5Genetics Group and 6Enzymology Group, Biotechnology Research Institute, National Research Council of Canada, Montreal H4P 2R2, Canada, and 7Department of Biology and 8Department Anatomy and Cell Biology, McGill University, Montreal H3A 2B2, Canada
Received on January 14, 2000; revised on February 24, 2000; accepted on February 24, 2000.
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Abstract |
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Key words: calnexin cycle/ER quality control apparatus/glycan processing/N-linked glycosylation
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Introduction |
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Inhibitors of the ER -glucosidases have been useful in elucidating the effects of glycan processing on the maturation of secretory and membrane glycoproteins (Ou et al., 1992
; Kearse et al., 1994
; Balow et al., 1995
; Hebert et al., 1995
; Ora and Helenius, 1995
; Flura et al., 1997
). While not all glycoproteins have been shown to interact with calnexin/calreticulin, impaired association with these lectins can lead to minor structural changes and loss of function, or ultimately to retro-translocation through the translocon and degradation in the cytosol by the ubiquitin-proteasome pathway (Brodsky and McCracker, 1997
; Kopito, 1997
; Sommer and Wolf, 1997
). In earlier studies with cultured cells (Karpas et al., 1988
; Taylor et al., 1988
; Block et al., 1994
; Fischer et al., 1995
; Zitzmann et al., 1999
), and more recently with animal model systems (Block et al., 1998
; Mehta et al., 1998
),
-glucosidase inhibitors have shown also to inhibit viral propagation by blocking viral envelope glycoprotein-ER lectin associations (Elbein, 1991
; Mehta et al., 1998
).
Glucosidase II has been described both biochemically and genetically as a heterodimer with the subunit displaying sequence homology with the glycoside hydrolase Family 31 (Trombetta et al., 1996
; Arendt and Ostergaard, 1997
; Hentges and Bause, 1997
; D'Alessio et al., 1999
). The
subunit contains the catalytic domain, which is characterized by the consensus sequence (G/F)-(L/I/V/M)-W-X-D-M-N-E (Henrissat and Bairoch, 1993
), while the ß subunit is presumably involved in ER localization through its C-terminal HDEL sequence. Although mostly localized to the ER, Brada et al. (1990)
found glucosidase II in endocytic structures beneath the plasma membrane as well as associated with vacuoles in kidney brush border cells. These authors were the first to postulate that there might be two forms of the enzyme. Recently, Arendt and Ostergaard (1997)
found glucosidase II associated with CD45, a transmembrane protein-tyrosine phosphatase (PTP) in SAKR mouse T-lymphocyte cell line. In the same study, they cloned a cDNA for the
subunit that encodes an additional 22 amino acids stretch not found in the available human sequence (GenBank accession number D42041). More recently, the same authors reported the existence of several isoforms of the murine
subunit originating from alternative splicing (Arendt et al., 1999
). It was suggested that these isoforms differ in their activity, regulation, and possibly in their proteinprotein interactions (Arendt et al., 1999
).
The ß subunit of glucosidase II was originally identified as the protein kinase C substrate 80 K-H (Hirai and Shimizu, 1990). It is characterized by its own ER signal sequence, EF-hand high-affinity calcium binding loops, two glutamic acid repeats in tandem and a putative ER retention motif HDEL (Arendt and Ostergaard, 1997
; Arendt et al., 1999
; Trombetta et al., 1996
). Work by Trombetta et al. (1996)
has shown that the
and ß subunits copurify while attempts to separate the
and ß chains under conditions that preserve enzymatic activity were unsuccessful. Alternatively, however, Flura et al. (1997)
observed a variable increase in glucosidase II activity when they expressed a pig liver cDNA encoding the
subunit alone in CHO cells. Furthermore, Hentges and Bause (1997)
had pig liver glucosidase II preparations both with and without a detectable 60 kDa component. Thus the requirement of the ß subunit and the functional nature of the heterodimeric glucosidase II complex remained to be established.
The current kinetic model for p-nitrophenyl -D-glucopyranosidase (p-NP-Glcase) and maltase activities of glucosidase II, proposed by Alonso et al. (1991)
, 1993b), suggests the existence of both high and low affinity substrate binding sites. This model was supported by the earlier work of Hubbard and Robbins (1979)
, which reported different rates of glucose hydrolysis from N-linked Glc2- versus Glc1Man9GlcNAc2 oligosaccharides. Moreover, bromoconduritol has been shown to only inhibit the hydrolysis of the Glc1 form of the oligosaccharide (Datema et al., 1982
; Alonso et al., 1993a
). There are two possible explanations for this model, the first being based on the proposed two substrate binding sites. However, with the discovery of
subunit splice variants, the possibility that these activities are properties of distinct isoforms is raised. Previous results could be due to heterogeneous enzyme preparations which are responsible for the differential activities. We can now test this hypothesis with genetically purified isoforms of glucosidase II.
