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Review

Hidden Relationships between N-Glycosylation and Disulfide Bonds in Individual Proteins

by
Tania Bakshi
1,
David Pham
2,
Raminderjeet Kaur
3 and
Bingyun Sun
1,4,*
1
Department of Molecular Biology and Biochemistry, Simon Fraser University, Burnaby, BC V5A 1S6, Canada
2
Department of Computing Science, Simon Fraser University, Burnaby, BC V5A 1S6, Canada
3
Faculty of Health Science, Simon Fraser University, Burnaby, BC V5A 1S6, Canada
4
Department of Chemistry, Simon Fraser University, Burnaby, BC V5A 1S6, Canada
*
Author to whom correspondence should be addressed.
Int. J. Mol. Sci. 2022, 23(7), 3742; https://doi.org/10.3390/ijms23073742
Submission received: 8 March 2022 / Revised: 25 March 2022 / Accepted: 28 March 2022 / Published: 29 March 2022
(This article belongs to the Special Issue Advances in Proteomic Research)
Browse Figures
Versions Notes

Abstract

:
N-Glycosylation (NG) and disulfide bonds (DBs) are two prevalent co/post-translational modifications (PTMs) that are often conserved and coexist in membrane and secreted proteins involved in a large number of diseases. Both in the past and in recent times, the enzymes and chaperones regulating these PTMs have been constantly discovered to directly interact with each other or colocalize in the ER. However, beyond a few model proteins, how such cooperation affects N-glycan modification and disulfide bonding at selective sites in individual proteins is largely unknown. Here, we reviewed the literature to discover the current status in understanding the relationships between NG and DBs in individual proteins. Our results showed that more than 2700 human proteins carry both PTMs, and fewer than 2% of them have been investigated in the associations between NG and DBs. We summarized both these proteins with the reported relationships in the two PTMs and the tools used to discover the relationships. We hope that, by exposing this largely understudied field, more investigations can be encouraged to unveil the hidden relationships of NG and DBs in the majority of membranes and secreted proteins for pathophysiological understanding and biotherapeutic development.

1. Introduction

Both N-glycosylation (NG) and disulfide bonds (DBs) can form co- and post-translational modifications (PTMs) [1] on proteins in the endoplasmic reticulum (ER) while they pass through the secretory pathway. These two modifications are not only common but often evolutionarily conserved in membrane and secreted proteins from prokaryotes to eukaryotes. As two critical modifications, they facilitate protein folding and regulate protein structure, function, stability, and cellular localization. Defects in either one can fail protein ER quality control, trigger unfolded protein response, and cause pathological conditions ranging from heritable congenital disorders of glycosylation as an example to acquired disorders such as cancers, dementia, diabetes, autoimmune, infectious, and cardiovascular diseases [2,3].
Owing to their importance, both NG and DBs have been frequently investigated in numerous proteins. In UniProt [4], over 2700 human proteins have both PTMs annotated. However, the associations between NG and DBs have only been well examined in a few model proteins, such as influenza hemagglutinin (HA) [5,6,7]. Both past and recent discoveries have shown that the enzymes responsible for adding, processing, and degrading N-glycans are closely related to proteins with the abilities of adding, isomerizing, and breaking disulfide bonds. Beyond some well-studied model proteins, how NG and DB formation affect each other in the remaining individual proteins is the focus of this review. By reviewing research articles, we generally cataloged the observed relationships from the host proteins into three kinds, including inhibition, promotion, and no relationship. More importantly, we noticed that the majority of the studies did not investigate the interactions between the two PTMs but studied them separately. As a result, some of the observed structural and functional changes in proteins can be a synergistic effect of both instead of one PTM. The reasons are likely that the tools required for these studies were not widely recognized and/or the importance of the associations between them were not commonly appreciated. To raise awareness, this review not only summarizes molecular foundations to support a potentially complex relationship and the current known relationships between NG and DBs in individual proteins but also enlists the relevant tools that can be used for addressing these relationships and provides our recommendations for future high-throughput analysis.

