141–806 can form hexamers without the addition of nucleotides. These variants all contain an intact D1 (#200–458) and the subsequent linker (#458–473) region (designated as D1-linker) but lack at least part of the N, D2, or C domains. Thus, the D1-linker may be necessary for the hexamerization, and N, D2, and C are dispensable for the process. Moreover, variants 2–458, 443–806, and 268–806, all lacking at least part of the D1-linker region, failed to form hexamers (Fig. 3, A and C), indicating the requirement for D1-linker. Comparing variants 2–458 (N-D1) and 1–481, it is apparent that the linker region plays a critical role in nucleotide-free hexamerization. Without the linker, VCP is mostly present in monomeric form. This may provide the explanation why N-D1 cannot form hexamers without ADP as reported in previous crystallography study (34). We conclude that the D1-linker domain, but not the N or D2-C domain, is required for the nucleotide-independent hexamerization of VCP.
Intrinsic Tryptophan Fluorescence Study: Dramatic Conformational Change of D2 upon Nucleotide Binding—We previously demonstrated that the ATPase activity of VCP is required in carrying out its biological functions, such as ubiquitin-proteasome-mediated protein degradation. Thus, it is important to characterize the conformational changes of VCP during the ATPase reaction. Because a crystal structure of full-length VCP is not available, we took biochemical approaches to study the conformation of VCP either unbound or bound to ATP/ADP, representing specific phases of the ATPase cycle. Based on the facts that Trp fluorescence represents a sensitive probe for conformational change and wild type VCP contains three tryptophan (Trp) residues, we measured the changes in the fluorescence emission spectra of Trp under different nucleotide conditions. Because the experiments were carried out at room temperature, at which VCP exhibits negligible ATPase activity (26), the change in fluorescence after ATP addition is attributed to mainly the binding and not the hydrolysis of ATP. As shown in Fig. 4A and Table I, the Trp fluorescence of VCP peaks at a wavelength of 345 nm, and binding to ATP or ADP results in increases of 53.9 ± 2.0% or 28.9 ± 1.7%, respectively. These increases suggest that nucleotide binding to VCP induces a conformational change in VCP molecule. The enhancement of fluorescence with ADP is weaker than that with ATP, probably implicating a less dramatic conformational change. Therefore, VCP binding to ATP induces an initial conformational change, and further changes take place during the subsequent ATP hydrolysis and ADP release.
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To determine whether D1 or D2 domain contributes to this ATP/ADP-enhanced Trp fluorescence, we further studied the ATP-binding site mutants, A1 and A2. Although the basal level and the peak wavelength (345 nm) of the Trp fluorescence of both mutants did not change from those of the wild type, the extent of fluorescence change in the presence of nucleotides varied significantly (Fig. 4B and Table I). When ATP and ADP were added, the Trp fluorescence of A1 increased 58.0 ± 3.6% and 25.3 ± 2.8%, respectively, similar to those observed in the wild type. By sharp contrast, the increase was totally abolished in A2. This result indicates that an intact ATP-binding site in D2, but not in D1, is necessary to bring about the ATP/ADP-enhanced Trp fluorescence of VCP. In other words, the Trp fluorescence change of VCP upon ATP/ADP binding reflects a significant conformational change in D2, but not in D1. Notably, this conformational change of D2 can take place without nucleotide binding to the D1 domain.
Fluorescence Change in Trp-476 as the Indicator for Conformational Changes in D2—To further characterize the ATP/ADP-increased Trp fluorescence, we identified the specific Trp residue that is responsible for the fluorescence changes. VCP contains three Trp residues at positions 454, 476, and 551. We changed each Trp to alanine to assess the impact (Fig. 1, A and B). Mutations of Trp-454 (Fig. 5A and Table I) and Trp-551 (Fig. 5B and Table I) did not affect the ATP/ADP-enhanced fluorescence pattern, although Trp-551 mutation resulted in a slightly lower basal level fluorescence. Thus, Trp-454 and Trp-551 are not the major contributors for the fluorescence changes in VCP upon ATP/ADP binding. Strikingly, the basal fluorescence intensity of W476A mutant was much lower than that of the wild type, and ATP/ADP binding did not enhance the fluorescence (Fig. 5C and Table I). The lack of fluorescence change is not a result of its incapacity to bind nucleotide or form hexamers, because the ATPase activity and hexamerization status of W476A mutant are the same as those of the wild type (data not shown). Therefore, Trp-476 is the main contributor to the ATP/ADP-enhanced fluorescence and serves as an indicator for the conformational change of D2. It should be noted that these data only assess the status of D2 and do not implicate a lack of changes in D1. It is possible that ATP/ADP binding also induces conformational changes in D1, but there is no appropriate Trp residue in D1 to indicate the changes, and/or the change in D1 is not sufficiently propagated to D2 to induce detectable fluorescence change in Trp-476.
