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Deamidation of N-terminal Gln by NtQ-amidase, a previously undescribed N-terminal amidohydrolase, is a part of the N-end rule pathway of protein degradation. We detected the activity of NtQ-amidase, termed Ntaq1, in mouse tissues, purified Ntaq1 from bovine brains, identified its gene, and began analyzing this enzyme. Ntaq1 is highly conserved among animals, plants and some fungi, but its sequence is dissimilar to sequences of other amidases. An earlier mutant in the Drosophila Cg8253 gene that we show here to encode NtQ-amidase has defective long-term memory. Other studies identified protein ligands of the uncharacterized human C8orf32 protein that we show here to be the Ntaq1 NtQ-amidase. Remarkably, “high-throughput” studies have recently solved the crystal structure of C8orf32 (Ntaq1). Our site-directed mutagenesis of Ntaq1 and its crystal structure indicate that the active site and catalytic mechanism of NtQ-amidase are similar to those of transglutaminases.
The N-end rule relates the in vivo half-life of a protein to the identity of its N-terminal residue (reviewed by (Mogk et al., 2007; Tasaki and Kwon, 2007; Varshavsky, 1996, 2008a; Varshavsky, 2008b). Degradation signals (degrons) that can be targeted by the N-end rule pathway are of two “topologically” distinct kinds: N-terminal degrons, called N-degrons, and internal (non-N-terminal) degrons (Ravid and Hochstrasser, 2008; Varshavsky, 1996; Wang et al., 2008). The main determinant of an N-degron is a destabilizing N-terminal residue of a substrate protein (Figure 1A). The other determinants of N-degron are a substrate’s internal Lys residue (the site of formation of a poly-Ub chain) and a nearby unstructured region (Bachmair and Varshavsky, 1989; Prakash et al., 2009; Suzuki and Varshavsky, 1999). An N-degron is produced from a precursor, called a pre-N-degron, through a protease-mediated cleavage of a substrate that exposes a destabilizing N-terminal residue.
E3 Ub ligases of the N-end rule pathway, called N-recognins, are defined as E3s that can recognize (target) at least some N-degrons (Figure 1A) (Tasaki and Kwon, 2007; Varshavsky, 1996). Some of substrate-binding sites of an N-recognin target N-degrons of specific substrates, while other sites of the same N-recognin target internal (non-N-terminal) degrons of other protein substrates. At least four N-recognins, Ubr1, Ubr2, Ubr4 and Ubr5, mediate the N-end rule pathway in mammals and other multicellular eukaryotes (Figure 1A) (Tasaki and Kwon, 2007; Tasaki et al., 2009). The N-end rule pathway of the yeast Saccharomyces cerevisiae is mediated by a single N-recognin, Ubr1, a 225-kDa sequelog of mammalian Ubr1 and Ubr2 (Hwang et al., 2009; Hwang and Varshavsky, 2008; Xia et al., 2008b). (A note on terminology: “sequelog” and “spalog” denote, respectively, a sequence that is similar, to a specified extent, to another sequence, and a 3D structure that is similar, to a specified extent, to another 3D structure. Besides their usefulness as separate terms for sequence and spatial similarities, the rigor-conferring advantage of “sequelog” and “spalog” is their evolutionary neutrality, in contrast to interpretation-laden terms such as “homolog”, “ortholog” and “paralog” (Varshavsky, 2004).)
The functions of the N-end rule pathway (Figure 1A) include selective degradation of misfolded proteins; the sensing of nitric oxide (NO), oxygen, heme, and short peptides; the fidelity of chromosome segregation; the control of peptide import; regulation of signaling by transmembrane receptors, through the NO/O2-controlled degradation of specific RGS proteins that regulate G proteins; regulation of DNA repair, apoptosis, meiosis, spermatogenesis, neurogenesis, and cardiovascular development; the functioning of specific organs, in particular the brain and the pancreas; and regulation of leaf senescence, seed germination, and other processes in plants ((Eisele and Wolf, 2008; Holman et al., 2009; Hu et al., 2005; Hu et al., 2008; Hwang et al., 2009; Hwang and Varshavsky, 2008; Rao et al., 2001; Tasaki and Kwon, 2007; Varshavsky, 2008a; Xia et al., 2008a; Zenker et al., 2005), and refs. therein).