2. Molecular Foundations

When nascent proteins are translocated into the ER, NG and DB formation are two closely associated events. NG is a complex process that refers to a dolichol pyrophosphate donor transferring a tetradecasaccharide precursor en bloc to the nitrogen atom of the asparagine side chain in a consensus sequence (namely, sequon), i.e., N–X–S/T, in which X can be any amino acid but not proline [8]. Newly added N-glycans are further processed while glycosylated proteins fold and mature in the ER. Glycoproteins that fail the quality control in the ER are subjected to the ER-associated degradation process (ERAD) [9]. N-Glycans are bulky. The addition of an N-glycan can shape the local conformation of a polypeptide chain through the first GlcNAc residue, the triose core, and the outer sugar moieties [10,11,12]. Either intra- or extramolecular N-glycans can stabilize a loose polypeptide conformation via both hydrophilic and hydrophobic interactions with the peptide backbone [13]. The stabilized conformation can bring two free cysteine side-chains in close proximity to promote an otherwise slow or energetically costly DB formation, as experimentally proven in model peptides and whole proteins [12,13,14,15].
The covalent disulfide bond is formed by oxidizing two free thiol groups in two cysteine residues in the vicinity. In the ER, DBs can be formed, isomerized, or broken by a number of oxidoreductases. Over 20 ER resident oxidoreductases, also called protein disulfide isomerase (PDI) family enzymes, have been discovered [16]. The characteristic feature of PDI family proteins is the thioredoxin fold, C–X–X–C. This motif is usually the catalytic domain of oxidoreductases. These enzymes can use the cysteines in the motif to exchange electrons in the thiols of the substrate to either form or break DBs [17]. In addition, the mixed DBs formed between the oxidoreductase and the substrate through the thioredoxin fold can often stabilize the substrate and allow further modifications, such as N-glycosylation, by other cooperating enzymes in the same complex or nearby [18]. Overall, PDIs can carry out a number of functions, including oxidoreduction, isomerization, and chaperone activity [19].
Due to the spatial requirement of DBs, the protein structure can be largely perturbed or stabilized after the formation of novel DBs or the reshuffling of existing DBs. For glycoproteins carrying bulky N-glycans to fold and mature in the ER, the formation of DBs can block or restrain the access of glycoenzymes or chaperones to N-glycans. Interestingly, glycoenzymes and glycochaperones are often accompanied by oxidoreductases in the ER, or the glycoenzyme itself has a thioredoxin fold that can interact with thiols in substrates, as recently reviewed by Patel et al. [9]. For example, the oxidoreductases of MAGT1 or TUSC3 are part of STT3B of OST, the enzyme responsive to adding N-glycans to proteins; the oxidoreductases of ERp57 and ERp72 form complexes with CNX/CRT, the ER chaperones of N-glycoproteins; in the ER N-glycosylation quality control system, UGGT1 itself has thioredoxin-like motifs and interacts with SELENOF (Sep15), a selenocysteine-containing oxidoreductase [20]; further along the thread in the ERAD, BIP binds PDI, P5, and ERdj5, whereas EDEMs bind TXNDC11, P4HB, ERp46, etc. The intriguing roles of NG and DBs are just beginning to be realized.
Beyond the ER, both NG and DBs can be further edited. For example, after exiting the ER, N-glycans can be processed in the Golgi [21]. For DBs, a number of enzymes both inside and outside of cells can break and reform these covalent bonds, which often function as switches to activate or suppress host protein functions [22]. How NG and DBs relate to each other beyond the ER remains a question [9]. A complete elucidation of these interactions requires kinetic information of the modification in the time domain, as well as spatial information on their cellular localization. As introduced later, kinetic measurements of PTMs can be performed through traditional pulse-chase or mass spectrometry (MS). The former has been well developed, while the latter is emerging [23]. Spatial information can be delineated through inhibitors specific to an enzymatic step or stressors to a particular organelle.
Nevertheless, not all DBs are linked to every NG in a protein. The functions of both NG and DBs are pleiotropic. The Weerapana group has cataloged the functions of reactive cysteines into five types, including structural, regulatory, redox catalytic, catalytic nucleophile, and metal-binding cysteines [24]. Similarly, the functions of NG range from facilitating local folding to promoting secondary structures, increasing protein stability, protecting hydrophobic surfaces, reducing aggregation, guiding trafficking, and functioning as epitopes for molecular recognition [25].
Given the close molecular associations between enzymes functioning in the formation and processing of the two PTMs in the ER, as well as the broad availability of both PTMs in membrane and secreted proteins, we asked what the current observed relationships of these two PTMs are in individual proteins. Given that one-third of the mammalian proteome is produced through the secretory pathway [26], most proteins have annotated DBs and NG, as shown in UniProt. We anticipated that rich information can be obtained from such exercises. Below, we summarize our findings on both the relationships in individual proteins and the tools used to study them.