We report here the isolation of human cDNAs encoding for the 1 (short form),
2 (long form), and ß subunits of glucosidase II. A role of the ß subunit was sought through expression in COS7 cells, while a heterologous expression system was developed to perform a detailed comparison of the recombinant
1/ß and
2/ß isoforms, based on their kinetic parameters for the p-nitrophenyl
-D-glucopyranoside substrate, and their substrate specificities for the physiological oligosaccharides.
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Results |
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Based on the human 80K-H cDNA sequence (GenBank J03075), the cDNA encoding the ß subunit was amplified from human lymphocyte mRNA. The amplified DNA fragment was identical to the published sequence except for an additional glutamic acid at position 314 (AF144075). Ophoff et al. (1996) have shown five polymorphisms for this gene, one of which results from altering the simple trinucleotide repeat length (GAG) encoding glutamic acid stretches. The observed alleles of (GAG)n varied from n = 8 to n =11. The cDNA isolated has 10 GAG repeats (n = 10).
1 and
2 isoforms originate from a single gene
The 66 nucleotide insertion found in the 2 isoform provides an additional XmnI restriction site. Thus a 220 bp XmnI/BamHI fragment from the human
2 cDNA was used to probe XmnI/BamHI digested genomic DNA, isolated from human lymphocytes or mouse ES cells. If more than one gene had been responsible for the isoforms of this enzyme, a BamHI/XmnI double digestion would have resulted in at least two bands: a higher molecular weight band for the short form and a lower one for the long form. Since only one band could be detected (data not shown), we conclude that both isoforms originate from a single gene. Alternative splicing of the mRNA is probably responsible for the expression of the isoforms of the
subunit.
Two /ß complexes of human glucosidase II are expressed in vivo
Western blot analysis was performed to study differential expression of and ß subunits in various human cell lines. Although the longer
subunit was expressed at lower levels, both isoforms were present in all human cell lines tested (Figure 1A) except for Peer T-cells. PHAR2.7, a mouse glucosidase II deficient cell line was shown to be completely devoid of
subunit whereas only one form of
subunit could be detected in its parental BW5147 cell line. The ß subunit was present in all cell lines tested, even in the glucosidase II deficient cell line PHAR2.7, where it appears as an abundant protein of ~80 kDa (Figure 1B).
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Expression of glucosidase II ß subunit promotes expression of soluble subunit, and yields enzymatically active glucosidase II
Glucosidase II and ß subunits were transiently transfected individually or together in COS7 cells. Endogenous glucosidase II subunits were visible in the Triton X-100 soluble fraction but barely detectable in the pellet fraction (Figure 2, lane 1). However, when
1 or
2 subunits were overexpressed (Figure 2A lanes 2, 5; Figure 2B, lanes 3, 5), there was a slight increase in the levels of soluble protein but most of the expressed
subunit was found in the Triton X-100 pellet. Overexpressed ß subunit (Figure 2A, lane 3) was generally soluble when expressed alone, but traces of insoluble material (pellet) were detected. Co-expression of the ß subunit with any of the
subunits (Figure 2A, lanes 4, 6; Figure 2B, lanes 2, 4, 6) significantly reduced the extent of the insoluble
subunits but did not significantly increase the total amount of soluble
subunit.
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The ß subunit HDEL-ER retrieval motif is responsible for the localization of the heterodimeric glucosidase II
The ß subunit of glucosidase II contains a C-terminal HDEL putative ER retrieval motif. We replaced this amino acid sequence with a (His)6-tag and transfected COS7 cells with an increasing amount of each ß subunit, together with a constant level of 1 subunit of glucosidase II. From these cells, but not in the control cells, glucosidase II could be detected extracellularly by immunoprecipitation and by p-nitrophenyl
-D-glucopyranosidase (p-NP-Glcase) activity (Figure 4). Equal loading of the immunoprecipitations can be assessed by the band at 90 kDa which is the result of nonspecific protein G binding (Figure 4). This data confirms that the C-terminal HDEL/ER-retrieval motif of the ß subunits is required to prevent the secretion of the active enzyme into the extracellular space. Optimal activity was observed with 0.4 µg of ß subunit DNA, followed by a decline which may indicate deleterious effects of the overexpression of this subunit (data not shown).
