- Research article
- Open Access
Detection of distinct glycosylation patterns on human γ-glutamyl transpeptidase 1 using antibody-lectin sandwich array (ALSA) technology
BMC Biotechnology volume 14, Article number: 101 (2014)
γ-Glutamyl transpeptidase 1 (GGT1) is an N-glycosylated membrane protein that catabolizes extracellular glutathione and other γ-glutamyl-containing substrates. In a variety of disease states, including tumor formation, the enzyme is shed from the surface of the cell and can be detected in serum. The structures of the N-glycans on human GGT1 (hGGT1) have been shown to be tissue-specific. Tumor-specific changes in the glycans have also been observed, suggesting that the N-glycans on hGGT1 would be an important biomarker for detecting tumors and monitoring their progression during treatment. However, the large quantities of purified protein required to fully characterize the carbohydrate content poses a significant challenge for biomarker development. Herein, we investigated a new antibody-lectin sandwich array (ALSA) platform to determine whether this microanalytical technique could be applied to the characterization of N-glycan content of hGGT1 in complex biological samples.
Our data show that hGGT1 can be isolated from detergent extracted membrane proteins by binding to the ALSA platform. Probing hGGT1 with lectins enables characterization of the N-glycans. We probed hGGT1 from normal human liver tissue, normal human kidney tissue, and hGGT1 expressed in the yeast Pichia pastoris. The lectin binding patterns obtained with the ALSA platform are consistent with the hGGT1 N-glycan composition obtained from previous large-scale hGGT1 N-glycan characterizations from these sources. We also validate the implementation of the Microcystis aeruginosa lectin, microvirin, in this platform and provide refined evidence for its efficacy in specifically recognizing high-mannose-type N-glycans, a class of carbohydrate modification that is distinctive of hGGT1 expressed by many tumors.
Using this microanalytical approach, we provide proof-of-concept for the implementation of ALSA in conducting high-throughput studies aimed at investigating disease-related changes in the glycosylation patterns on hGGT1 with the goal of enhancing clinical diagnoses and targeted treatment regimens.
γ-Glutamyl Transpeptidase 1 (GGT1), is a clinically important enzyme that has been studied for over 95 years. Expressed on the surfaces of a variety of ductal and glandular epithelial cells throughout the body, GGT1 is strategically localized to catalyze the cleavage of glutathione in circulating fluids, allowing for the recovery of its constituent amino acids ,. As such, GGT1 plays a key role in cysteine homeostasis . However, abnormal expression and localization patterns of GGT1 are common in several human malignancies, including liver, kidney, prostate, pancreatic, ovarian, colon, and lung cancers -. The induction of GGT1 expression has been shown to protect tumors against oxidative stress by initiating the recovery of amino acids from extracellular glutathione for its intracellular synthesis, conferring GGT1-positive tumors with enhanced resistance to alkylating agents and other classes of chemotherapeutic drugs -. While elevated serum levels of GGT1 associated with liver and pancreatic cancers have been used as a diagnostic marker for monitoring disease progression and response to clinical intervention, its utility as a pre-symptomatic cancer biomarker has been hampered by the fact that high serum GGT1 levels are also observed in non-malignant diseases, ranging from alcoholic hepatitis to myocardial infarction -. Thus, the potential of serum GGT1 as a diagnostic marker of tumor formation and progression has been discounted historically.
Human GGT1 (hGGT1, Swiss-Prot: P19440), is a type II membrane-bound glycoprotein composed of two asymmetric subunits, possessing seven potential N-glycosylation sites [sequon NX(S/T), X ≠ P], with six sites on the large subunit and a single site on the small subunit -. Using high-resolution mass spectrometry, we have previously shown that all seven of these asparagine residues are capable of being glycosylated when hGGT1 is expressed in normal human tissues and have demonstrated that the structure and composition of the N-glycans vary in a tissue-specific manner . While it has long been appreciated that the structural compositions of the N-glycans on hGGT1 change during malignant transformation, the large quantities of the tumor-derived glycoprotein required to characterize its carbohydrate content has posed a significant challenge for differential analyses -. Moreover, conventional methods, such as comparative lectin blotting or affinity chromatography coupled with mass spectrometry are labor-intensive and sample-exhaustive. Thus, the development of a more facile, high-throughput analytical method for reproducibly detecting differences in N-glycan content on small quantities of hGGT1 in complex biological samples would be of considerable benefit for investigative and diagnostic studies.
A promising emerging methodology for potentially addressing each of these intrinsic obstacles is antibody-lectin sandwich array (ALSA) technology . Adapting existing multiplexed protein technology, ALSA couples the immuno-capture of glycoproteins from biological samples, using target-specific antibodies, with the ability to interrogate the bound target with a variety of biotinylated probes. Thus, a diverse group of lectins or glycan binding antibodies can be used to simultaneously probe for a variety of carbohydrate moieties or glycoepitopes on a glycoprotein of interest with a very small amount of starting material. Unlike most large-scale approaches, this methodology introduces an objective quantitative component that enhances the interpretative value associated with the qualitative changes that it detects. The amount of fluorophore-labeled streptavidin bound by a specific biotinylated probe at each capture site is directly related to the prevalence of a particular glycan modification . Therefore, considerable compositional information can be gleaned from a single, small-scale sample preparation, a feature of ALSA which has been widely exploited for a diverse array of pathologies -.
In recent years, glycans have experienced a renaissance as potential biomarkers of cancer and other human pathologies -. A great deal of effort has been devoted to developing techniques for characterizing and cataloging changes in disease-related glycosylation patterns. Historically, however, methodological approaches that have exploited the use of glycan binding proteins  have required relatively large samples for conducting discriminatory comparisons, and as a result, primary screening using glycan binding proteins could exhaust all of a sample before the optimal discriminatory lectin is even identified . While the use of alternative complementary approaches, such as mass spectrometry, can provide finer structural resolution of glycosylation changes within individual samples, these techniques are not optimal for making simultaneous quantitative comparisons of glycan content between multiple sample pools, thus limiting their utility for primary biomarker screening . The recent advent of ALSA has attempted to address these inherent technical limitations.
In the current study, we investigated whether the microanalytical advantages of the ALSA platform could be applied to the differential characterization of hGGT1 purified from disparate sources and bearing distinct, pre-defined N-glycan content. We show that immuno-captured hGGT1, originating from microgram quantities of either normal human liver tissue, normal human kidney tissue, or from hGGT1 expressed in the yeast Pichia pastoris, exhibits distinct ALSA binding patterns that complement results obtained from previous large-scale hGGT1 N-glycan characterizations from these sources. We also demonstrate the first use of the Microcystis aeruginosa lectin, microvirin (MVN), in this type of screening assay and provide evidence for its utility in specifically recognizing high-mannose-type N-glycans on hGGT1, a modification which is apparently unique to hGGT1 isoforms expressed in malignant kidney and liver tissues ,. Hence, we provide proof of principle support for the implementation of ALSA in carrying out future high-throughput studies aimed at investigating changes in the glycosylation patterns on hGGT1 associated with human pathophysiological processes. We anticipate that this approach can be applied to developing primary diagnostic screening strategies and/or the development of a hGGT1 biomarker in studies evaluating therapeutic intervention.