The N-end rule has a hierarchic structure (Figure 1A). N-terminal Asn and Gln are tertiary destabilizing residues in that they function through their enzymatic deamidation, to yield the secondary destabilizing N-terminal residues Asp and Glu (Baker and Varshavsky, 1995; Kwon et al., 2000). Destabilizing activity of N-terminal Asp and Glu requires their conjugation to Arg, one of the primary destabilizing residues, by the ATE1-encoded Arg-tRNA-protein transferase (R-transferase) (Hu et al., 2005; Hu et al., 2008; Kwon et al., 2002). In mammals and other eukaryotes that produce NO, the set of arginylated residues contains not only Asp and Glu but also N-terminal Cys, which is arginylated after its oxidation to Cys-sulfinate or Cys-sulfonate, in reactions that require NO, oxygen (O2) or their derivatives (Figure 1A) (Hu et al., 2005; Tasaki and Kwon, 2007).
In S. cerevisiae, the deamidation branch of the N-end rule pathway is mediated by the Nta1 NtN,Q-amidase, which can deamidate either Asn or Gln at the N-termini of polypeptide substrates (Baker and Varshavsky, 1995). In mammals and other multicellular eukaryotes, N-terminal Asn and Gln are deamidated by N-terminal amidases (Nt-amidases) of two kinds (Figure 1A). One of them, the previously characterized Ntan1 NtN-amidase, is specific for N-terminal Asn (Grigoryev et al., 1996). In part through analyses of Ntan1−/− mice, which could not deamidate N-terminal Asn (Kwon et al., 2000), it has been inferred that there also exists a Gln-specific NtQ-amidase.
In the present work, we detected the activity of NtQ-amidase, termed Ntaq1, in mouse tissues, purified Ntaq1 from bovine brains, identified its gene, and began studies of this previously undescribed enzyme (Figure 1A). The sequence of mouse Ntaq1 (NtQ-amidase) is highly conserved among animals, plants and some fungi, but is dissimilar to sequences of other amidases, including the N-terminal amidases Ntan1 (NtN-amidase) and Nta1 (NtN,Q-amidase). A tungus mutant in the previously uncharacterized Drosophila melanogaster Cg8253 gene was found to have defective long-term memory (Dubnau et al., 2003). We show here that this Drosophila gene encodes the counterpart of mouse Ntaq1. In addition, previous proteomic studies identified ~15 putative protein ligands of an uncharacterized human protein encoded by C8orf32 ((Lim et al., 2006) and refs. therein). We show here that C8orf32 is the human Ntaq1 NtQ-amidase. Remarkably, “high-throughput” crystallographic studies of human proteins have recently solved the crystal structure of C8orf32 (Ntaq1) (Bitto et al., 2008). In conjunction with its crystal structure, our site-directed mutagenesis of Ntaq1 indicates that the active site and catalytic mechanism of NtQ-amidase are similar to those of transglutaminases. Thus, the discovery and study of NtQ-amidase as a component of the N-end rule pathway (Figure 1A) were “instantly” complemented by a crystal structure of this enzyme, a set of its putative protein ligands, and evidence for its role in memory processes.
The S. cerevisiae Nta1 NtN,Q-amidase (Baker and Varshavsky, 1995) (Figure S1) belongs to the nitrilase superfamily, defined through sequelogies (sequence similarities) and spalogies (spatial similarities) (Varshavsky, 2004) among its members. Mammalian Ntan1 NtN-amidases, which can deamidate N-terminal Asn but not N-terminal Gln (Grigoryev et al., 1996), are not sequelogous to yeast Nta1. Initially, we attempted a bioinformatics-based identification of a putative NtQ-amidase, termed Ntaq1. Several (weak) sequelogs of mouse Ntan1 or S. cerevisiae Nta1 were identified in the mouse genome, but none of those proteins, when expressed in nta1Δ S. cerevisiae, were able to restore the Gln-specific branch of the N-end rule pathway in that mutant (data not shown). The resulting impasse led to a direct-isolation approach (Figure 1B, C).