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Next, either 1 or
2 subunits were simultaneously coexpressed with the ß subunit. This coexpression lead to a significant increase in soluble human recombinant
subunit (data not shown). In this case, only the
subunit was (His)6-tagged to allow for separation of the human recombinant glucosidase II from the endogenous insect enzyme. The first step of purification consisted of Ni2+-NTA chromatography. This separation was followed by anion exchange chromatography and contributed to a significant improvement in purification factor (Figure 6A) thus increasing the specific activity of recombinant glucosidase II (Figure 6B). The relative specific activity levels obtained for each isoform throughout purification correlated with the expression levels which were consistently higher for
1/ß than
2/ß (Figure 6B).
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Comparison of the kinetic parameters for p-nitrophenyl -D-glucopyranosidase activity for recombinant glucosidase II isoforms
Reaction rates of glucosidase II with the substrate p-NP-Glc did not obey the simple hyperbolic form of the Michaelis-Menten equation (Figure 7A), but can be described by a double hyperbolic form corresponding to a model that takes into account the two postulated binding sites (Figure 7B) (Alonso et al., 1991). This can also be clearly visualized using an Eadie-Hofstee plot (Figure 7C). These findings agreed with the results of Alonso et al., 1991
for rat liver glucosidase II activity on p-NP-Glc (1991) and for maltase activities (1993b). The KM1-2 values for both the high and low affinity sites were indistinguishable for both isoforms using the Students t-test (Table I). The observed KM1 for the high affinity sites of
1/ß and
2/ß were slightly lower at 0.50 and 0.52 mM, than for the KM1 of the high affinity site of the rat liver enzyme at 0.78 mM (Alonso et al., 1991
). They also approach the rat liver glucosidase II high affinity KM1 for maltose at 0.43 mM (Alonso et al., 1993b
). The KM2 for the low affinity sites of
1/ß and
2/ß were 61.2 and 68.5 mM, which are lower than the reported KM2 for rat liver glucosidase II for p-NP-Glc at 481 mM (Alonso et al., 1991
) but approaches, however, the KM2 for maltose, at 57.7 mM (Alonso et al., 1993b
).
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Inhibition of p-NP-Glcase activity
Inhibition at both the high and low affinity sites was tested for the two ranges of substrate concentration, 0.251.0 mM and 8.014 mM p-NP-Glc, respectively. Plots of reciprocal activity versus inhibitor concentration at these ranges suggested similar inhibition of p-NP-Glcase activity for both isoforms. We report here Ki1-2 values for deoxynojirimycin of 3.0 and 18.8 µM (1/ß), and 2.9 and 22.0 µM (
2/ß) for the high and low affinity sites respectively (Table I). Similarly with castanospermine we measured Ki1-2 values of 17.0 and 45.3 µM (
1/ß), and 15.0 and 39.8 µM (
2/ß) for the high/low affinity sites (Table I). These values were indistinguishable between isoforms demonstrating similar inhibition by deoxynojirimycin and castanospermine of p-NP-Glcase activity for both isoforms. It should be noted that neither
1/ß nor
2/ß were affected by EDTA nor EGTA at concentrations up to 10 mM (data not shown). Hence, recombinant glucosidase II activity was not affected by the depletion of cations, including calcium.
Glucose hydrolysis from Glc1-3Man9GlcNAc1 oligosaccharides by 1/ß and
2/ß forms of glucosidase II
Glucosidase II assays were performed for both 1/ß and
2/ß forms of recombinant enzyme after normalizing for p-NP-Glcase activity. [3H]-Mannose labeled lipid-linked Glc1-3Man9GlcNAc1 oligosaccharides were extracted, purified and pooled from S. cerevisiae
alg8
gls2,
alg10
gls2, and
gls2 mutants (Jakob et al., 1998
) and used as substrates. The extent of hydrolysis was determined by following changes in HPLC elution profiles (Figure 8). While the Glc3Man9GlcNAc1 oligosaccharide remained uncleaved after 30 min, glucose hydrolysis from both Glc2- and Glc1Man9GlcNAc1 was shown for both enzyme isoforms. Hydrolysis from the Glc2Man9GlcNAc1 was observed as a downward shift for the Glc2 peak with a concomitant rise in the Glc1 peak. Moreover, the rise in the Man9GlcNAc1 demonstrated the subsequent cleavage of the Glc1Man9GlcNAc1 oligosaccharides. The profiles for both forms of recombinant glucosidase II not only suggested that they share substrate specificities, but with similar vectorial changes in peak height confirm that they are catalytically indistinguishable for the substrates examined.