Glycan microarray analysis to determine the fine carbohydrate binding specificity of microvirin
MVN has previously been shown to contain a single carbohydrate recognition domain (CRD) that can bind Manα(1–2)Man- linkages, the terminal disaccharide units on the arms of high-mannose-type N-linked oligosaccharides ,. To more precisely and comprehensively determine the ligand specificity of the CRD of MVN, biotinylated MVN (at concentrations of 2, 20, and 200 μg/mL) was subjected to high-throughput glycan array screening among 611 structurally-defined carbohydrates by Core H of the Consortium for Functional Glycomics (CFG) utilizing Version 5.0 of the printed glycan microarray (Figure 1). The highest affinity carbohydrates from the 200 μg/mL data set are rank-ordered in Table 1. Unambiguous positive binding of MVN occurred with ten glycans, each of which contained the Manα(1–2)Man- motif (Figures 1A and 2).
To discriminate between primary and secondary binding specificities, we applied Outlier Motif Analysis to the 200 μg/mL MVN CFG data set. This analytical tool has been described previously as a method for refining the inherent specification of binding determinants from complex data sets such as those compiled from CFG glycan arrays . From this analysis, MVN exhibited a clear demarcation between bound and unbound states (fluorescence threshold =2,319 RFU), with the Manα(1–2)Man- moiety serving as the common motif in all of the bound glycans (Figure 2A and B). Moreover, this motif was not present within any of the unbound constituents on the CFG glycan array. Other 2’ substituted mannose motifs, such as GlcNAcβ(1–2)Man-, a glycan well-represented within Version 5.0 of the CFG glycan array and a binding determinant for the Lens culinaris agglutinin (LCA) lectin, were not bound by MVN. Since the Manα(1–2)Man- motif adequately discriminated the bound versus unbound carbohydrates within the CFG data set for MVN, we then screened for motifs among the ten MVN-bound structures which might explain the varied binding within this group. Among the MVN-bound structures that contained a chitobiose core motif (GlcNAcβ - GlcNAc, i.e. bona fide N-glycans), the presence of an intervening Manα(1–2)Man linkage on the central arm of the N-glycan structure resulted in decreased MVN binding affinity (Figure 1B and Table 1). Strikingly, the two carbohydrate structures to which MVN bound with the highest- and lowest-affinity among the ten positive hits on the CFG glycan array varied by the absence or presence, respectively, of a single Manα(1–2)Man- substituent at this position (Figure 1B and Table 1). This observation may indicate that MVN exhibits preferential affinity for structural or rotational isomers with less restricted access to the Manα(1–2)Man- binding determinant (Figure 2B). This analysis validates the utility of MVN as a unique carbohydrate binding protein that specifically targets a structural motif that is present within the type of high-mannose N-glycans that are most commonly encountered in biological samples.
Characterization of human GGT1 expressed in Pichia pastoris as a potential substrate pool that is exclusively modified with high-mannose-type N-glycans
We previously showed that pools of hGGT1 purified from normal human kidney and liver tissue are each modified by a specific array of virtually non-overlapping complex-type N-glycans, with no high-mannose-type structures observed on hGGT1 glycopeptides originating from either of these tissues (Figure 3 and ). Indeed, high-mannose-type N-glycans on hGGT1 have only been observed in samples of diseased tissues from these organs ,. To evaluate the utility of our hGGT1 microanalytical system and the diagnostic efficacy of our biotinylated MVN-reagent in assessing disease status, we generated hGGT1 modified with high-mannose-type structures. Others have shown that Pichia pastoris N-glycosylates recombinant human proteins with high-mannose-type structures -, and we previously demonstrated that hGGT1 expressed in and purified from the yeast Pichia pastoris (Pp-hGGT1) is N-glycosylated and retains full enzymatic activity ,,. To investigate the N-glycan content of purified Pp-hGGT1, total N-glycans were enzymatically-released with the endoglycosidase PNGase F and profiled by MALDI-TOF/MS (Figure 4A). A family of ions were observed corresponding to predicted N-glycans that included Man8GlcNAc2 (4%), Man9GlcNAc2 (49%), Man10GlcNAc2 (37%), Man11GlcNAc2 (8%), and Man12GlcNAc2 (2%), consistent with findings from other recombinant human glycoproteins expressed in Pichia pastoris ,.
The distribution of N-glycans at different sites was addressed by LC-MS/MS profiling of tryptic glycopeptides, using diagnostic oxonium ions at m/z 163.0 and 204.1 to initially identify glycopeptide families, which elute as discrete chromatographic units . As an example (Figure 4B), the N-glycans on the LAFATMFNSSEQSQK (Asn-120) hGGT1 glycopeptide approximately correspond to the range of high-mannose-type compositions found in total Pp-hGGT1 (Figure 4A). Collision-induced dissociation MS/MS was carried out to confirm the structure models, as illustrated by fragmentation (Figure 4C) of the triply-charged glycopeptide bearing a Man11GlcNAc2 glycan (m/z = 1293.2) to yield a spectrum of triply-, doubly- and singly-charged ions, including the core GlcNAc-modified peptide (m/z = 946.5) (Figure 4C). Similar N-glycan microheterogeneity was observed at Asn344 and Asn511, of the large and small subunits, respectively (Table 2). These results support the use of Pp-hGGT1 as a pool of hGGT1 that is uniformly modified by high-mannose type N-glycans (Figure 3).
To evaluate whether purified Pp-hGGT1 is a high-affinity ligand of MVN, this pool was subjected to lectin and Western blot analyses using biotinylated MVN and an antibody specific for a peptide on the C-terminus of the large subunit of hGGT1. As shown in Figure 5, MVN and anti-hGGT1 similarly recognized the large subunit, which migrates broadly owing to microheterogeneity at the six N-glycosylation sites (Figure 5, lanes 1 and 3 and ). Enzymatic deglycosylation collapses Pp-hGGT1 into a sharper band, which is no longer recognized by MVN (Figure 5, lanes 2 and 4). These results demonstrate that MVN recognizes Pp-hGGT1 by virtue of its N-glycans.
Differential profiling of hGGT1 glycoepitopes by ALSA
We next investigated whether MVN and other lectins could be utilized in conjunction with ALSA technology to illuminate differences in carbohydrate content on the low quantities of hGGT1 present within complex biological samples. As depicted in Figure 6A, a previously-characterized polyclonal antibody (GGT129) that binds a C-terminal epitope in the large subunit of hGGT1 was immobilized and chemically-derivatized to prevent recognition by lectins or glycan-specific antibodies. The region containing the antibody epitope is not predicted to undergo post-translational modification .
We first asked whether the immobilized hGGT1 antibody was able to capture the hGGT1 that was produced by normal human kidney tissue, normal human liver tissue, and Pichia pastoris. As shown in Figure 6C, the immobilized antibody immuno-captured equivalent amounts of hGGT1 from each pool of activity-normalized hGGT1, indicating that the method was appropriate for comparative analyses. Furthermore, a two-fold dilution of hGGT1 typically resulted in reduced signal (Figure 7), suggesting that lectin binding was approximately proportional to hGGT1 levels. From this analysis, a detection limit of approximately 0.3 nanograms for Pichia pastoris-expressed hGGT1 was achieved. Based on activity normalization of the sample pools and their similar dilution profiles, this also provides an estimate for the detection limits achieved for the immuno-captured hGGT1 in the more complex kidney and liver extracts, as well (Figure 7).