Reporters for the NtQ-amidase assay (Figure 1B and Figure S2A) comprised the E. coli dihydrofolate reductase (DHFR) moiety fused to a C-terminal peptide (denoted as “bt”) that was biotinylated in vivo, and also the N-terminal His10-Ub moiety followed by a sequence derived from the N-terminal sequence of α-lactalbumin (Hu et al., 2008). The resulting set of reporters, His10-Ub-X-(LTKCEV)-DHFRbt (X = Q; E; N; EQ; MQ; GQ; REQ) is denoted as His10-Ub-X-DHFRbt. A purified His10-Ub-X-DHFRbt was immobilized, via its C-terminal biotin moiety, on neutravidin beads, and thereafter treated with purified USP2cc deubiquitylating enzyme to remove N-terminal His10-Ub, followed by incubation with a cell extract. The resulting samples were washed and incubated with purified R-transferase and radiolabeled Arg, followed by SDS-PAGE and autoradiography of a reporter (Figure 1B, Figure 2A–C and Figure S2).
This assay (Figure 1B) detected varying levels of NtQ-amidase activity in all mouse tissues examined (Figure 2A, B and Figure S2). Control assays included incubations of immobilized X-DHFRbt reporters with buffer alone, before the addition of R-transferase (Figure 2B). The NtQ-amidase activity was detected by comparing the arginylation of Glu-DHFRbt, a substrate of R-transferase (Figure 1A), to the arginylation of Gln-DHFRbt, which can be arginylated only after its N-terminal deamidation (Figure 1B and Figure 2A, B). Yet another control involved pre-heating of brain extracts at 95°C for 5 min. Glu-DHFRbt could be arginylated by the (subsequently added) R-transferase irrespective of whether a brain extract was heated or unheated before incubation with this reporter. In contrast, the same test with Gln-DHFRbt resulted in a negligible arginylation if a heated brain extract was used (data not shown), implying that deamidation of Gln-DHFRbt was an enzymatic reaction. The non-reporter bands of 14C-labeled (arginylated) proteins were endogenous proteins that cofractionated with neutravidin beads (Figure 2A and Figure S2B). Some of these proteins might be physiological substrates of R-transferase.
Having detected NtQ-amidase (Ntaq1), we developed a procedure for its purification from calf brains that included ammonium sulfate precipitation of proteins from a brain extract, followed by ion exchange, hydrophobic and gel filtration chromatography (Figure 1C, Figure 2C and Figure S3A, B). In the last step, a gel filtration on a Superose-12 column, the Ntaq1 NtQ-amidase activity migrated as a symmetric peak at ~26 kDa (vis-a-vis globular proteins as Mr standards) (Figure 2C). Silver staining of SDS-PAGE-fractionated proteins from peak activity fractions showed two nearly comigrating major bands, the lower band being more abundant in the peak activity fraction (Figure 2C, D). The two proteins were separately excised from the gel and partially sequenced, using in-gel digestion with trypsin and mass spectrometry (MS) (Figure 2D). The upper band was identified as the bovine counterpart of the human heme-binding protein HEBP2. The lower band was identified as the 207-residue bovine counterpart of human C8orf32 (FLJ10204), a previously inferred 205-residue (24-kDa) protein of unknown function (Figure 2D).
Mouse Hebp2 cDNA and Wdyhv1 cDNA (Acc. No. NC_000081.5) (the latter is the counterpart of human C8orf32 (FLJ10204) cDNA) were subcloned into the plasmid p425Met25. The FLAG-tagged mouse Hebp2f and Wdyhv1f were expressed in an nta1Δ mutant of S. cerevisiae that lacked the endogenous Nta1 NtN,Q-amidase, and cell extracts were examined using the NtQ-amidase assay described in Figure 1B. Although mouse Hebp2f and Wdyhv1f were expressed in S. cerevisiae at comparable levels, as determined by SDS-PAGE and immunoblotting with anti-FLAG antibody, only extracts from cells that expressed Wdyhv1f exhibited the NtQ-amidase activity (data not shown). To verify the conclusion that Wdyhv1f was the Ntaq1 NtQ-amidase (Figure 1A), we examined Wdyhv1f in vivo as well, using nta1Δ S. cerevisiae that carried plasmids expressing Ub-X-β-galactosidases (Ub-X-βgals), a set of reporters in which X was a variable residue. Cotranslational deubiquitylation of these Ub fusions produces X-βgal reporter proteins. Their enzymatic activity can be employed to compare metabolic stabilities of these (otherwise identical) reporters bearing different N-terminal residues (Baker and Varshavsky, 1995; Varshavsky, 2005).