3. Overview of the Studies

To obtain the relevant articles, we searched PubMed using various keywords, including “N-glycosylation and disulfide bonds”, “N-linked glycosylation and disulfide bonds”, “N-linked glycans and disulfide bonds”, “carbohydrate and disulfide bond”, or “glycans and disulfide”. Furthermore, we included the associated studies cited in the selected papers. The combined list had nearly 600 articles.
After establishing the list, we first examined the types of proteins that were studied. Most studied proteins were membrane and secreted proteins of humans, model organisms, and viruses, as shown in Figure 1. Others examined proteins from venomous species such as snakes and wasps, parasites such as hookworms, and agricultural species such as vegetables, fishes, and silkworms. Most of these proteins were surface receptors, adhesion molecules, secreted or membrane-tethered enzymes, cytokines, hormones, signaling molecules, and extracellular matrix proteins. For viruses, the most studied proteins were surface glycoproteins involved in recognition and fusion with host cells. All these results suggested the importance of these two PTMs in diseases originating from cell–protein interactions and cell–cell communications.
Second, we broadly classified all the reports into four categories. For most studies that included both PTMs but ignored their relationships, we cataloged them as “no studies”. We further divided the investigated relationships into three categories: promotion, inhibition, and independent relationships, as summarized in Figure 2 and detailed in Table 1. In Figure 2, the promoting relationship dominated current studies. This relationship, however, was often observed passively by the diminished or inhibited formation of one type of PTM when the other type of PTM was experimentally removed. To a much lesser extent, an inhibitory relationship was observed, in which the formation of one PTM blocked the development of the other. Only in very limited reports did proteins show independent modifications of these two PTMs, in which the removal of one PTM did not affect the formation or the processing of the other. In the four sections below, we use detailed examples to illustrate these observed relationships.
Table
Table 1. Summary of the proteins showing interactions between N-glycosylation and disulfide bonds.
Table 1. Summary of the proteins showing interactions between N-glycosylation and disulfide bonds.
UniProt AccessionProtein NamePosition of DBsPosition of N-GlycansClassReference
A0A346IHA8CD4-binding region of the envelope glycoproteins50–70 a, 219–248 a, 229–240 a, 369–402 a, 362–429, 597–603 a390, 447No relation[27]
Q9Y6R1SLC4 Na+-coupled transporter (NBCe1-A)583–585, 630–642 c597, 617Inhibition[28]
Q99062Granulocyte colony-stimulating factor receptor107–118, 153–162, 224–271, 364–37127, 69, 104, 110, 365, 450, 547, 555, 586Promotion[29]
Q62635Gastric mucin (rat) 160 a, 420 a, 667 a, 767 a, 837 a, 892 a, 1136 a, 1151 a, 1212 a, 1227 a, 1243 a, 1350 a,Promotion[30]
P49018GPI-anchor transamidase (GPI8) yeast85 (interchain with C-194 in GPI16) b256 a, 346 aPromotion[31]