The results from probing the captured hGGT1s with a variety of glycan binding proteins are depicted in Figure 6 (panels B and C) and summarized in Table 3. MVN bound only Pp-hGGT1, consistent with exclusive expression of high-mannose type N-glycans on hGGT1 from this source. Concanavalin A (ConA), which exhibits strong affinity for high-mannose type N-glycans, also bound only Pp-hGGT1 (Figure 7). ConA also has weak affinity for complex type N-glycans, which we would expect to be present on the liver- and kidney-derived hGGT1, but under the conditions of our assay, no binding was observed on hGGT1 in these sample pools. Galanthus nivalis lectin (GNL), which like ConA also has strong affinity for high-mannose type N-glycans and weak affinity for complex N-glycans ,, also bound only Pp-hGGT1 (Figure 7). The similar binding patterns observed for MVN, ConA, and GNL are consistent with the presence of high-mannose type N-glycans on Pp-hGGT1 but not on the kidney- or liver-derived hGGT1.
Euonymus europaeus lectin (EEL) binds α-linked galactose primarily in the context of blood group B [Galα1-3(Fucα1-2)GlcNAc], and more weakly to α1-2 linked fucose ,. As shown in Figure 7, EEL exhibited clear, concentration-dependent affinity for kidney-derived hGGT1. EEL also exhibited greater affinity for Pp-hGGT1 than liver-derived hGGT1 with increasing sample input (Figure 7). Griffonia simplicifolia Lectin 1(GSL-1) similarly binds terminal α-linked galactose but also α-linked GalNAc , and its affinity pattern for kidney- and liver-derived hGGT1 was similar to that measured for EEL at the higher sample dilution (Figure 7). However, unlike EEL, its affinity pattern for Pp-hGGT1 exceeded that observed for kidney-derived hGGT1 with increasing sample concentrations. ECL, which has specificity primarily for terminal Galβ1-4GlcNAc , exhibited high affinity for both Pp-hGGT1 and kidney-derived hGGT1 at both sample dilutions, although its apparent affinity for Pp-hGGT1 exceeded that for kidney hGGT1 on the array. Together, these results suggest the presence of terminal galactose, either α- or β-linked, on hGGT1 from kidney and Pichia pastoris. However, while we have demonstrated these glycan motifs on human kidney-derived hGGT1 (Figure 3 and ), we have no evidence that they are present on Pp-hGGT1, which is restricted to the production of high-mannose type carbohydrate motifs. Therefore, the affinity pattern of this particular subgroup of lectins for Pp-hGGT1 may arise from an inherent, yet cryptic, binding of high-mannose type N-glycans, a possibility that has recently been confirmed for EEL .
In marked contrast, Datura stramonium lectin (DSL) bound at saturating levels to kidney-derived hGGT1, weakly to liver-expressed hGGT1, and not at all to Pp-hGGT1 (Figures 6 and 7). The “hook effect” observed for DSL binding to kidney hGGT1, is commonly observed in immunoassays and other multivalent binding assays at saturating levels of the analyte . DSL has specificity for N-acetyl-lactosamine (LAcNAc, Galβ1-4GlcNAc), as typically found on extended N-glycans . This binding pattern is consistent with both the greater size and heterogeneity of complex type N-glycans which we identified on kidney-derived hGGT1 and demonstrated were not present on liver-derived hGGT1 or Pp-hGGT1 (Figures 3 and 4 and ).
Phaseolus vulgaris-Erythroagglutinin (Pha-E) specifically binds bisected N-linked glycans . As Pha-E exhibited weaker binding affinity overall, we used higher concentrations (i.e. reduced dilutions) of hGGT1 for these analyses (Figures 6C and 7). The detection of bisecting GlcNAc on kidney-derived hGGT1 is consistent with our previous mass spectrometric analysis of hGGT1 isolated from this tissue source (Figure 3 and ). This type of modification is restricted to complex type N-glycans. Thus, the lack of interaction between Pha-E and Pp-hGGT1 is consistent with the expected absence of complex type N-glycans (Figure 4). Moreover, our mass spectrometric analysis did not detect bisected N-glycans on hGGT1 expressed in normal human liver, lending further credibility to the specificity of the ALSA platform and the specificity of the lectin binding pattern (Figure 3 and ).
Lectin affinity blot validation of key source-specific differences in hGGT1 N-glycan content identified by ALSA microanalyses
ALSA analysis of hGGT1 expressed in Pichia pastoris and normal human kidney and liver revealed discriminatory lectin binding patterns that were consistent with documented differences in N-glycan content (Figure 3 and Table 3). To support these microanalytical findings, we investigated whether a subset of these binding patterns could be confirmed using the more time- and sample-exhaustive method associated with coupled immunoprecipitation and lectin blot analysis. Thus, hGGT1 was immunoprecipitated from activity-normalized aliquots of each class of hGGT1, and the bound fractions were subjected to SDS-PAGE and subsequent lectin blotting analysis with MVN, Pha-E, or DSL. ALSA analyses predicted that MVN would uniquely bind to Pichia pastoris-expressed hGGT1, while Pha-E would uniquely bind to kidney hGGT1 (Table 3). In the absence of a lectin that only bound liver hGGT1 in the ALSA platform, we used DSL, which exhibited high affinity for kidney-expressed hGGT1, modest affinity for liver-expressed hGGT1, and no apparent affinity for Pichia pastoris-expressed hGGT1 (Table 3).
As shown in Figure 8, western blot analysis against hGGT1 confirmed that equivalent amounts of the protein were immuno-captured from the three samples and revealed that Pp-hGGT1 exhibits greater microheterogeneity in its migration pattern relative to kidney- or liver-derived hGGT1 (Figure 8, top panel). Previous studies from our lab showed that all six of the N-glycosylation sites on the large subunit of hGGT1 are occupied on the kidney- and liver-expressed enzyme, while only five are fully occupied on Pp-hGGT1 -. Therefore, these distinct banding patterns may reflect differences in glycosylation site occupancy or N-glycan composition. The apparent non-specific bands in the hGGT1 blot are likely the dissociated heavy chain of the rabbit IgG used to immunoprecipitate hGGT1 being recognized by the HRP-conjugated anti-rabbit secondary antibody used to visualize the hGGT1. In the ALSA analyses, the antibody that is printed is chemically-modified to prevent interactions between it and lectin probes or secondary antibodies ,. MVN probing confirmed the ALSA data, showing specific recognition of Pp-hGGT1 (Figure 8, MVN panel, lane 1). Conversely, Pha-E exhibited strong, specific binding to kidney hGGT1 (Figure 8, Pha-E panel, lane 2), with no detectable binding to either Pichia pastoris- or liver-derived hGGT1 (Figure 8, Pha-E panel, lanes 1 and 3), again confirming the ALSA data. Lastly, DSL exhibited a strong binding preference for kidney hGGT1 and a modest interaction with liver hGGT1 (Figure 8, DSL panel, lanes 2 and 3), yet this lectin exhibited no apparent affinity for Pichia pastoris-expressed hGGT1 (Figure 8, DSL panel, lane 1). These results qualitatively recapitulate the quantitative evaluations from the ALSA microanalyses and support the application of ALSA as a valid approach for identifying differential hGGT1-specific lectin binding patterns in small aliquots of simple (e.g. purified Pp-hGGT1) and complex (e.g. tissue extracts) biological samples.