As would be expected (Figure 1A), the levels of Asp-βgal and Glu-βgal (their degradation does not require deamidation) were low in all of the tested genetic backgrounds, signifying short in vivo half-lives of these X-βgals, whereas the levels of long-lived Met-βgal were high in the same backgrounds (Figure 3A–D). The levels of Asn-βgal and Gln-βgal were high in nta1Δ cells but could be made low by re-introduction of yeast NTA1 encoding NtN,Q-amidase (Figure 3A, D). Crucially, the levels of Gln-βgal were high in nta1Δ S. cerevisiae but became low in the presence of the mouse Ntaq1f NtQ-amidase (Figure 3A, B). A “reciprocal” result was obtained with nta1Δ cells that expressed the previously characterized mouse Ntan1 NtN-amidase (Figure 3A, C). Thus, mouse Ntaq1 and Ntan1 are specific for N-terminal Gln and N-terminal Asn, respectively, but not for both of these residues, in contrast to S. cerevisiae Nta1. These in vivo results, in agreement with the in vitro data cited above, confirmed the identification of mouse Ntaq1 as an NtQ-amidase.
A plasmid that expressed a mouse Ntaq1-EGFP fusion from the PCMV promoter was transiently transfected into NIH-3T3 cells. The resulting fluorescence patterns (Figure S3C–H) suggested a cytosolic/nuclear location of Ntaq1. One caveat is that Ntaq1-EGFP was overexpressed in comparison to the endogenous Ntaq1 NtQ-amidase. The endogenous Ntaq1 gene is expressed, at varying levels, in most cell types, given the presence of NtQ-amidase activity in all mouse tissues examined (Figure 2A–D and S2). In agreement with this conclusion, the data in Allen Brain Atlas (http://www.brain-map.org/) indicate that Ntaq1 mRNA (denoted as Cg8253 in the Atlas) is expressed, at varying levels, throughout the mouse brain.
A mouse gene (Acc. No. NC_000081.5), termed Ntaq1 in the present work, is located on Chromosome 15, is ~17.2 kb long, contains 6 exons, and encodes the 209-residue (24-kDa) Ntaq1 NtQ-amidase (Figure 4A). The mouse genome does not contain statistically significant sequelogs of mouse Ntaq1, suggesting (but not proving) that Ntaq1 is the sole source of NtQ-amidase at least in mammals. Given the in vitro and in vivo evidence described above (Figure 1–Figure 3), it was expected that a down-regulation of Ntaq1 in mouse cells would result in a decrease of NtQ-amidase activity. To verify this expectation, we carried out RNAi with mouse NIH-3T3 cells that expressed Ntaq1-specific pre-microRNA (pre-miRNA), and indeed observed a significant decrease of the in vivo levels of both the NtQ-amidase activity and the Ntaq1 protein, in comparison to control cells (Figure S4A, B; see Experimental Procedures and the legend to Figure S4 for details). This decrease could be detected either by carrying out the NtQ-amidase activity assay with extracts of RNAi-treated and mock-treated cells (Figure S4A), or by immunoblotting the same extracts with an affinity-purified rabbit anti-Ntaq1 antibody, raised against purified mouse Ntaq1 that was produced in the yeast Pichia pastoris (Figure 2E and Figure S4B).
In a different, in vitro-based approach, we selectively depleted Ntaq1 from cell extracts, using the above affinity-purified anti-Ntaq1 antibody. A depletion of endogenous Ntaq1 from extracts of NIH-3T3 cells with the antibody to Ntaq1 resulted in extracts that did not contain NtQ-amidase activity above “nonspecific” (control) backgrounds, whereas the otherwise identical treatment of cell extracts with preimmune serum did not significantly decrease this activity (Figure 5A and Figure S4C–E). In agreement with the absence of (statistically significant) sequelogs of mouse Ntaq1 in the mouse genome, the effect of Ntaq1-specific RNAi on the activity of NtQ-amidase and a similar but even stronger effect of depleting Ntaq1 with anti-Ntaq1 antibody (Figure 5A and Figure S4) suggested (but did not prove) that Ntaq1 is the sole NtQ-amidase in the mouse.