P00750Tissue-type plasminogen activator (t-PA)41–71, 69–78, 86–97, 91–108, 110–119, 127–208 b, 148–190 b, 179–203 b, 215–296, 236–278, 267–291, 299–430, 342–358 b, 350–419 b, 444–519 b, 476–492 b, 509–537 b117, 184, 448Inhibition[32,33]
P04275Von Willebrand factor (VWF)35–162 d, 57–200 d, 388–524 d, 410–559 d, 432–440 d, 509–695, 767–808, 776–804, 810–821, 867–996 d, 889–1031 d, 898–993 d, 914–921 d, 1060–1084, 1071–1111, 1089–1091, 1126–1130, 1149–1169, 1153–1165, 1196–1199, 1234–1237, 1272–1458, 1669–1670, 1686–1872, 1879–1904, 1899–1940 d, 1927–2088, 1950–2085 d, 1972–2123 d, 1993–2001 d, 2724–2774 b, 2739–2788 b, 2750–2804 b, 2754–2806 b99 a, 156 a, 211 a, 666 a, 857 e, 1147 (atypical) e, 1231 e, 1515, 1574 e, 2223 e, 2290 e, 2357 e, 2400 e, 2546, 2585 e, 2790 ePromotion[34,35,36]
P0DN86Human chorionic gonadotropin beta-subunit9–57, 23–72, 26–110, 34–88, 38–90, 93–10013, 30Promotion[37,38,39]
Engineered heterodimeric knob-into-hole Fc fragments349–354 (interchain)297Promotion[40]
P32906Yeast-alpha1,2 mannosidase340–385, 468–47196, 155, 224Promotion[41]
O60896Receptor activity-modifying protein 3 (RAMP3)40–72 b, 57–104 b28, 57, 70, 102Inhibition[42]
Q13087PDIA218 (interchain)127, 284, 516Inhibition[43]
P04853Hemagglutinin-neuraminidase (Sendai virus)129 (interchain) a77, 499, 511Promotion[21,44]
Q91UL0Hemagglutinin-neuraminidase (NDV)123 (interchain), 172–196, 186–247, 238–251, 344–461, 455–465, 531–542119, 341, 433, 481Inhibition[45,46]
Hemagglutinin (Influenza A virus)14–466, 52–277, 64–76, 97–139, 281–305, 473–4778, 22, 38, 81, 165, 285, 483Promotion[47,48]
P01229Human lutropin subunit beta29–77 b, 43–92 b, 46–130 b, 54–108 b, 58–110 b, 113–120 b30Promotion[49]
P35625Metalloproteinase inhibitor 3 (TIMP3)24–91, 26–118, 36–143, 145–192 d, 150–155 d, 163–184 d Inhibition[50]
Q16820Meprin A103–255, 124–144, 265–427, 273 a (interchain), 305 (interchain), 492 (interchain) d, 608–619 d, 613–628 d, 630–643 d41, 152, 234, 270, 330, 426, 452, 546, 553Promotion[51,52]
P01130Low-density lipoprotein (LDL) receptor27–39 e, 34–52 e, 46–63 e, 68–82 e, 75–95 e, 89–104 e, 109–121 b, 116–134 e, 128–143 e, 148–160 e, 155–173 e, 167–184 e, 197–209 e, 204–222 e, 216–231 e, 236–248 e, 243–261 e, 255–270 e, 276–289 e, 284–302 e, 296–313 e, 318–329 e, 325–338 e, 340–352 e, 358–368 e, 364–377 e, 379–392 e, 667–681 e, 677–696 e, 698–711 e97 a, 156, 272, 515 a, 657Inhibition[53,54,55]
Q02817MUC2 mucin59–67 b, 37–169 d, 59–206 d, 391–528 d, 413–563 d, 435–443 d, 860–992 d, 882–1027 d, 891–989 d, 909–916 d, 4481–4622 d, 4503–4661 d, 4527–4535 d, 5075–5122 b, 5089–5136 b, 5098–5152 b, 5102–5154 b163 a, 423 a, 670 a, 770 a, 894 a, 1139 a, 1154 a, 1215 a, 1230 a, 1246 a, 1787 a, 1820 a, 4339 a, 4351 a, 4362 a, 4373 a, 4422 a, 4438 a, 4502 a, 4616 a, 4627 a, 4752 a, 4787 a, 4881 a, 4888 a, 4955 a, 4970 a, 5019 a, 5038 a, 5069 aPromotion[56,57]
P12476VP782–135, 165–249, 191–244, 196–20769Promotion[22,54]
P04156Major prion protein179–214181, 197Promotion[58]
P05026Sodium/potassium-transporting ATPase subunit beta-1126–149, 159–175, 213–276158, 193, 265Promotion[59,60]
P05231Interleukin-6 (IL6)45–51, 74–8446Inhibition[61,62,63]