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Discussion |
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Different levels of expression have previously been observed for the subunit isoforms (Arendt et al., 1999
; Hentges and Bause, 1997
). Hentges and Bause (1997), in the purification of pig liver glucosidase II, found lower yields for the slower mobility form in their 107/112 kDa
subunit doublet. Also, cloning experiments by Arendt et al. (1999)
suggest a 5-fold lower expression of the form 1 (A1+ A2-) than form 3 (A1- A2-) using a PCR cloning strategy. We also found lower yields for
2 subunit, when expressed in COS7 cells (Figure 2) and Sf9 insect cells (Figure 7B). While factors that lead to differential expression of the
subunits remain unknown, protein complex stability may be ruled out since purified recombinant
1/ß and
2/ß display equal stability in continuous enzymatic assays, with linear progress curves proceeding for close to one h (data not shown).
These studies also sought to clarify the role of the ß subunit in the expression of active human glucosidase II in mammalian cells. Trombetta et al. (1996) first characterized glucosidase II as a heterodimer. They noted that the lower molecular weight subunit could not be removed while maintaining glucosidase II activity. More recently, D'Alessio et al. (1999)
genetically demonstrated the heterodimeric structure of Schizosaccharomyces pombe glucosidase II through the loss of endogenous glucosidase II activity in cells disrupted for GIIß. It was postulated in both studies that the ß subunit was involved in maintaining the integrity of catalytically active glucosidase II and the ER localization though its HDEL-ER retrieval signal. Flura et al. (1997)
on the other hand observed a slight increase in glucosidase II activity in CHO cells upon the lone expression of a pig liver derived cDNA encoding the
subunit. Moreover, while Hentges and Bause (1997)
identified a 60 kDa component, it was undetectable by Coomassie staining in some of their preparations. We found however that the
1 or
2 subunits were largely insoluble when expressed alone but this could be counteracted through the coexpression of the ß subunit, which concomitantly produced active glucosidase II. As well, we demonstrate here the requirement of heterodimeric structure for enzyme activity. Thus, the ß subunit contributes to the solubility/stability of the
/ß complex and is a prerequisite for the formation of the active enzyme. This rules out the hypothesis that the ß subunit is simply required for
subunit folding and that the
subunit then remains active upon dissociation. Moreover, the detection of active glucosidase II in the culture medium upon the replacement of the C-terminal HDEL sequon with a (His)6-tag, establishes a role of the ß subunit in retaining the
/ß glucosidase II dimer in the ER. It is possible however that the variable-fold increase in enzyme activity observed by Flura et al. (1997)
may be attributable to heterodimer assembly with endogenously expressed ß subunit. While abundantly expressed, the level of endogenous ß subunit does in fact vary according to cell line, as observed in our study (Figure 1B).
Heterologous expression of the subunit in Sf9 insect cells confirmed these functions of the ß subunit but also by the formation of active human/insect heteroenzymes remarkably demonstrates the wide conservation of its properties. While the yields of
subunit were high when expressed alone, most of the recombinant protein was insoluble. The small fraction of
subunit that was soluble always copurified with an insect protein with a molecular weight similar to that of the human ß subunit. Conversely, purified recombinant human ß subunit, when expressed alone, had an associated insect protein at ~110 kDa. These preparations also displayed p-NP-Glcase activity characteristic of glucosidase II. Protein alignments of the human ß subunit with homologues in Caenorhabditis elegans (Z47356) and S.pombe (D89245) suggest that it is a highly conserved protein. Both have putative ER targeting and retrieval signals, and overall homologies of 36% and 22%, respectively, particularly concentrated in the N-terminal region (Q50-E105). This region of high conservation, with 71% and 79% for C.elegans and S.pombe, respectively, may play a role in mediating
/ß interactions. Interestingly, the open reading frame YDR221w in S.cerevisiae (S59428) with an homology of 21% has both a putative ER targeting signal peptide and a transmembrane domain. Moreover, most of its homology is found within the conserved domain (61%). This open reading frame probably encodes a likely candidate for the glucosidase II ß subunit for this species. While it remains to be demonstrated, we propose that this highly conserved region acts as the major
/ß proteinprotein interaction domain.
One hypothesis for the existence of the 1and
2 forms was that they each may display different specificities for the Glc2Man9GlcNAc1 and Glc1Man9GlcNAc1 substrates. The current kinetic model for p-NP-Glc and maltose, which predicts both high and low affinity substrate binding sites (Alonso et al., 1991
) could have easily been derived from the copurification of two isoforms of glucosidase II with such substrate specificities. The first evidence of this differential activity was demonstrated by Hubbard and Robbins (1979)
. They showed that the sequential hydrolysis of glucose from the N-linked oligosaccharides occurred at different rates. Alonso et al. (1993a)
later assigned the cleavage of the innermost
-1,3-linked glucose (Glc1Man9GlcNAc2) to the low affinity site since bromoconduritol, which selectively inhibited both p-NP-Glc and maltose binding to this site, had also been shown to inhibit glucose hydrolysis from Glc1Man9GlcNAc2 (Datema et al., 1982
; Alonso et al., 1993a
). However, we have found, through the expression and purification of both recombinant
1/ß and
2/ß complexes of glucosidase II and through the determination of their kinetic parameters for the p-NP-Glc substrate, that both forms displayed activity that fit well to the two binding site model proposed by Alonso et al. (1991)
. Hence, the kinetics displayed are truly representative of an intricate active site and not the result of copurified isoforms with different substrate affinities. Furthermore, we have shown that the
1/ß and
2/ß forms of glucosidase II share similar properties of p-NP-Glcase hydrolysis and inhibition while exhibiting similar substrate specificities for the physiological oligosaccharide substrates.