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Protection of VCP from Trypsin Proteolysis in the Presence of
Nucleotides—To detect the conformational changes at a more global
level, we then performed limited proteolysis in different nucleotide
conditions. In this assay, it is presumed that a high sensitivity to
proteolysis suggests a more open and dissociated conformation, whereas a low
sensitivity indicates a relatively closed and associated conformation. Also,
the efficiency of proteolytic cleavage at exposed sites on the surface of the
complex correlates with the flexibility of the protein. The trypsin digestion
pattern revealed by silver staining showed that VCP is readily digested in the
absence of nucleotides after 40 min. However, in the presence of ATP, ADP, or
ATP
S an 87-kDa fragment (p87) is protected from digestion even after
100 min of incubation (Fig.
6A). Subsequent immunoblot analysis showed that p87 was
only detected by the antiserum specific to the N terminus
(Fig. 6B) but not the
C terminus (Fig. 6C)
of VCP. Therefore, p87 consists of N, D1, and D2 domains
(Fig. 6D), and the C-terminal
the 10-kDa fragment of VCP is readily cleaved off by trypsin and probably
represents a loosely structured tail. It was also noted that, in the absence
of nucleotide, several C-terminally truncated intermediates were observed
(Fig. 6B). Among them,
a major intermediate with a molecular size of 58 kDa (p58) was detected
at 60 min. Based on the calculated molecular size and similar gel mobility
between p58 and VCP1–481 protein (data not shown), we deduced that p58
represents the N-D1-linker fragment (Fig.
6D). These results suggest that, in the absence of
nucleotide, the hexameric VCP complex comprises three substructures: a
relatively compact and trypsin-resistant N-D1-linker structure, a more open
and trypsin-sensitive D2, and a highly protease-sensitive C-terminal domain.
In response to nucleotide binding, VCP undergoes a conformational change such
that a trypsin-resistant N-D1-D2 hexameric structure is formed. This
conformational change likely takes place more drastically in the D2 domain,
which changes from a trypsin sensitive to a resistant state.
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Requirement of Nucleotide Binding to D2 for Trypsin Resistance—To demonstrate that ATP binding to D2 is responsible for the protection and stabilization of the D2 subcomplex, ATP-binding site mutants, A1 and A2, were subjected to limited trypsin proteolysis. As shown in Fig. 7A, when the binding site in D1 is mutated ATP/ADP still protects the N-D1-D2 complex, resulting in the stabilization of p87 fragment as it does in the wild type (Fig. 6B). By contrast, mutation in D2 abolished this protection effect of ATP/ADP such that the predominant digestion product was the N-D1-linker fragment (p58) (Fig. 7B). Thus, an intact ATP-binding site in D2, but not D1, is required to confer protection of the N-D1-D2 complex from proteolysis. In other words, D1 almost always forms a trypsin-resistant ring regardless of the nucleotide conditions, but D2 only does so when it binds to nucleotides.
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Stable D1 Ring and Minor Conformational Changes in D1 upon Nucleotide Binding—A closer examination of Fig. 7B revealed that ATP/ADP binding to D1 does confer a slightly increased protection to the p58 N-D1-linker subcomplex. This observation suggests that nucleotide binding to D1 also induces conformational changes. To directly study this, we carried out trypsin digestion analysis on VCP 1–481 mutant (Fig. 3, A and B), which is devoid of the D2-C domain. As shown in Fig. 8, the presence of ATP or ADP indeed changes the protein to be more resistant to trypsin. However, the change is significantly less dramatic than that observed in D2 (compare Figs. 6B, 7A, and 8). In summary, VCP 1–481 exists as a stable hexamer in the absence of nucleotides, and the D1 ring undergoes minor conformational changes during the ATPase cycle.
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DISCUSSION |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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The difference in nucleotide requirement between VCP and other AAA hexamers
may be explained by the structural details revealed by the crystallography
studies of p97 N-D1 (34), NSF
D2 (38,
39), and full-length ClpA
(40). In the
nucleotide-binding pocket of NSF D2, in addition to Lys-549 and Lys-708,
another lysine, Lys-631, from one of the neighboring subunits also contacts
the -phosphate of ATP
(38,
39). Therefore, upon releasing
ADP at the end of ATPase cycle, the resulting electrostatic repulsion between
the three Lys residues and the change of hydrophobic interfaces lead to a
dramatic structural destabilization. The recently solved crystal structure of
full-length ClpA also reveals strong electrostatic interactions in D1, the
major hexamerization domain. At least three positively charged residues from
the neighboring subunit are within salt bridge distance from the bound ADP. In
addition, five positively charged residues from the same neighbor also
contribute to the nucleotide-binding site
(40). Therefore, nucleotide
binding is intimately coupled with hexamer formation in ClpA D1. By contrast,
residues interacting with the 
-phosphate of the bound ADP in p97 N-D1
are all in the vicinity of Lys-251, which is highly conserved in the P-loop
and is the only Lys in the nucleotide binding pocket of p97 N-D1. Although two
Arg residues (Arg-359 and Arg-362) from an adjacent protomer protrude into the
nucleotide-binding pocket, Arg-362 forms a salt bridge with Glu-305 in the
Walker B motif, leaving only Arg-359 to interact with the bound nucleotide
(34). Because VCP lacks the
electrical repulsion observed in NSF and ClpA, the hexamer would not be
destabilized when ADP is released.