H2AM12Glycoprotein Gc523–550, 580–589, 591–598, 471–487493, 686Promotion[64]
P221461,3-beta-Glucanosyltransferase74–103, 216–348, 234–265, 370–421, 372–462 b, 379–445 b, 398–403 b40 a, 57, 95 a, 149 a, 165 a, 253, 283 a, 321 a, 409 a, 495 aPromotion[65,66]
P32623Probable glycosidase CRH2 28, 96 a, 190 a, 196 a, 233 a, 237 a, 261 a, 297 a, 310 aPromotion[66]
Q9UMF0Intercellular adhesion molecule-5 (ICAM5)55–99, 59–103, 142–198, 249–302 d, 344–383 d, 415–470 d, 498–552 d, 580–645 d, 673–725 d, 769–814 d54,74,137,195,214,274,316,371,397,582,636,645,762,793,794Promotion[67,68]
O75829Chondromodulin-I131–193 b, 282–286 b, 283–323 b, 293–317 b, 297–313 b243 aNo relation[69]
P40225Thrombopoietin7–151, 29–85197, 206, 234, 255, 340 a, 348 aNo relation[70,71]
Q9UNQ0ABCG2 protein592–608, 603 (interchain)596Promotion[8,72,73]
P56817beta-Site APP-cleaving enzyme (BACE)216–420, 278–443, 330–380153 a, 172 a, 223 a, 354 aPromotion[74]
Q9H1U4Multiple epidermal growth factor-like domains protein 9 (MEGF9)204–217 a, 206–224 a, 226–235 a, 238–251 a, 254–266 a, 256–272 a, 274–283 a, 286–298 a, 301–310 a, 303–317 a, 320–329 a, 332–346 a, 349–360 a, 351–371 a, 374–383 a, 386–397 a, 400–415 a, 402–422 a, 425–434 a, 437–449 a40 a, 182 a, 205 a, 218 a, 245 a, 267 a, 305 a, 428 a, 468 a, 481 a, 500 aInhibition[75]
P53634Cathepsin30–118, 54–136 e, 255–298 e, 291–331 e, 321–337 e29Inhibition[76,77]
P08709Coagulation factor VII348–367360Inhibition[76]
Q07837rBAT242–273, 571–666, 673–685214, 261, 332, 495, 513, 575Promotion[78]
O75355Nucleoside triphosphate diphosphohydrolase 3 (NTPDase3)92–116, 261–308, 289–334, 347–353, 399–42281 a, 149 a, 238 a, 381 a, 392 a, 402 a, 454 aInhibition[79]
P08563E2 glycoprotein (rubella virus) 53, 71, 115Promotion[80]
Q9H9S5Fukutin-related protein (FKRP)6 (interchain)172, 209No relation[81]
O14773Tripeptidyl-peptidase I111–122, 365–526, 522–537210, 222, 286, 313, 443Promotion[82,83,84,85]
P15813CD1d120–184, 224–27920, 42, 108, 163Promotion[86,87,88,89]
O14656TorsinA44–162 a, 280–319143, 158Promotion[90,91]
P21825Translocation protein SEC62 153, 62 ePromotion[92]
P04070Protein C331–34597, 248, 313, 329 (atypical)Promotion[93]
K7WJ21PtrMAN6448, 452, 45623, 194, 227, 375, 392No relation[94]
P01848/P01850TCR alpha and beta22–72, 94 (with C-130 in TRBC1 or TRBC2) and 30–95, 130 (with C-94 in TRAC)32, 66, 77 d, 113 d and 69 dInhibition[95]
P01857Immunoglobulin G1 Fc27–83 d, 103 e, 109 e, 112 e, 144–204 d, 250–308 d180, 297Promotion[84,96,97,98]
Nicotinic acetylcholine receptor fragment128–142141Promotion[12]
Q07108CD6968 (interchain) e, 85–96 e, 113–194 e, 173–186 e111 (atypical), 166Inhibition[99,100]
P15813Antigen-presenting glycoprotein CD1d120–184 e, 224–279 e38 e, 60 e, 126 e, 181 ePromotion[101,102]
P04439MHC class I heavy chain125–188 e, 227–283 e110 ePromotion[103,104]
a—predicted by sequence analysis (accessed from UniProt); b—by similarity (accessed from UniProt); c—a discrepancy between NG sites in the abstract and main text was found in [28]. We used the sites mentioned in the main text as they correspond with UniProt; d—PROSITE-ProRule annotation; e—UniProt.