With the goal of miniaturizing comparative glycoanalyses on hGGT1, we incorporated the use of the highly-versatile ALSA platform to discern whether it was capable of reproducibly identifying differential lectin binding patterns among human kidney and liver tissue sample preparations of hGGT1, which have distinct N-glycan content. To augment the differential analysis, we generated a pool of hGGT1 in the yeast Pichia pastoris that we confirmed by mass spectrometry to be uniquely modified by high-mannose type N-glycans (Figures 3 and 4), a structural class of carbohydrates that are not observed on hGGT1 expressed in normal human kidney and liver tissues but have been documented on hGGT1 expressed in human malignancies ,. We developed a biotinylated version of the Microcystis aeruginosa lectin MVN as a reagent that specifically interacts with high-mannose type N-glycans. With the aid of Core H of the Consortium for Functional Glycomics, we confirmed that MVN exhibits exquisite specificity for Manα(1–2)Man disaccharide, confirming and extending the original analyses conducted by Shahzad-ul-Hussan and colleagues on a more limited array of glycans . Using outlier motif analysis , we gained new insights into the fine saccharide binding specificity of the carbohydrate recognition domain of MVN. Our analysis suggests that an intervening Manα(1–2)Man substituent comprising the central (B) arm of high-mannose structures significantly reduces the affinity of MVN (Figure 1B and Table 1). The affinity pattern of MVN is distinct from the high-mannose binding lectins GNL and ConA, which can cross-react with complex type N-glycans ,.
With the help of this new reagent, we demonstrated that the ALSA platform could reveal clear, precise distinctions in the glycan content on hGGT1 immuno-captured from three distinct sources. Despite significant differences in the complexity of the hGGT1 samples, the immobilized hGGT1 antibody reproducibly captured the target glycoprotein with equivalent efficiency, demonstrating that there was no inherent technical bias in this phase of the analysis (Figures 6C and 7). Moreover, this observation underscores the capacity of this platform to accommodate sample preparations with variable enrichment of the analytical target. In general, the lectin binding patterns illuminated by the ALSA analysis were consistent with known, quantifiable differences in the glycan content on hGGT1 that we had previously identified by mass spectrometry (Figure 4 and ). However, unlike other complementary approaches, discriminatory distinctions in glycan content could be detected on hGGT1 using sub-microgram quantities of total protein within the complex tissue sample pools, and in the case of the Pp-hGGT1, sub-nanogram amounts of total protein were successfully analyzed. As expected, lectins (MVN, GNL, and ConA) with high affinity for high-mannose structures exhibited strong, preferential binding for immuno-captured Pp-hGGT1, which is exclusively modified with high-mannose structures (Figures 4 and 7 and Table 3). In contrast, Pha-E exhibited unique affinity for kidney-expressed hGGT1 (Figure 7 and Table 3). Pha-E is selective for complex type N-glycans containing bisecting GlcNAc motifs . This structural feature was predicted by previous mass spectrometric and enzymatic analyses to be unique to the kidney hGGT1 pool examined in this study (Figure 3 and ,), providing validity to the differential ALSA binding pattern. DSL, on the other hand, exhibited high affinity for kidney hGGT1, moderate affinity for liver hGGT1, and no detectable affinity for Pichia pastoris-expressed hGGT1 by ALSA (Figure 7 and Table 3). In light of the fact that DSL is known to bind N-acetyl-lactosamine motifs (Galβ1-4GlcNAc) ,, a feature unique to hybrid or complex type N-glycans, the ALSA binding pattern exhibited by this lectin is consistent with the greater size and complexity of N-glycans on kidney hGGT1 relative to those identified on the liver enzyme and with the absence of these structural motifs on the Pichia pastoris-expressed enzyme (Figure 4 and ). These patterns were faithfully replicated in standard Western blots of immunoprecipitated hGGT1 samples, albeit consuming approximately 60 times more primary sample. Therefore, these results not only provide proof of concept support for the validity of the ALSA platform in detecting differences in glycosylation patterns on hGGT1 but also demonstrate that primary screening with ALSA using limited amounts of biological material can lead to responsible conservation of primary samples that can subsequently be used for other complementary targeted profiling techniques. A broader search of lectins, or application of lectin arrays , is needed to identify ALSA-exploitable lectins that detect features specific to liver-derived hGGT1. However, liver glycosylation frequently includes sialic acid ,, whose negative charges can inhibit the binding of certain lectins. The lectins in this study do not bind sialylated motifs. We probed for sialic acid modifications on the immunocaptured hGGT1, but we had only low binding with lectins that detect sialylation. We are working to improve the binding of these lectins in the ALSA. Quantitative binding data from an expanded lectin pool may predict glycan motifs that are unique to hGGT1 from each of these sources . Interestingly, GSL-1 and ECL, which are known for Gal-associated motifs not expected on Pichia pastoris-expressed glycoproteins, exhibited substantial binding to Pp-hGGT1 (Figures 6C and 7). However, even these lectins show weak cross-reactivity with certain high mannose N-glycans in publically available databases (www.functionalglycomics.org). This suggests that certain N-glycans formed by the Pichia pastoris strain employed here are able to adopt a conformation that can be recognized by GSL-1 and ECL.
Based on the promising attributes of this analytical approach, we anticipate that this adapted version of the ALSA platform can be applied to directly survey the manner and extent in which altered glycosylation patterns on hGGT1 positively correlate with various primary malignancies and other relevant pathologies in order to evaluate their potential for providing diagnostic or prognostic information that might assist with clinical intervention strategies.
The nucleotide sequence for the open-reading frame (ORF) of MVN (EMBL accession AM041066) was synthesized with flanking NdeI and BamHI restriction sites in the pUC57 shuttle vector GenScript (Piscataway, NJ). The MVN ORF was transferred into the E. coli expression construct pET-15b (Invitrogen, Grand Island, NY), using NdeI and BamHI, where it was expected to encode the full-length protein with an N-terminal hexahistadine tag. The resultant construct was transformed into E. coli BL21 (DE3) and transformants were isolated at 37°C on Luria-Bertani (LB) agarose media containing 100 μg/mL ampicillin. A clonal transformant was propagated at 37°C to an OD600 of ~0.6. The culture was then cooled to room temperature in a water bath, supplemented with isopropyl β-D-1-thiogalactopyranoside (IPTG) to 0.5 mM, and shaken for another 3 h at 25°C. Cells were harvested at 4,000 × g for 15 min at room temperature, resuspended in Binding Buffer (50 mM sodium phosphate, pH 8.0, 300 mM NaCl, 1 μM leupeptin, 1 μg/mL aprotinin) containing 10 mM imidazole, and lysed in an ice-cold French Press. The lysate was centrifuged at 10,000 × g for 20 min at 4°C, and the clarified supernatant loaded onto PerfectPro Ni-NTA (5Prime, Gaithersburg, MA) column. The column was washed with 20 bed volumes of Binding Buffer containing 20 mM imidazole, and the affinity-bound protein was eluted with Binding Buffer containing 250 mM imidazole. Fractions containing affinity-purified MVN [as monitored by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE)] were pooled and dialyzed against phosphate-buffered saline (PBS: 10 mM Na2HPO4, 1.8 mM KH2PO4, 137 mM NaCl, 2.7 mM KCl, pH 7.4). MVN was biotinylated using the EZ-Link NHS-SS- Biotinylation kit (Pierce, Rockland, IL), according to the manufacturer’s protocol, and then fractionated away from unconjugated biotin on a Sephadex G-25 (Sigma-Aldrich, St. Louis, MO) column equilibrated in PBS. The resulting biotinylated MVN stock (1.0 mg/mL) was supplemented with 0.05% sodium azide and stored at 4°C.