The NtQ-amidase assay (Figure 1B) was applied to C-terminally His6-tagged, purified mouse Ntaq1 (Ntaq1H6) that was expressed in the yeast P. pastoris (Figure 2E). The results confirmed the Gln-specific NtQ-amidase activity of Ntaq1 (Figure 5B), and also indicated that Ntaq1 could be inhibited by thiol-specific reagents such as iodoacetamide or N-ethylmaleimide (data not shown). To address the properties of Ntaq1 in yet another way, X-(LTKCEV)-DHFRbt reporters (X = Q; N; E; MQ; GQ; EQ) were incubated with purified mouse Ntaq1H6, followed by N-terminal sequencing of the resulting proteins by Edman degradation. Gln-((LTKCEV)-DHFRbt became Glu-(LTKCEV)-DHFRbt after incubation with Ntaq1, whereas Asn-(LTKCEV)-DHFRbt, Glu-(LTKCEV)-DHFRbt, Met-Gln-(LTKCEV)-DHFRbt, Gly-Gln-(LTKCEV)-DHFRbt, and Glu-Gln-(LTKCEV)-DHFRbt remained unchanged (Figure 3F). These experiments directly demonstrated that Ntaq1 is an NtQ-amidase, and also showed that Gln at position 2 was not a substrate of Ntaq1, confirming its high specificity for N-terminal Gln (Figure 5C).
At this stage of the project, we developed an entirely different NtQ-amidase assay, which utilized purified Ntaq1 and 7-residue synthetic peptides XY-GSGAW (XY = QH; QK; QL; QD; QY; QP; KQ; YH; NH; Ac-QH) as reporters (Figure 4B, C). In this “Q-peptide” assay, deamidation of, for example, Gln-HGSGAW was measured by quantifying the production of ammonia (NH3). It was detected through the presence of NADH-dependent glutamate dehydrogenase (Figure 4B). The consumption of NADH, monitored through a decrease of A340, was used to measure the formation of ammonia and thus the activity of purified NtQ-amidase. In agreement with the inferred specificity of Ntaq1 for the unmodified N-terminal Gln of a polypeptide, the Q-peptide assay showed that Ntaq1 could not deamidate acetylated N-terminal Gln, and was also inactive toward non-Gln N-terminal residues (Figure 4C). With the sole exception of proline, all tested second-position residues did not influence the activity of Ntaq1 by more than 2-fold (Figure 4C). In contrast, a Pro at position 2, in the QPGSGAW peptide, virtually abolished deamidation of N-terminal Gln (Figure 4C), a potential clue to stereochemistry and mechanism of NtQ-amidase.
Strong sequelogs of the mouse, human and bovine Ntaq1 NtQ-amidases are present throughout the animal kingdom (including fishes, insects and nematodes), in plants (including Arabidopsis thaliana), and in some fungi, such as the fission yeast Schizosaccharomyces pombe, but not in the budding yeast S. cerevisiae (Figure S5). (S. cerevisiae contains the Nta1 NtN,Q-amidase (Figure S1).) Although Ntaq1 of the present work and the previously characterized Ntan1 (Kwon et al., 2000) catalyze analogous reactions (Figure 1A), there is no statistically significant sequelogy among Ntaq1, Ntan1 and Nta1. This remarkable lack of sequelogy suggests independent origins of these Nt-amidases, presumably late in evolution of the N-end pathway, after the emergence of its arginylation branch (Figure 1A). In contrast to Nt-amidases, there is a sequelogy between eukaryotic Ate1 R-transferases (Figure 1A) and prokaryotic Bpt L-transferases (Graciet et al., 2006), suggesting that beginnings of the N-end rule’s arginylation branch predate the emergence of eukaryotes.