A role for two or more isoforms of glucosidase II still remains to be determined. However, as an early step in glycan processing of nascent glycoproteins and the entry point into the calnexin cycle, glucosidase II is widely used by most, if not all secreted glycoproteins that may or may not require ER quality control. It is not without precedent to find biological complexity in such a pivotal step. And while glucosidase II was not found complexed with other ER constituents, transient interactions with the translocon, ER chaperones or even proteins of the ER matrix may exist that are isoform specific. Differential regulation cannot be ruled out and may be mediated by yet unknown interactions. While it remains to be determined, any new found complexity in the early steps of glycan trimming may provide us with novel and very specific antiviral strategies, as inhibitors of the ER -glucosidases have already shown great promise against viruses that require the host ER lectin-like chaperone protein folding apparatus (Zitzmann et al., 1999
).
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Materials and methods |
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Cell lines
RPMI8402 cells were obtained from Dr. C.Milstein (Cambridge, UK), Peer cell lines from Fujisaki Cell Center (Tokyo, Japan), mouse ES cells from Genome Systems Inc. (St. Louis, MO) and PHAR2.7 from Dr. I.Trowbridge (La Jolla, CA). All other cell lines were purchased from American Type Culture Collection (ATCC, Manassas, VA).
Cloning of human glucosidase II cDNAs
-Subunit. Rat glucosidase II was purified as described previously (Zapun et al., 1997
) electroblotted onto a PVDF membrane and the major 120 kDa protein was N-terminally sequenced by using an Applied Biosystems 470A protein sequencer equipped with an on-line phenylthiohydantoin amino acid analyzer. The N-terminal sequence was determined as VDRSNFKTCEESSFCKRQRS. A partial ORF sequence of human immature myeloid cell line KG1 (accession number D42041) displayed homology to the N-terminal amino acid sequence. mRNA was isolated from HeLa cells using the Quick Prep mRNA Purification Kit (Amersham Pharmarcia Biotech,) and cDNA amplified using the Marathon cDNA Amplification Kit (Clontech, Palo Alto, CA). Oligonucleotides 5' CAT GCT CAG GGA TCC CAT AGA CAT GCT (anti-sense) and 5' AAG CAT ACG GCC AGG CCT CTC TCC ATA CCG (sense) were used in conjunction with the adapter primer AP1 supplied with the kit (underlined nucleotides indicate BamHI and StuI restriction sites, respectively). PCR conditions were as described by the manufacturer (all PCR reactions were performed with a Perkin Elmer 9600 instrument). The amplicons of ~0.8 kb (doublet) and ~3.6 kb, respectively, were mixed and reamplified using AP2 primer and Expand Long Template PCR (Boehringer Mannheim Canada). The resulting ~3.9 kb fragment was digested with NotI and ligated in the mammalian expression vector pcDNA3 (Invitrogen, San Diego, CA). The EcoRV/HindIII fragment of the polylinker was deleted to remove a hairpin structure to enhance translation and protein production. Full-length cDNAs for human glucosidase II were sequenced. The point-mutated
subunit was generated using the primer pairs 5' GTC TGG AAT AAC ATG AAC GAA CC (sense) (boldface indicates the mutated codon) / 5' GCT GAA GCT TAT CGC AGG TGA ATA CTC CAA TC (anti-sense) and 5'-GGT TCG TTC ATG TTA TTC CAG AC (anti-sense) (bold face indicates the mutated codon) / 5'-AAG CAT ACG GCC AGG CCT CTC TCC ATA CCG (sense) (underlined nucleotides indicate a StuI restriction site). The fragments obtained were purified and reamplified using the flanking primers 5' GCT GAA GCT TAT CGC AGG TGA ATA CTC CAA TC (anti-sense) and 5'-AAG CAT ACG GCC AGG CCT CTC TCC ATA CCG (sense). An AatII/KpnI fragment (901 bp) was replaced in the original full-length clones and resequenced. The final 3.9 kb amplicon contains original 5' and 3' untranslated regions.