Glycan array analysis
The glycan array data were collected by Core H of the Consortium for Functional Glycomics (CFG), using biotinylated MVN and Alexa Fluor 488-conjugated avidin (Invitrogen) on Version 5.0 of the printed glycan array, according to protocols that were published previously . Version 5.0 of the glycan array consists of 611 unique glycans in replicates of six.
Purification of human GGT1 from Pichia pastoris
Recombinant glycosylated human GGT1 was affinity-purified from Pichia pastoris X-33 strain ,, and aliquots (0.25 mg/mL) were stored at −80°C in 25 mM Tris–HCl, 1 mM dithiothreitol, 0.5 mM EDTA, pH 8.0.
Mass spectrometric analyses
Release of N-Glycans
N-glycans were released from 5 μg of recombinant hGGT1 using peptide:N-glycosidase F (PNGase F, New England Biolabs, Ipswich, MA) and then purified, using Sep-Pak C18 columns (Waters Corp., Milford, MA) and activated charcoal Carbograph cartridges (Harvard Apparatus, Holliston, MA). The N-glycan pool was then dried and resuspended in 20 μL of 50% methanol/50% H2O, as described previously .
N-glycans (0.5 μL) were analyzed by MALDI-TOF-MS in positive ion mode on an Ultraflex II mass spectrometer (Bruker Daltonics, Billerica, MA) with a SMARTbeam laser, using 2,5-dihydroxybenzoic acid, as described . A dextrin ladder (M r 500–3000, V-laboratories, Covington, LA) was spotted and analyzed in parallel as an external mass calibrant. Mass accuracy was typically <50 ppm for glycans.
Tryptic digests were prepared and analyzed on a QSTAR Elite hybrid quadrupole-TOF mass spectrometer (Applied Biosystems, Grand Island, NY) equipped with a nanospray ionization source (Ultimate 3000, Dionex, Sunnyvale, CA), as described previously . Briefly, 1.2 μg of trypsinized protein was eluted from a C18 column using acetonitrile/TFA directly into the mass spectrometer programmed to perform MS/MS fragmentation on the three most abundant ions under data-dependent conditions. Candidate glycopeptides were manually identified within the data set by probing the entire LC/MS-MS run for mass matches against predicted glycopeptides and expanded by the inclusion of glycans of related compositions, as informed by the glycans identified in the glycomics data. Assuming equal ionization efficiency of each glycoform at a particular N-glycosylation site, the relative abundance of each glycoform on a single glycosylation site was determined by summing the total ion intensities for all of the glycoforms within a glycopeptide family over the entire elution window. Each total ion intensity was then calculated as a percentage relative to the other family members. The reported percentages represent the average of at least three separate LC/MS-MS experiments.
Tissue extracts and sample preparations
Normal human kidney and liver tissues were obtained from the National Disease Research Interchange (Philadelphia, PA) and stored at −80°C. CHAPS-solubilized membrane fractions containing hGGT1 were prepared as described previously . Using a standardized quantitative biochemical assay for GGT1 transpeptidation activity , tissue extracts and aliquots of Pichia pastoris-expressed hGGT1 were volume-normalized, such that equivalent total units of hGGT1 activity from each sample pool were diluted into 25 mM Tris–HCl buffer (pH 7.4) containing 0.5% CHAPS. The total protein concentrations of the activity-normalized samples used for ALSA analyses were 4.8, 25.5, and 0.007 mg/mL for kidney, liver, and Pichia pastoris-expressed hGGT1 preparations, respectively. These studies were approved by the Institutional Review Board at the University of Oklahoma Health Sciences Center under IRB Protocol #11000.
Microarray fabrication and preparation
Antibody microarrays were prepared as previously described . A microarrayer (2470 Arrayer, Aushon Biosystems, Billerica, MA) was used to spot subnanoliter droplets of each antibody solution, prepared at 250 μg/mL in 1X PBS, on the surfaces of ultrathin nitrocellulose-coated glass microscope slides (PATH slides, Grace Bio-Labs, Bend, OR). Forty-eight identical arrays were printed on each slide, with each array consisting of the antibody targeting hGGT1, as well as negative and positive control antibodies, printed in six replicates. A wax border was imprinted around each of the arrays to define hydrophobic boundaries (SlideImprinter, The Gel Company, San Francisco, CA). For chemical derivatization of the printed antibodies, each slide was incubated in 150 mM sodium metaperiodate diluted in 0.02 M sodium acetate (pH 5.5) for two hours at 4°C, washed in 0.02 M sodium acetate (pH 5.5) for three minutes at room temperature, and then incubated in 0.02 M sodium acetate containing 10 mM L-glutamic acid for two hours at room temperature. Slides were then washed three times in PBS containing 0.5% Tween-20, centrifuged briefly, and then were stored at 4°C in a desiccated, vacuum-sealed slide box until use.
Assays were performed similar to previously described methods ,. Aliquots of volume-and activity-normalized stocks of kidney and liver tissue extracts or Pichia pastoris-expressed hGGT1 were supplemented with SDS to a final concentration 0.5% and denatured at 100°C for 10 minutes in order to dissociate hGGT1 from co-purifying membrane-bound glycoproteins. Samples were then cooled to room temperature and then diluted two-fold into a PBS buffer containing 0.1% Brij, 0.1% Tween-20 and 50 μg/mL of protease inhibitor. An IgG/IgY cocktail consisting of a final concentration of 400 μg/mL goat and sheep IgG and 800 μg/mL rabbit and mouse IgG (Jackson Immunoresearch, West Grove, PA) was added to each sample to eliminate non-specific binding to the printed antibodies. Slides were blocked in a solution containing PBS-0.5% Tween-20 buffer with the addition of 1% BSA. Six microliters of sample were then applied to each array overnight at 4°C. The arrays were washed in three changes of PBS/0.1% Tween-20 for three minutes each and dried by centrifugation (Eppendorf 5810R, rotor A-4-62, 1500 × g for three minutes). Captured antigens were detected with biotinylated detection reagents at a concentration of 1–10 μg/mL for one hour at room temperature followed by incubation with 1 μg/mL streptavidin-phycoerythrin (Roche Applied Science, Indianapolis, IN). The slides were washed and dried as above and scanned for fluorescence emission at 575 nm using a microarray scanner (LS Reloaded, TECAN, Durham, NC). At least three independent sample array analyses were conducted for each ALSA experiment. The data analysis and preparation was performed using Microsoft Excel and Canvas X.