4. Promoting Relationship

Feng et al. [37] demonstrated through kinetic studies of intracellular folding of the human chorionic gonadotropin (hCG)-β subunit that NG facilitated the rapid formation of DBs and the folding of the hCG-β subunit, which harbors six DBs [39]. The relative positions of NG and DBs are shown in Figure 3. Lacking the two NG sites slowed down the folding of the β subunit more than fourfold from 7 min to 33 min in CHO cells, and the slow formation of DBs retained the misfolded proteins up to 5 h in the ER before degradation [37]. The co-expression of the α subunit could assist the appropriate folding and secretion of the β subunit of the hormone lacking the NG. Among the six DBs in the hCG-β subunit shown in Figure 3, the formation of Cys34–Cys88 occurred earlier than that of Cys9–Cys57/Cys38–Cys90, while the remaining three pairs occurred later [39]. The first three pairs are important in protein folding and secretion and N-glycan processing. Eliminating these early formed DBs rendered part of the N-glycans to be high mannose instead of complex glycans, which were sensitive to ER quality control and degradation.
Another study was conducted in the β subunit of Na, K-ATPase. Na, K-ATPase is a plasma membrane transporter that is responsible for the maintenance of potassium and sodium homeostasis in animal cells [59]. The functional β subunit is a type II glycoprotein composed of a large C-terminal ectodomain with three NG sites (Asn158, Asn193, Asn265) and three conserved DBs (Cys126–Cys149, Cys159–Cys175, and Cys213–Cys276) [59]. The mutation of Cys126–Cys149 increased the non-glycosylated proportion of the protein compared to the wildtype from the Western blot [60], suggesting a promoting relationship. Mutating each of the three glycosylation sites indicated their involvement in initial folding [59]. The acquisition of at least one sugar moiety was necessary for the β subunit to ensure its association with the α subunit through pulse chase. Interestingly, when all three N-glycans were removed, the protein did not form aggregates through DBs but permanently associated with BIP from degradation [59].
In addition to hCG and Na, K-ATPase, multiple other examples also indicate a “strengthening” relationship between NG and DB. Mirazimi and Svensson [105] showed that the chief role of NG on rotavirus VP7 is to facilitate correct intermolecular DB formation in dimerization. Removal of NG induced VP7 misfolding through random intermolecular DBs. Similar effects were also observed for MUC2 [56], vWF [36], meprin A [52], and hemagglutinin [47], as shown in Table 1.