ß-Subunit.
The ß subunit of human glucosidase II sequence was previously identified (GenBank accession #J03075) (Tabaczewski and Stroynowski, 1994; Trombetta et al., 1996
). This gene was amplified using normal human lymphocytes mRNA as template. cDNA was obtained using the TITAN RT-PCR kit (Boehringer Mannheim) using oligos 5' GCT CGA GAA TTC GGT GAG ATG CTG TTG CCG CTG (sense) (underlined nucleotides indicate the EcoRI restriction site used for cloning) and 5' CGC GGT CTA GAT TAC TAG AGC TCG TCA TGG TCG TCT TC (anti-sense) (underlined nucleotides indicate the XbaI restriction site used for cloning). The 1.6 kb amplicon obtained was digested with EcoRI/XbaI and cloned in pcDNA3. Both DNA strands were sequenced. A 135 bp NcoI/XbaI fragment of sequence encoding the C-terminal HDEL was removed and replaced by a mutagenic PCR fragment amplified with the primer 5' CG CGG TCT AGA TTA CTA ATG GTG ATG GTG ATG ATG GTC GTC TTC GGT GGG TGC (anti-sense) (underlined nucleotides indicate the XbaI restriction site used for cloning, and bold represents the (His)6-tag) and 5' GTC CGA GAA TTC GGT GAG ATG CTG TTG CCG CTG (sense).
Southern blot analysis of glucosidase II
Human lymphocyte or mouse ES cell genomic DNA (10µg) was digested overnight at 37°C with 100U of BamHI and/or XmnI, separated on a 0.7% agarose gel and transferred to Hybond N+ membrane (Amersham Pharmacia Biotech). Blotted DNA was probed with a [32p]-labeled XmnI/BamHI cDNA fragment (220 bp). The blot was washed twice in 2x SSC, 0.1% SDS at 65°C for 30 min and exposed with Kodak XAR-5 film.
Transfections
COS7 African green monkey kidney cells were cultured in D-10 (DMEM supplemented with 10% FBS inactivated at 56 °C for 30 min). Cell monolayers at 40% confluency were transfected with 9.5 µg DNA and 40 µl lipofectamine in 100 mm plates or 1.2 µg DNA and 5 µl lipofectamine in 35 mm plates in Opti-MEM I and incubated for 16 h. Medium was replaced with fresh D-10 medium and cells were collected 24 h later. Large-scale cotransfections were performed with 4 µg pcDNA3 and 4 µg subunit, with 4 µg pcDNA3 and 4 µg ß subunit, or with 4 µg
and 4 µg ß subunit. Small-scale transfections were performed with combinations of DNA as described in Figure 8. Transfections included either 1.5 µg (large-scale) or 0.2 µg (small-scale) of the vector pQBI25 (Quantum Biotechnologies Inc., Montreal, Quebec) coding for the Green Fluorescent Protein in order to evaluate transfection efficiency.
Mammalian cell lysate preparation
Cells were scraped and washed three times in D-PBS. They were then lysed on ice for 20 min in 10 mM TrisHCl pH 6.8, 300 mM NaCl, 2 mM CaCl2 and 1% Triton X-100 supplemented with CompleteTM EDTA-free Protease Inhibitors (Boehringer Mannheim). Samples were homogenized using a Potter Elvejheim for 30 s on ice. The lysates were diluted 10-fold (0.1% Triton X-100, final concentration) and cleared by centrifugation at 13000 x g for 5 min. The supernatant was collected and protein concentration measured using the Bio-Rad Protein Assay (Bio-Rad, Hercules, CA).
Glucosidase II Assays on N-linked [3H]Glc1Man9GlcNAc2
Acid phosphatase (AcP) was purified from Saccharomyces cerevisiae (DT111 strain that secretes glycoproteins with asparagine-linked Man9GlcNAc2 glycans) and glucosylated in vitro with recombinant rat liver UDP-glucose glycoprotein:glucosyltransferase (UGGT) (Tessier et al., 2000). Briefly, 10 µg of purified Man9GlcNAc2-acid phosphatase (G0-AcP) in 20mM TrisHCl pH 7.5, 10 mM CaCl2 was labeled with 50 µCi UDP-[3H]glucose (30 Ci/mmol, Amersham Pharmacia Biotech) using 100 nM of purified recombinant UGGT for 4 h at 37°C. Unincorporated UDP-[3H]glucose was removed using G-50 Sepharose spin columns (Amersham Pharmacia Biotech). Typical labeling obtained was 24 x 105 c.p.m./µg AcP. Cell lysates adjusted to a protein concentration of 500 µg/ml were incubated at 37 °C with 5 x 105 c.p.m. [3H]Glc1-AcP/ml, with or without 100 µM or 500 µM DNJ. Aliquots were removed every 15 min and immediately diluted in 3x SDS sample buffer with DTT (New England Biolabs) and boiled for 5 min. Half of each of the sample was resolved on 8% SDSPAGE, followed by fluorography (Amersham Pharmacia Biotech). Dry gels were exposed with Kodak XAR-5 film for 60 h at 80°C. Films were scanned and image analyzed using the NIH Image Software (public domain).