While preparing this study for publication we came across a recent entry in the Protein Data Bank (PDB #3C9Q; target name: BC008781) (Bitto et al., 2008). This entry, a part of “high-throughput” crystallographic studies by the Center for Eukaryotic Structural Genomics, described the crystal structure of the otherwise uncharacterized C8orf32 human protein (Figure 6A). As shown by our findings (Figure 2–Figure 5, Figure S2–S4, and discussion above), the mouse Ntaq1 NtQ-amidase is the counterpart of human C8orf32. Consequently, C8orf32 will now be called Ntaq1. The 1.5 Å structure of human Ntaq1 (C8orf32), solved with a bound peptide-like compound with a well-resolved N-terminal tripeptide Ser-Thr/Val-Ala (Bitto et al., 2008), is a monomeric globular protein of a novel structural fold, with an α-β-α three-layer sandwich architecture (Figure 6A). The residues Cys28, His81 and Asp97 (they correspond to Cys30, His83 and Asp99 in mouse Ntaq1) are highly conserved among Ntaq1 proteins of different organisms (Figure S4) and are spatially proximal in the crystal structure of human Ntaq1 (Figure 6C), in a region that resembles an active site, in proximity to the bound peptide-like compound (Bitto et al., 2008).
Guided by Ntaq1 sequence alignments (Figure S5) and the crystal structure of human Ntaq1 (Figure 6A), we used site-directed mutagenesis and expression in the yeast P. pastoris to produce and purify 9 mutants of mouse Ntaq1, in addition to wild-type enzyme (Figure 2E and data not shown). The results of examining these mutants by the Q-peptide assay were in agreement with the inferred significance of Cys30 and His83 as key residues of the active site (Figure 4D). Specifically, Ntaq1C30A and Ntaq1H83A had no detectable NtQ-amidase activity, in contrast to wild-type or nearly wild-type levels of activity exhibited by mutants at other evolutionarily conserved positions, such as Ntaq1C23A, Ntaq1C28A, Ntaq1C-38A, Ntaq1E39Q, and Ntaq1H170A (Figure 4E). The Ntaq1D81N mutant was impaired but still active (Figure 4D).
An analogous Cys…His…Asp triad of spatially proximal residues mediates the catalysis by cysteine proteases (such as, for example, papain), and by transglutaminases as well. The latter enzymes catalyze an acyl transfer in which the γ-carboxamide group of an internal Gln residue in a polypeptide acts as the acyl donor, usually to the ε-amino group of a Lys residue, resulting in an isopeptide bond that crosslinks two polypeptides or different regions of the same polypeptide. There is no significant sequelogy between Ntaq1 NtQ-amidases (Figure S4) and other proteins, including cysteine proteases or transglutaminases. Remarkably, however, we found (using Entrez-3D and the VAST algorithm) that human Ntaq1 is spalogous (spatially similar) to mouse peptide N-glycanase (PDB 2F4M_A) in the region of the glucanase’s “transglutaminase core” domain. Given this result, we carried out a spatial alignment between Ntaq1 (Figure 5A) and Factor XIII transglutaminase (Figure 6B) (Pedersen et al., 1994). The inferred active site region of the human Ntaq1 NtQ-amidase was found to be a strikingly strong spalog of the active site of human transglutaminase factor XIII, despite the absence of sequelogy between these enzymes (Figure 6C; compare with Figure 6D).
In the catalysis of crosslinking by transglutaminases, the ε-amino group of a Lys residue attacks a (transiently) enzyme-linked Gln residue of a substrate polypeptide (Pedersen et al., 1994), but an attack by water is possible as well, leading, in such instances, to deamidation of Gln to Glu by a transglutaminase. To examine the “converse” possibility of NtQ-amidase exhibiting a transglutaminase activity, we employed a crosslinking assay with biotinylated cadaverin as a source of amino group (Dutton and Singer, 1975), a Gln-DHFR reporter, and purified mouse Ntaq1. No crosslinking of cadaverin to Gln-DHFR by Ntaq1 was observed (data not shown), suggesting (but not proving, given the logic of negative evidence) that NtQ-amidase is devoid of transglutaminase activity. This tentative conclusion is also consistent with the absence of sequelogy between NtQ-amidases and transglutaminases. Taken together, our results with site-directed mutants of NtQ-amidase (Figure 4D), the obvious spalogy (but no sequelogy) between the active sites of NtQ-amidase and transglutaminases (Figure 6C, D), and the resulting Cys…His…Asp catalytic triade of NtQ-amidase lead us to propose the verifiable conjecture that deamidation of N-terminal Gln by the Ntaq1 NtQ-amidase employs a transglutaminase-like catalytic mechanism.