Equivalent units of hGGT1 activity from Pichia pastoris-expressed hGGT1 stocks and from normal human kidney and liver tissue extracts were subjected to immunoprecipitation with GGT129 antibody and bovine serum albumin-blocked protein G-Sepharose beads (GE Healthcare, Piscataway, NJ), as described . Bound proteins were eluted in 50 μL of Laemmli sample buffer (2% SDS, 5% glycerol, 5% 2-mercaptoethanol, 0.002% bromphenol blue, 62.5 mM Tris–HCl, pH 6.8) for 10 min at 100°C, and five microliter aliquots of each eluate were resolved on 8% SDS-PAGE gels. The resolved proteins were electroblotted onto nitrocellulose membranes and blocked overnight at 4°C in Carbo-Free blocking agent (Vector Labs, Burlingame, CA). Lectin blotting was conducted using the appropriate biotinylated lectins diluted in PBS containing 1 mM calcium chloride and 0.05% Tween-20 (PBST). Each membrane was incubated in PBST with either 1.0 μg/mL biotinylated MVN (described herein), 1.0 μg/mL biotinylated Datura stramonium lectin (DSL, Vector Labs), or 0.2 μg/mL biotinylated Phaseolus vulgaris-Erythroagglutinin (Pha-E, Vector Labs) for 1 h at room temperature. Membranes were then washed six times for five minutes with PBST and incubated with 0.5 μg/mL horseradish peroxidase-conjugated avidin (avidin-HRP, Vector Labs) for 1 h at room temperature in PBST. The membranes were subjected to an additional round of washing with PBST, and the blots were visualized by chemiluminescence, according to the manufacturer's protocol (ECL Plus, GE Healthcare). Western blotting against the large subunit of GGT1 was carried out as described previously .
Antibody-lectin sandwich arrays
Consortium for Functional Glycomics
Concanavalin A the Canavalia ensiformis lectin
Carbohydrate recognition domain
Datura stramonium lectin
Euonymus europaeus lectin
γ-Glutamyl transpeptidase 1
Galanthus nivalis lectin
Griffonia simplicifolia lectin 1
Lens culinaris agglutinin lectin
- Pp-hGGT1 Human GGT1 :
expressed in Pichia pastoris
Hanigan MH, Ricketts WA: Extracellular glutathione is a source of cysteine for cells that express gamma-glutamyl transpeptidase. Biochemistry. 1993, 32 (24): 6302-6306. 10.1021/bi00075a026.
Hanigan MH, Frierson HF: Immunohistochemical detection of gamma-glutamyl transpeptidase in normal human tissue. J Histochem Cytochem. 1996, 44 (10): 1101-1108. 10.1177/44.10.8813074.
Lieberman MW, Wiseman AL, Shi ZZ, Carter BZ, Barrios R, Ou CN, Chevez-Barrios P, Wang Y, Habib GM, Goodman JC, Huang SL, Lebovitz RM, Matzuk MM: Growth retardation and cysteine deficiency in gamma-glutamyl transpeptidase-deficient mice. Proc Natl Acad Sci U S A. 1996, 93 (15): 7923-7926. 10.1073/pnas.93.15.7923.
Hanigan MH, Gallagher BC, Taylor PT, Large MK: Inhibition of gamma-glutamyl transpeptidase activity by acivicin in vivo protects the kidney from cisplatin-induced toxicity. Cancer Res. 1994, 54 (22): 5925-5929.
Hanigan MH, Frierson HF, Swanson PE, De Young BR: Altered expression of gamma-glutamyl transpeptidase in human tumors. Hum Pathol. 1999, 30 (3): 300-305. 10.1016/S0046-8177(99)90009-6.
Tsutsumi M, Sakamuro D, Takada A, Zang SC, Furukawa T, Taniguchi N: Detection of a unique gamma-glutamyl transpeptidase messenger RNA species closely related to the development of hepatocellular carcinoma in humans: a new candidate for early diagnosis of hepatocellular carcinoma. Hepatology. 1996, 23 (5): 1093-1097.
Murata J, Ricciardi-Castagnoli P, Dessous L'Eglise Mange P, Martin F, Juillerat-Jeanneret L: Microglial cells induce cytotoxic effects toward colon carcinoma cells: measurement of tumor cytotoxicity with a gamma-glutamyl transpeptidase assay. Int J Cancer. 1997, 70 (2): 169-174. 10.1002/(SICI)1097-0215(19970117)70:2<169::AID-IJC6>3.0.CO;2-V.
Hanigan MH, Gallagher BC, Townsend DM, Gabarra V: Gamma-glutamyl transpeptidase accelerates tumor growth and increases the resistance of tumors to cisplatin in vivo. Carcinogenesis. 1999, 20 (4): 553-559. 10.1093/carcin/20.4.553.
Pompella A, Corti A, Paolicchi A, Giommarelli C, Zunino F: Gamma-glutamyltransferase, redox regulation and cancer drug resistance. Curr Opin Pharmacol. 2007, 7 (4): 360-366. 10.1016/j.coph.2007.04.004.
Corti A, Franzini M, Paolicchi A, Pompella A: Gamma-glutamyltransferase of cancer cells at the crossroads of tumor progression, drug resistance and drug targeting. Anticancer Res. 2010, 30 (4): 1169-1181.
Whitfield JB: Gamma glutamyl transferase. Crit Rev Clin Lab Sci. 2001, 38 (4): 263-355. 10.1080/20014091084227.
Emdin M, Pompella A, Paolicchi A: Gamma-glutamyltransferase, atherosclerosis, and cardiovascular disease: triggering oxidative stress within the plaque. Circulation. 2005, 112 (14): 2078-2080. 10.1161/CIRCULATIONAHA.105.571919.
Turgut O, Tandogan I: Gamma-glutamyltransferase to determine cardiovascular risk: shifting the paradigm forward. J Atheroscler Thromb. 2011, 18 (3): 177-181. 10.5551/jat.6189.
Castonguay R, Halim D, Morin M, Furtos A, Lherbet C, Bonneil E, Thibault P, Keillor JW: Kinetic characterization and identification of the acylation and glycosylation sites of recombinant human gamma-glutamyltranspeptidase. Biochemistry. 2007, 46 (43): 12253-12262. 10.1021/bi700956c.
West MB, Wickham S, Quinalty LM, Pavlovicz RE, Li C, Hanigan MH: Autocatalytic cleavage of human gamma-glutamyl transpeptidase is highly dependent on N-glycosylation at asparagine 95. J Biol Chem. 2011, 286 (33): 28876-28888. 10.1074/jbc.M111.248823.
West MB, Chen Y, Wickham S, Heroux A, Cahill K, Hanigan MH, Mooers BH: Novel insights into eukaryotic gamma-glutamyltranspeptidase 1 from the crystal structure of the glutamate-bound human enzyme. J Biol Chem. 2013, 288 (44): 31902-31913. 10.1074/jbc.M113.498139.
West MB, Segu ZM, Feasley CL, Kang P, Klouckova I, Li C, Novotny MV, West CM, Mechref Y, Hanigan MH: Analysis of site-specific glycosylation of renal and hepatic gamma-glutamyl transpeptidase from normal human tissue. J Biol Chem. 2010, 285 (38): 29511-29524. 10.1074/jbc.M110.145938.
Nemesanszky E, Lott JA: Gamma-glutamyltransferase and its isoenzymes: progress and problems. Clin Chem. 1985, 31 (6): 797-803.
Yamashita K, Totani K, Iwaki Y, Takamisawa I, Tateishi N, Higashi T, Sakamoto Y, Kobata A: Comparative study of the sugar chains of gamma-glutamyltranspeptidases purified from human hepatocellular carcinoma and from human liver. J Biochem. 1989, 105 (5): 728-735.