Blue native-polyacrylamide gel electrophoresis
HeLa cell extracts were solubilized in 2% CHAPS, 1% Triton X-100, or 2% octyl-glucoside for 30 min on ice. Unsolubilized proteins were removed by centrifugation for 30 min at 100,000 x g. Samples were mixed with Serva blue and E-amino-caproic acid and separated on a linear 5 to 10 % acrylamide gradient as previously described (Schagger and von Jagow, 1991). Separated proteins were transferred to Immobilon-P membrane and detected by Western blot analysis.
In gel 4-methylumbellifyl -D-glucopyranosidase assay
Glucosidase II assays using the fluorescent substrate 4-methylumbelliferyl -D-glucopyranoside were performed as described elsewhere (Brada and Dubach, 1984
).
Antibodies
Map-peptide antibodies were raised in New Zealand rabbits. They correspond to amino acid sequence SFQHDPETSVLVLRK ( subunit) and DHDKSFAMKYEQGTG (ß subunit). The antisera also recognized the mouse glucosidase II homologue. Affinity-purified antibodies were prepared as described in The Xenopus Molecular Marker Resource (http://vize222.zo.utexas.edu) using the appropriate immobilized peptide Sepharose. Anti-ß antiserum was raised by injecting human ß subunit, electroeluted from SDSPAGE, into New Zealand rabbits. Mouse anti-human glucosidase II
/ß antiserum was raised by injecting BALB/c mouse with purified recombinant glucosidase II.
Western blot analysis
Protein samples were resolved on 8% SDSPAGE and transferred on Immobilon-P membrane (Millipore). The membranes were first probed with subunit anti-peptide antiserum or affinity-purified antibodies, incubated with anti-rabbit HRP (Bio-Rad or Santa-Cruz) and developed using Lumilight (for overexpressed proteins) or Lumilight Plus (endogenously expressed proteins) chemiluminescent substrate (Boehringer Mannheim). They were stripped according to the manufacturers instructions and reprobed with anti-ß subunit antibodies.
Immunoprecipitations
HeLa cells were labeled with [35S] methionine ([35S] Promix Protein Labeling Mix, Amersham Pharmacia Biotech), and immunoprecipitations were performed with either protein A (Figure 1B) or protein G Sepharose (Figure 4C) as described in Current Protocols in Immunology (Coligan et al., 1997) using rabbit anti-electroeluted ß subunit or mouse anti-glucosidase II
/ß.
Baculovirus production and protein expression
Human cDNAs encoding both 1 (D42041 with Y850H) and
2 subunits (AF144074) with (His)6-tags at the C-terminus and the ß subunit of glucosidase II, both with and without a (His)6-tag (AF144075) were subcloned into pFastBac1 and transformed into E.coli DH10Bac to produce recombinant bacmids. Sf9 cells were transfected with bacmid DNAs and the virus stocks amplified as described by the manufacturer (Gibco/Life Technologies). Cells were grown in Sf900 II SFM serum-free medium at 27°C for 3 days to a cell density of 1.52.5 x 106/ml and infected with either one or both virus for an
subunit and ß subunit virus at an M.O.I. of 25 pfu/cell. Only the ß subunit without a (His)6-tag was used in
/ß coinfections. Infected cells were incubated for 3 days, harvested by centrifugation at 3000 x g, and stored at 80 °C.
Recombinant glucosidase II purification
Infected cells (~7.5 x 108 ) were lysed in a Dounce homogenizer in 20 ml of Buffer A (250 mM NaCl, 20 mM TrisHCl pH 7.5) supplemented with 1% Triton X-100 and CompleteTM EDTA-free protease inhibitors (Boehringer Mannheim Canada). The homogenate was treated with bovine pancreas deoxyribonuclease I (Amersham Pharmacia Biotech) for 30 min on ice, and centrifuged at 10,000 x g for 10 min at 4°C. The supernatant was loaded by gravity flow onto a 1 ml Ni2+-NTA Superflow column (Qiagen Inc., Valencia, CA). 2x Buffer A with 1% Triton X-100 and 20 mM imidazole was added to the flow through and was loaded again onto the Ni2+-NTA column. The column was then washed with 50 ml of 2x Buffer A with 10 mM imidazole, followed by 4 ml each of 2x Buffer A with 25 mM imidazole, and 50 mM imidazole. Glucosidase II was then eluted in 5x 1ml fractions of 2x Buffer A with 200 mM imidazole. The eluate was desalted on a Sephadex G-25M column (PD-10; Amersham Pharmacia Biotech) in Buffer B (20 mM TrisHCl pH 7.5, 5 mM ß-mercaptoethanol).