Progress in biological research, including “high-throughput” structural studies, has produced a disposition all but improbable a decade ago: the Ntaq1 NtQ-amidase, a previously undescribed enzyme, finds itself surrounded by directly relevant genomic, proteomic and even crystallographic evidence. These earlier data have become unified and informed in the present work by the revealed enzymatic identity of Ntaq1, its mechanistic similarity to transglutaminases, and its place in the N-end rule pathway. Before the present study, the Ntaq1 gene was called Cg8253 in Drosophila melanogaster, Wdyhv1 in mice and C8orf32 in humans (Figure 2D and Figure S5). Some of the vistas opened up by our findings about the Ntaq1 NtQ-amidase stem from earlier data, such as, for example, the detection of putative protein ligands of human C8orf32 (Ntaq1) ((Lim et al., 2006) and refs. therein), which remain to be explored.
A mutant, termed tungus, in Drosophila Cg8253 (Ntaq1) that encodes the fly counterpart of mouse NtQ-amidase, has defective long-term memory ((Dubnau et al., 2003); see also FlyBase FBrf0188553). This finding is consistent with the previously demonstrated major role of the N-end rule pathway in mouse brain development (An et al., 2006), with some of the putative ligands of human C8orf32 (Ntaq1) being relevant to neurodegeneration syndromes (Lim et al., 2006), with regulation of the nematode (C. elegans) counterpart of mouse Ntaq1 by neuron-specific transcription factors (NCBI>GEO>Series GSE9665), and with an involvement of human C8orf32 (Ntaq1) in regulation of genes containing cAMP-response elements (Tian et al., 2007).
Deamidation of N-terminal Gln by NtQ-amidase (Figure 1A) is mutually exclusive with the formation of N-terminal pyroglutamate. The latter reaction is catalyzed by glutaminyl cyclase (Schilling et al., 2008). NtQ-amidase is present in the cytosol and the nucleus (Figure S3C–H), as is the rest of the N-end rule pathway, whereas glutaminyl cyclase is in the secretory compartment, including the endoplasmic reticulum (ER). However, given complexities of traffic between intracellular compartments (including retrotranslocation of proteins from the ER to the cytosol), the extent of in vivo “competition” between NtQ-amidase and glutaminyl cyclase, i.e., the extent of overlap between the sets of their physiological substrates, remains to be determined.
Despite their multiplicity and broad range, the discovered functions of the N-end rule pathway (see Introduction) are still the tip of the iceberg. The known physiological substrates of this pathway (Hwang et al., 2009; Varshavsky, 2008a) are the beginning of a longer list that may require new methods for its systematic elucidation. Given their distinct N-terminal residues, Asn versus Gln, the sets of physiological substrates of NtN-amidase (Ntan1) and NtQ-amidase (Ntaq1) most likely do not overlap. Therefore it is not possible to predict, at present, whether Ntaq1−/− mice will be viable as adults, similarly to Ntan1−/− mice (Kwon et al., 2000), or whether they will be embryonic lethals, similarly to Ate1−/− mice, which lack N-terminal arginylation, a step downstream of N-terminal deamidation (Figure 1A) (Kwon et al., 2002).
The subunit selectivity of processive proteolysis, first discovered in the context of the N-end rule pathway (Johnson et al., 1990), underlies most functions of the Ub system, as it allows protein remodeling through subunit-specific degradation. A cleaved subunit whose C-terminal fragment bears a destabilizing N-terminal residue (Figure 1A) would be a potential substrate for selective proteolytic removal from a protein complex, thus making possible its remodeling (Johnson et al., 1990; Prakash et al., 2009). Because the N-end rule pathway can target either N-degrons or internal (non-N-terminal) degrons (see Introduction), this remodeling can involve not only cleaved but also intact subunits of a protein complex. Previous work indicated that one function of the N-end rule pathway is to operate, in such contexts, as a device that employs its capacity for subunit-specific proteolysis to reset the states of relevant circuits. Examples include the degradation of a separase-produced fragment of a cohesin subunit, a step that has been shown to be required for the high fidelity of chromosome segregation (Rao et al., 2001; Varshavsky, 2008a). Another likely example is the degradation of the yeast Mgt1 DNA alkylguanine transferase (Hwang et al., 2009). Recent studies (Huang et al., 2006) suggested that a circuit-resetting function of the N-end rule pathway may involve the Ntaq1-dependent degradation of a fragment of the USP1 deubiquitylating enzyme, whose substrates include ubiquitylated PCNA, the DNA replication processivity factor. Conditional self-cleavage of human USP1 produces a C-terminal fragment of USP1 that bears N-terminal Gln. This fragment is apparently short-lived in vivo (Huang et al., 2006), and may be an N-end rule substrate targeted for degradation by the Ntaq1 NtQ-amidase. A verification of this conjecture should be possible through the use of Ntaq1−/− mouse strains. Their construction is under way.