Arai K, Yoshida K, Komoda T, Kobayashi N, Sakagishi Y: Differences in the enzymatic nature and the sugar-chain structure of gamma-glutamyl transferase between normal and carcinomatous human kidney and prostate. Clin Chim Acta. 1992, 210 (1–2): 35-46. 10.1016/0009-8981(92)90043-P.
Arai K, Sumi SH, Yoshida K, Komoda T: A precursor form of human kidney gamma-glutamyl transferase in normal and cancerous tissues, and its possible post-translational modification. Biochim Biophys Acta. 1995, 1253 (1): 33-38. 10.1016/0167-4838(95)00141-G.
Yoshida K, Sumi S, Honda M, Hosoya Y, Yano M, Arai K, Ueda Y: Serial lectin affinity chromatography demonstrates altered asparagine-linked sugar chain structures of gamma-glutamyltransferase in human renal cell carcinoma. J Chromatogr B Biomed Appl. 1995, 672 (1): 45-51. 10.1016/0378-4347(95)00199-S.
Ohta H, Sawabu N, Odani H, Kawakami H, Watanabe H, Toya D, Ozaki K, Hattori N: Characterization of gamma-glutamyltranspeptidase from human pancreatic cancer. Pancreas. 1990, 5 (1): 82-90. 10.1097/00006676-199001000-00012.
Okuyama K: Separation and identification of serum gamma-glutamyl transpeptidase isoenzymes by wheat germ agglutinin affinity electrophoresis: a basic analysis and its clinical application to various liver diseases. Keio J Med. 1993, 42 (4): 149-156.
Yamaguchi N, Kawai K, Ashihara T: Discrimination of gamma-glutamyltranspeptidase from normal and carcinomatous pancreas. Clin Chim Acta. 1986, 154 (2): 133-140. 10.1016/0009-8981(86)90005-7.
Chen S, LaRoche T, Hamelinck D, Bergsma D, Brenner D, Simeone D, Brand RE, Haab BB: Multiplexed analysis of glycan variation on native proteins captured by antibody microarrays. Nat Methods. 2007, 4 (5): 437-444.
Yue T, Goldstein IJ, Hollingsworth MA, Kaul K, Brand RE, Haab BB: The prevalence and nature of glycan alterations on specific proteins in pancreatic cancer patients revealed using antibody-lectin sandwich arrays. Mol Cell Proteomics. 2009, 8 (7): 1697-1707. 10.1074/mcp.M900135-MCP200.
Haab BB: Antibody-lectin sandwich arrays for biomarker and glycobiology studies. Expert Rev Proteomics. 2010, 7 (1): 9-11. 10.1586/epr.09.102.
Yue T, Maupin KA, Fallon B, Li L, Partyka K, Anderson MA, Brenner DE, Kaul K, Zeh H, Moser AJ, Simeone DM, Feng Z, Brand RE, Haab BB: Enhanced discrimination of malignant from benign pancreatic disease by measuring the CA 19–9 antigen on specific protein carriers. PLoS One. 2011, 6 (12): e29180-10.1371/journal.pone.0029180.
Cao Z, Maupin K, Curnutte B, Fallon B, Feasley CL, Brouhard E, Kwon R, West CM, Cunningham J, Brand R, Castelli P, Crippa S, Feng Z, Allen P, Simeone DM, Haab BB: Specific glycoforms of MUC5AC and endorepellin accurately distinguish mucinous from nonmucinous pancreatic cysts. Mol Cell Proteomics. 2013, 12 (10): 2724-2734. 10.1074/mcp.M113.030700.
Adamczyk B, Tharmalingam T, Rudd PM: Glycans as cancer biomarkers. Biochim Biophys Acta. 2012, 1820 (9): 1347-1353. 10.1016/j.bbagen.2011.12.001.
Angata T, Fujinawa R, Kurimoto A, Nakajima K, Kato M, Takamatsu S, Korekane H, Gao CX, Ohtsubo K, Kitazume S, Taniguchi N: Integrated approach toward the discovery of glyco-biomarkers of inflammation-related diseases. Ann N Y Acad Sci. 2012, 1253: 159-169. 10.1111/j.1749-6632.2012.06469.x.
Fuster MM, Esko JD: The sweet and sour of cancer: glycans as novel therapeutic targets. Nat Rev Cancer. 2005, 5 (7): 526-542. 10.1038/nrc1649.
Ribeiro JP, Mahal LK: Dot by dot: analyzing the glycome using lectin microarrays. Curr Opin Chem Biol. 2013, 17 (5): 827-831. 10.1016/j.cbpa.2013.06.009.
Haab BB: Using lectins in biomarker research: addressing the limitations of sensitivity and availability. Proteomics Clin Appl. 2012, 6 (7–8): 346-350. 10.1002/prca.201200014.
Rudiger H, Gabius HJ: Plant lectins: occurrence, biochemistry, functions and applications. Glycoconj J. 2001, 18 (8): 589-613. 10.1023/A:1020687518999.
North SJ, Hitchen PG, Haslam SM, Dell A: Mass spectrometry in the analysis of N-linked and O-linked glycans. Curr Opin Struct Biol. 2009, 19 (5): 498-506. 10.1016/j.sbi.2009.05.005.
Kehr JC, Zilliges Y, Springer A, Disney MD, Ratner DD, Bouchier C, Seeberger PH, de Marsac NT, Dittmann E: A mannan binding lectin is involved in cell-cell attachment in a toxic strain of Microcystis aeruginosa. Mol Microbiol. 2006, 59 (3): 893-906. 10.1111/j.1365-2958.2005.05001.x.
Shahzad-ul-Hussan S, Gustchina E, Ghirlando R, Clore GM, Bewley CA: Solution structure of the monovalent lectin microvirin in complex with Man(alpha)(1–2)Man provides a basis for anti-HIV activity with low toxicity. J Biol Chem. 2011, 286 (23): 20788-20796. 10.1074/jbc.M111.232678.
Maupin KA, Liden D, Haab BB: The fine specificity of mannose-binding and galactose-binding lectins revealed using outlier motif analysis of glycan array data. Glycobiology. 2012, 22 (1): 160-169. 10.1093/glycob/cwr128.
Blanchard V, Gadkari RA, Gerwig GJ, Leeflang BR, Dighe RR, Kamerling JP: Characterization of the N-linked oligosaccharides from human chorionic gonadotropin expressed in the methylotrophic yeast Pichia pastoris. Glycoconj J. 2007, 24 (1): 33-47. 10.1007/s10719-006-9010-3.
Blanchard V, Gadkari RA, George AV, Roy S, Gerwig GJ, Leeflang BR, Dighe RR, Boelens R, Kamerling JP: High-level expression of biologically active glycoprotein hormones in Pichia pastoris strains–selection of strain GS115, and not X-33, for the production of biologically active N-glycosylated 15 N-labeled phCG. Glycoconj J. 2008, 25 (3): 245-257. 10.1007/s10719-007-9082-8.
Hirose M, Kameyama S, Ohi H: Characterization of N-linked oligosaccharides attached to recombinant human antithrombin expressed in the yeast Pichia pastoris. Yeast. 2002, 19 (14): 1191-1202. 10.1002/yea.914.
King JB, West MB, Cook PF, Hanigan MH: A novel, species-specific class of uncompetitive inhibitors of gamma-glutamyl transpeptidase. J Biol Chem. 2009, 284 (14): 9059-9065. 10.1074/jbc.M809608200.