In this study, we report the novel finding that D1-linker sequences are required for the nucleotide-independent hexamerization. The absolute requirement for the linker region in this event explains why N-D1 could not form hexamers on its own (34). The high trypsin resistance of the p58 N-D1-linker (containing 18 and 1 trypsin cleavage sites in D1 and linker, respectively) suggests that the linker region is sterically inaccessible to the protease. Moreover, our unpublished result also suggests that this linker region is at least partially buried. This is because when a PreScission protease (Amersham Biosciences) cleavage site was inserted between residues 459 and 460, whereas the protease readily cuts the urea-dissociated VCP, it could not access the hexamer at any nucleotide states (empty, ATP, or ADP). Because the linker sequence was originally defined by sequence alignment, it is possible that this linker region (or at least part of it) could be considered part of the D1 domain.
The Trp florescence study showed that VCP binding to ATP and ADP induces a
fluorescence increase of 54 and 29%, respectively
(Fig. 4 and
Table I). Site-specific mutant
analyses further indicated that this fluorescence change is mainly contributed
by nucleotide binding to the D2 domain. Although VCP molecule has three Trp
residues (positions 454, 476, and 551), only Trp-476 is critical for this
ATP/ADP-induced fluorescence change. Thus Trp-476 can serve as the indicator
for the fluorescence assay (Fig.
5 and Table I). The
change is unlikely resulted from a direct contact between Trp-476 and the
nucleotide, because W476A mutant still binds ATP and maintains a wild type
ATPase activity (data not shown), and moreover, functional alignment of D1 and
D2 does not suggest a direct interaction between Trp-476 and nucleotide. Thus,
the Trp fluorescence increase likely results from the conformational changes
of VCP induced by nucleotide binding to D2 domain without direct contacting
Trp-476. Our unpublished result also showed that VCP variant that contains a
PreScission protease cleavage site inserted at position 476 could only be cut
in the presence of ATP, which obviously changes the peptide segment from a
buried to an exposed state. Hence, ATP binding to D2 domain probably induces
intra- and inter-subunit conformational changes, resulting in alterations in
the microenvironment around the Trp-476 residue. It should be noted that,
because D1 domain does not have an indicator Trp residue, this assay could not
be used to assess the possible conformational changes in the D1 domain.
Limited trypsin digestion has been used to characterize the conformational changes resulted from oligomerization of a number of AAA proteins, e.g. NSF (41). Comparison of the proteolysis patterns of the wild type, A1, A2, and VCP 1–481 in different nucleotide conditions (Figs. 6, 7, 8) led to the conclusions consistent with those obtained in fluorescence study. Although N-D1-linker subcomplex has a relatively compact and trypsin-resistant structure, it exhibits minor conformational changes during the ATPase cycle. On the other hand, the D2 subcomplex is much more flexible. In the context of a full-length VCP hexamer, D2 converts from a trypsin-sensitive to a resistant form after ATP/ADP binding. Therefore, in the presence of nucleotide, N-D1-D2 (p87) is still protected from trypsin digestion even after a prolonged reaction (>60 min) (Fig. 6). These data directly suggest that during the ATPase cycle D2 forms a compact hexamer upon ATP binding but destabilizes and adopts a more relaxed and open structure after ADP release. This result is consistent with our previous finding that at physiological temperature D1 exhibits very low ATPase activity but D2 mediates the major enzyme activity. It is speculated that at physiological temperature the two AAA domains carry out distinct functions during the ATPase cycle. The D1 ring, although it also undergoes minor conformational changes, provides a structural framework that keeps the substrate-binding N domain and the enzymatic D2 domain in a proper context. On the other hand, the primary function of D2 is to carry out ATP hydrolysis, which couples with the conformational changes that can be propagated to the D1 and N domains. Our previous study showed that, at elevated temperature, e.g. 50 °C, D1 is capable of mediating heat-enhanced ATPase activity. It is possible that at such an elevated temperature the D1 ring is expanded and less rigid, and becomes more D2 like, in terms of undergoing more dramatic conformational changes and catalyzing ATP hydrolysis.