For a detailed description of Experimental Procedures, see Supplemental Data.
In the reporter proteins His10-Ub-XLTKCEV-DHFRbt (see the legend to Figure 1B), X was a 1-, 2-or 3-residue sequence (X = Q; E; N; EQ; MQ; GQ; REQ)
This assay was based on coupling the deamidation of N-terminal Gln to the arginylation, by purified R-transferase, of the resulting N-terminal Glu residue (Figure 1A) in the presence of radiolabeled Arg. The assay is outlined in Figure 1B and described in Supplemental Data.
This assay, which employed purified NtQ-amidase and 7-residue peptides XZ-GSGAW (XZ = QH; QK; QL; QD; QY; QP; KQ; YH; NH; Ac-QH), measured deamidation-produced ammonia using NADH-dependent glutamate dehydrogenase, as described in Supplemental Data.
NtQ-amidase was purified from calf brains through steps that included ion exchange, hydrophobic and gel filtration chromatography (Figure 1C, Figure 2C, Figure S2 and S3A, B). Mass spectrometry (MS-MS) identified a partially purified bovine NtQ-amidase as the counterpart of a previously uncharacterized protein encoded by human C8orf32. See Supplemental Data for details.
C-terminally FLAG-tagged mouse Ntaq1 NtQ-amidase (Ntaq1f) and other proteins were expressed in S. cerevisiae from the high-copy vector p425MET25 (Table S1)
ORFs encoding C-terminally His6-tagged mouse Ntaq1 NtQ-amidase (Ntaq1H6) and its missense mutants were subcloned into pPICZα-C (Table S1) and expressed in the yeast P. pastoris, followed by purification of overexpressed proteins by Ni-affinity chromatography.
Assays for βgal activity (Baker and Varshavsky, 1995) were performed with extracts from WHQ8 (nta1Δ) S. cerevisiae carrying pUB23-X plasmids (X = Met, Asp, Asn, Glu, or Gln) that expressed Ub-X-βgal reporters.
Alterations of specific residues in mouse Ntaq1 were carried out using two-step PCR and pPICZα-mNtaq1-mNtaq1 (Table S1).
Purified XLTKCEV-DHFRbt proteins (X = MQ; EQ; GQ; E; Q; N) were incubated with purified mouse Ntaq1 NtQ-amidase, followed by SDS-PAGE and N-terminal sequencing of test proteins by Edman degradation
A fusion between mouse Ntaq1 and EGFP was constructed in the pEGFP-N1 vector (Clontech) and examined with NIH-3T3 mouse cells as described in the main text.
A rabbit antibody to Ntaq1 was produced using mouse Ntaq1H6 (see above) purified from P. pastoris. The antibody was affinity-purified using immobilized Ntaq1H6, and was thereafter employed (vis-a-vis preimmune serum) to deplete the Ntaq1 NtQ-amidase from extracts of NIH-3T3 cells (Figure 5A, Figure S4C–E, and Supplemental Data). RNAi procedures for down-regulation of the expression of endogenous Ntaq1 in mouse NIH-3T3 cells using pre-microRNAs (pre-miRNAs) (Figure S4A, B) are described in Supplemental Data.
We thank current and former members of the Varshavsky laboratory for their advice and help, particularly R.-G. (Cory) Hu and Z. Xia for the plasmids pWHQ91 and pH10UE. We are grateful to J. Zhou and E. A. Wall (California Institute of Technology) for assistance with Ntaq1 mass spectrometry and genetic analysis, respectively, and to B. Stanley and A. Stanley (Pennsylvania State University, Hershey, PA) for N-terminal sequencing of reporter proteins. This study was supported by grants to A. V. from the National Institutes of Health (GM31530, GM85371, DK39520) and the American Asthma Foundation.
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