Anion exchange chromatography
The desalted Ni2+-NTA fractions were loaded onto a Mono Q HR5/5 column (Amersham Pharmacia Biotech) equilibrated in Buffer B, on a BioCAD Perfusion Chromatography Workstation (PerSeptive BioSystems Inc., Framingham, MA). A linear gradient of 50 ml from 0 to 0.5 M NaCl in Buffer B was performed and the eluate collected in 1 ml fractions. The fractions were tested for activity and protein concentrations determined using a Bio-Rad Protein Assay (Bio-Rad, Hercules, CA). All fractions for each step of purification were analyzed by SDSPAGE and Western blot.
p-Nitrophenyl -D-glucopyranosidase assays and analysis of kinetic parameters
The activity for p-nitrophenyl -D-glucopyranosidase (p-NP-Glcase) was tested in a 100 µl reaction mixture consisting of 5 mM p-NP-Glc (Sigma) in 50 mM PIPES pH 6.5 for 30 min at 37°C. Assayed culture medium (COS7 cells) (Figure 4C) was precleared with activated charcoal (BDH, Ville St. Laurent, Canada) to remove traces of phenol red. The reactions were stopped with an equal volume of 1 M glycine/NaOH and the OD405 read immediately. One unit is the production of 1 µmol/minute of p-nitrophenol at 37°C. Progress curves were monitored for both isoforms by continuous assay (n = 5) for 30 min at 37°C in a SpectraMax 250 spectrophotometer (Molecular Devices Corp., Sunnyvale, CA). Continuous assay reactions were performed in 200 µl of 50 mM PIPES pH6.5 with a substrate concentration ranging from 0.1 to 14 mM p-NP-Glc. The slopes of the progress curves were determined by linear regression analysis using SoftMax Pro software version 1.1.1 (Molecular Devices, Corp), and kinetic parameters determined using ENZFITTER version 1.05 (Biosoft, Cambridge, UK). The two-binding site adaptations of the Michaelis-Menten and the Eadie-Hofstee equations described by Alonso et al. (1991)
were used to analyze the data.
p-Nitrophenyl -D-glucopyranosidase inhibition
Inhibition experiments were also performed by continuous measurement of p-NP-Glcase activity. Deoxynojirimycin (DNJ) and castanospermine (CST) (Calbiochem) were tested between 1.2510 µM and 2080 µM, respectively. The velocity was measured for the substrate concentration range of the high affinity site (0.251 mM) and the low affinity site (814 mM). Apparent Ki values were determined from plots of reciprocal activity versus inhibitor concentration.
Purification and glucosidase II hydrolysis of [3H]Glc1-3Man9GlcNAc1
Metabolic labeling with [3H]glucose and extraction of lipid-linked oligosaccharides was performed as described by Zufferey et al. (1995) from the following strains of Saccharomyces cerevisiae: YG424 (MATa, ade2-101, his3
200, lys2-801,
alg8::HIS3,
gls2::KanMX) (Jakob et al., 1998
); YG491 (MATa, ade2-101, his3
200,
alg10::KanMX,
gls2::KanMX) (Jakob et al., 1998
); SS328 (MAT
, ade2-101, his3
200, lys2-801, ura3-52) (Vijayraghavan et al., 1989
), to yield [3H]Glc1Man9GlcNAc2, [3H]Glc2Man9GlcNAc2, and [3H]Glc3Man9GlcNAc2, respectively. The oligosaccharides were quantified by liquid scintillation counting, pooled, and treated overnight with 5 x 103 units Endo H (New England Biolabs). Glucosidase II assays were performed with both purified recombinant isoforms with enzyme concentrations normalized for p-NP-Glcase activity. The reactions were in 840 µl with 210 µl of enzyme, 50 mM PIPES pH 6.5 and 2.0 x 104 c.p.m. of [3H]Glc13Man9GlcNAc2 pooled oligosaccharides. The time points used for the assays were 0, 15, 30, and 60 min, and the reactions were terminated by boiling for 2 min. Glucose hydrolysis from the oligosaccharides was monitored by HPLC as described by Romero and Herscovics (1986)
.
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Abbreviations |
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References |
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