While the manuscript for this report was being prepared, Rouiller et
al. (33) and Beuron
et al. (35) reported
cryo-EM studies of VCP at different nucleotide conditions. Based on the
molecular "snapshots" captured in these studies, models were
proposed to depict the conformational changes of VCP during the ATPase cycle.
Interestingly, although in general agreement, the two studies report a number
of conflicting findings. For instance, Rouiller et al., but not
Beuron et al., showed six side protrusions associated with the D2
ring near the central plane of the p97 hexamer
(33). Although the
identification of this side protrusion is not clear, two possibilities have
been proposed, namely the linker region (residues 458–473) between D1
and D2 and the C-terminal tail
(33). The side protrusions
appear on the surface of the hexameric complex and are expected to be
accessible to proteases. Nevertheless, our trypsin and PreScission digestion
experiments showed that the linker region is inaccessible to the proteases and
at least partially buried (see above). Thus, the linker is not likely to be
the side protrusion detected on the surface of the complex. On the other hand,
our limited proteolysis study (Figs.
6 and
7A) indicated that the
C-terminal tail of VCP (approximately from residue 733 to 806) is readily
digested. Given the fact that this region contains five trypsin cutting sites
and that trypsin digestion failed to recover a 10-kDa C-terminal
fragment, the C domain likely is loosely structured and hence readily cleaved.
Together, our results would favor the speculation of C domain being the side
protrusion.
In general, our findings are in close agreement with those reported by Rouiller et al., in the following aspects: 1) hexamer formation does not require the presence of nucleotide; 2) the N domain is not required for hexamerization; 3) D1 undergoes minor conformational changes during ATP hydrolysis; and 4) nucleotide binding induces pronounced conformational changes in D2. Although our proteolysis assays did not detect significant differences between the ATP- and ADP-bound forms of VCP, Trp fluorescence analysis revealed distinct profiles of the two states. Our previous study showed that ATP-bound VCP can bind polyubiquitin chains, but ADP form cannot. Because N domain is responsible for binding to the substrate and cofactors, the ADP-induced conformational change must be sufficient to cause the N domain to release the ligand. Presumably, N domain also undergoes coordinated conformational or positional changes to bind or to release the ligand. In agreement, both EM studies demonstrated that N domain is highly mobile and undergoes significant positional changes during the ATPase cycle (33, 35). Crystallography study identified a partially buried linker region (residues 186–208) between the N and D1 domains (34). This linker supposedly works as an arm that moves the N domain up and down or around the periphery of D1 ring. Based on the high flexibility of this "linker arm," it is predicted to be readily accessible to proteases. Unexpectedly, despite the presence of two potential cleavage sites in this linker sequence (Lys-190 and Arg-191), this region is not readily digested by trypsin. We speculate that, whereas the majority of the linker may be indeed exposed and mobile, the sequences around the trypsin cleavage sites may happen to be buried in the complex. Hence, our inability to detect ready digestion in this region is because of the lacking of trypsin sites in the exposed and mobile region rather than physical inaccessibility.
Based on the biochemical data presented in this study, we propose the following model (Fig. 9). The full-length VCP exists in a homo-hexameric structure regardless of the nucleotide condition. Neighboring D1-linker domains form a relatively stable ring, which holds the full-length VCP hexamer together throughout the ATPase cycles. Although D1 undergoes detectable conformational changes during the ATPase cycle, the changes are relatively minor. On the other hand, the hexameric ring made of the neighboring D2 domains is much more mobile. It is more open and relaxed in the absence of nucleotide, but adopts a more closed and compact conformation after binding to nucleotide. Although the differences between the ATP and ADP forms of VCP is not specified in this study, the ADP-bound VCP adopts a unique conformation (illustrated by strips) such that it is incapable of binding to the substrate (11). Obviously, this model needs to be further tested by other experimental systems, such as high resolution structures in different nucleotide conditions.
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FOOTNOTES |
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¶ To whom correspondence should be addressed. Tel.: 301-846-1478; Fax: 301-846-7034; E-mail: licc{at}ncifcrf.gov.
1 The abbreviations used are: VCP, valosin-containing protein; ER,
endoplasmic reticulum; EM, electron microscopy; DTT, dithiothreitol; HPLC,
high-pressure liquid chromatography.
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ACKNOWLEDGMENTS |
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REFERENCES |
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TOPABSTRACTINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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 L. C. Briggs, G. S. Baldwin, N. Miyata, H. Kondo, X. Zhang, and P. S. Freemont Analysis of Nucleotide Binding to P97 Reveals the Properties of a Tandem AAA Hexameric ATPase J. Biol. Chem., May 16, 2008; 283(20): 13745 - 13752. [Abstract] [Full Text] [PDF] |