Fouquaert E, Smith DF, Peumans WJ, Proost P, Balzarini J, Savvides SN, Damme EJ: Related lectins from snowdrop and maize differ in their carbohydrate-binding specificity. Biochem Biophys Res Commun. 2009, 380 (2): 260-265. 10.1016/j.bbrc.2009.01.048.
Porter A, Yue T, Heeringa L, Day S, Suh E, Haab BB: A motif-based analysis of glycan array data to determine the specificities of glycan-binding proteins. Glycobiology. 2010, 20 (3): 369-380. 10.1093/glycob/cwp187.
Petryniak J, Goldstein IJ: Evonymus europaea lectin. Methods Enzymol. 1987, 138: 552-561. 10.1016/0076-6879(87)38050-4.
Teneberg S, Alsen B, Angstrom J, Winter HC, Goldstein IJ: Studies on Galalpha3-binding proteins: comparison of the glycosphingolipid binding specificities of Marasmius oreades lectin and Euonymus europaeus lectin. Glycobiology. 2003, 13 (6): 479-486. 10.1093/glycob/cwg049.
Goldstein IJ, Blake DA, Ebisu S, Williams TJ, Murphy LA: Carbohydrate binding studies on the Bandeiraea simplicifolia I isolectins. Lectins which are mono-, di-, tri-, and tetravalent for N-acetyl-D-galactosamine. J Biol Chem. 1981, 256 (8): 3890-3893.
Teneberg S, Angstrom J, Jovall PA, Karlsson KA: Characterization of binding of Gal beta 4GlcNAc-specific lectins from Erythrina cristagalli and Erythrina corallodendron to glycosphinogolipids. Detection, isolation, and characterization of a novel glycosphinglipid of bovine buttermilk. J Biol Chem. 1994, 269 (11): 8554-8563.
Fouquaert E, Peumans WJ, Smith DF, Proost P, Savvides SN, Van Damme EJ: The "old" Euonymus europaeus agglutinin represents a novel family of ubiquitous plant proteins. Plant Physiol. 2008, 147 (3): 1316-1324. 10.1104/pp.108.116764.
Ryall RG, Story CJ, Turner DR: Reappraisal of the causes of the "hook effect" in two-site immunoradiometric assays. Anal Biochem. 1982, 127 (2): 308-315. 10.1016/0003-2697(82)90178-6.
Crowley JF, Goldstein IJ, Arnarp J, Lonngren J: Carbohydrate binding studies on the lectin from Datura stramonium seeds. Arch Biochem Biophys. 1984, 231 (2): 524-533. 10.1016/0003-9861(84)90417-X.
Cummings RD, Kornfeld S: Characterization of the structural determinants required for the high affinity interaction of asparagine-linked oligosaccharides with immobilized Phaseolus vulgaris leukoagglutinating and erythroagglutinating lectins. J Biol Chem. 1982, 257 (19): 11230-11234.
Orchekowski R, Hamelinck D, Li L, Gliwa E, van Brocklin M, Marrero JA, Vande Woude GF, Feng Z, Brand R, Haab BB: Antibody microarray profiling reveals individual and combined serum proteins associated with pancreatic cancer. Cancer Res. 2005, 65 (23): 11193-11202. 10.1158/0008-5472.CAN-05-1436.
Yamashita K, Totani K, Ohkura T, Takasaki S, Goldstein IJ, Kobata A: Carbohydrate binding properties of complex-type oligosaccharides on immobilized Datura stramonium lectin. J Biol Chem. 1987, 262 (4): 1602-1607.
Wu AM, Song SC, Sugii S, Herp A: Differential binding properties of Gal/GalNAc specific lectins available for characterization of glycoreceptors. Indian J Biochem Biophys. 1997, 34 (1–2): 61-71.
Pilobello KT, Krishnamoorthy L, Slawek D, Mahal LK: Development of a lectin microarray for the rapid analysis of protein glycopatterns. Chembiochem. 2005, 6 (6): 985-989. 10.1002/cbic.200400403.
Bekesova S, Kosti O, Chandler KB, Wu J, Madej HL, Brown KC, Simonyan V, Goldman R: N-glycans in liver-secreted and immunoglogulin-derived protein fractions. J Proteomics. 2012, 75 (7): 2216-2224. 10.1016/j.jprot.2012.01.024.
McCarter C, Kletter D, Tang H, Partyka K, Ma Y, Singh S, Yadav J, Bern M, Haab BB: Prediction of glycan motifs using quantitative analysis of multi-lectin binding: Motifs on MUC1 produced by cultured pancreatic cancer cells. Proteomics Clin Appl. 2013, 7 (9–10): 632-641.
Blixt O, Head S, Mondala T, Scanlan C, Huflejt ME, Alvarez R, Bryan MC, Fazio F, Calarese D, Stevens J, Skehel JJ, van Die I, Burton DR, Wilson IA, Cummings R, Bovin N, Wong CH, Paulson JC: Printed covalent glycan array for ligand profiling of diverse glycan binding proteins. Proc Natl Acad Sci U S A. 2004, 101 (49): 17033-17038. 10.1073/pnas.0407902101.
Feasley CL, Hykollari A, Paschinger K, Wilson IB, West CM: N-glycomic and N-glycoproteomic studies in the social amoebae. Methods Mol Biol. 2013, 983: 205-229. 10.1007/978-1-62703-302-2_11.
This work was supported by Early Detection Research Network, grant 1U01CA152653 (B.B.H.), an Institutional Development Award (IDeA) from the National Institute of General Medical Sciences of the National Institutes of Health P20GM103640 and National Institutes of Health grants RO1 CA57530 and R56 CA57530 (M.H.H.) and F32 CA128338 (M.B.W.). We also acknowledge the Consortium for Functional Glycomics, which is funded by NIGMS (GM62116), for support of the glycan array analysis.
The authors declare that they have no competing interests.
MBW conceived of the study, made the construct for the microvirin, expressed the microvirin and arranged for its evaluation on the glycan microarray at the CFG, prepared the hGGT1 samples, Western blot analyses, prepared Figures 3,4,5, 8 and Tables 1 and 2, and wrote the manuscript. KP conducted the ALSA studies, wrote the methods section for the ALSA. CLF conducted the mass spectrometry studies. KAM worked with KP on the ALSA experiments, prepared Table 1, Figures 1 and 2. IG participated in the ALSA studies and assisted with editing the manuscript. CMW oversaw the mass spectrometry studies and was actively involved in editing the manuscript. BBH supervised the ALSA studies prepared Figures 6 and 7 and edited the manuscript. MHH oversaw the design of the study, was actively involved in its progress, contributed to the writing of the manuscript, formatted and submitted the manuscript for publication. All authors read and approved the final manuscript.
Electronic supplementary material
Authors’ original submitted files for images
Below are the links to the authors’ original submitted files for images.
About this article
Cite this article
West, M.B., Partyka, K., Feasley, C.L. et al. Detection of distinct glycosylation patterns on human γ-glutamyl transpeptidase 1 using antibody-lectin sandwich array (ALSA) technology. BMC Biotechnol 14, 101 (2014). https://doi.org/10.1186/s12896-014-0101-0
- γ-Glutamyl transpeptidase
- Antibody-lectin sandwich arrays