5. Inhibitory Relationship

The hemagglutinin-neuraminidase (HN) glycoprotein of Newcastle disease virus (NDV) is responsible for virus attachment to host cell receptors, thereby initiating infection [4]. The HN protein is a type II membrane protein containing six potential NG sites: Asn119, Asn341, Asn433, Asn481, Asn508, and Asn538 [45]. Among them, only four (Asn119, Asn341, Asn433, Asn481) are utilized for NG [106]. The protein also has 13 cysteine residues in the ectodomain [106], as summarized in Table 1. The cysteine residue closest to the membrane anchor (Cys123) is involved in an intermolecular DB [107,108], while the other 12 cysteine residues form intramolecular DBs [107].
McGinnes and Morrison found that intramolecular DBs might play a critical role in the usage of glycosylation sites [107]. They explored whether DB formation could be a determinant of the two unused glycosylation sites, Asn508 (site 5) and Asn538 (site 6), in HN protein [45]. Removing Cys531–Cys542 flanking the unused glycosylation site Asn538 by mutation or DTT promoted the NG of Asn538 for an efficiency of 39–59% and 26–27%, respectively [45]. The successful NG was supported by the deglycosylation analysis with endo H. Under similar conditions, the usage of the non-glycosylated site 5, Asn508, which is far from any DB, was not improved. Together, these results suggest that the glycosylation of Asn538 is under steric hindrance by the DB in the vicinity [45], whereas the non-glycosylated Asn508 could be caused by other factors not related to DBs [45].
Another study investigating the lack of sequon utilization in tissue-type plasminogen activator (t-PA) reported similar findings that folding and DB formation of t-PA negatively impact the extent of core N-glycosylation [33]. As a result, they suggested that variable usage of glycosylation sites could be caused by the transient accessibility and appropriate orientation of the sequon relative to the transferase or dolichol-linked donor in a folding event [33].
Human sodium bicarbonate cotransporter 1, NBCe1 (SLC4A4 gene), is an electrogenic sodium/bicarbonate cotransporter localized in the plasma membrane [4]. The malfunction of this gene is related to a series of diseases in the kidney, eye, ear, brain, and tooth. All SLC4 Na+-coupled transporters are multipass transmembrane proteins containing a large extracellular loop (EL-3) with multiple NG consensus sites and four highly conserved cysteines [109]. NBCe1-A, one of the three variants, is a homodimer, and its two EL-3 loops form unique conformations that are potentially critical to the function of the protein [28]. In the EL-3 loop of NBCe1-A, two sequons are glycosylated (Asn597 and Asn617) but not Asn592, and four conserved cysteines form two intramolecular DBs (Cys583–Cys585 and Cys617–Cys642), as shown in Figure 3 [28].
In a detailed study evaluating the interplay between DBs and NG to define the EL-3 loop topology in NBCe1, it was found that the two EL-3 loops of the dimer formed a unique clove conformation [28]. This conformation was “finely tuned” by glycosylation [28]. In the absence of Cys583–Cys585 or the two NG sites, the third NG site, Asn592, became glycosylated. With glycans, the two DBs were deeply buried from the external surface of the EL-3 loop, which can sustain DDT-induced denaturation and enzymatic digestion under basic conditions. Losing both DBs and NG made the loop adopt an extended structure that could not be recognized by the designated antibody and was susceptible to chymotrypsin digestion [28]. Instead of considering the steric hindrance between DBs and NG at Asn592, the authors hypothesized that Asn592 was originally glycosylated at the nascent polypeptide chain of NBCe1-A and later removed when DBs and other glycosylation sites were formed [28]. Removing NG did not affect the formation of two DBs; however, an additional removal of one cysteine in the DBs by mutagenesis promoted the formation of intermolecular DBs in the homodimer, which maintained transport function [28]. A complex relationship must exist between NG and DBs in determining the final folding of EL-3 during NBCe1-A protein maturation; however, no kinetic experiments were performed to monitor protein folding, and ER maturation was not specifically probed. It is, therefore, difficult to elucidate how ER resident enzymes facilitate these processes. The study, on the other hand, had systematic structural delineation by a combinatorial mutation of all four cysteines in two DBs for a total of 12 mutants.

6. Independent Relationship

Envelope glycoprotein 160 (gp160) on human immunodeficiency virus (HIV) is critical for viral binding to the CD4 receptor and fusion with CD4+ cells. The precursor gp160 needs to be cleaved to gp120 and gp41 to activate the binding domain on gp120 with CD4. A study on the linkage region between gp120 and gp41, which is also the future binding site of gp120 to CD4, suggested that DBs and NG in this region function independently [27]. The relative position between NG and DBs in this region is shown in Figure 3. Cys402 and Cys429 are both located in the linker region but form separate DBs, of which Cys402 is critical for cleavage. Mutation of Cys402 not only prevented the cleavage but also affected the transport of gp160 and the future binding of gp120 to CD4+ cells [110,111]. Around Cys402, there are two occupied NG sites Asn390 and Asn447. Mutating these NG sites did not affect disulfide bonding through Cys402 or the relevant functions, suggesting an independent relationship between DBs and NG.
In another study of the 25 kD extracellular matrix protein chondromodulin-I (ChM-I), NG was critical in its solubility but had no effect on DBs [69]. ChM-I is a secreted protein and has two separate domains, in which the hydrophilic N-terminal domain is heavily glycosylated by one N-glycan and two O-glycans, whereas the hydrophobic C-terminal domain harbors four DBs. As the two domains are separated, the removal of either the NG or the N-terminal domain seems to have no effect on the formation of DBs in the C-terminal domain, as shown in Figure 3.

7. Unknown Relation

For most of our searched studies that concerned both DBs and NG, the exact relationship between the two PTMs was not experimentally examined. Half of these studies focused on experimental mapping of their sites without functional studies. One-third of the remaining studies only predicted the potential DBs and NG by sequence alignment or computational modeling without experimental data. For the articles that did examine the functions of both modifications, many of them did not study or discuss their interactions but rather examined them separately. For a very small number of papers, the potential interactions were hypothesized but not experimentally verified.
For example, a very nice study investigated the role of NG and DB in the rat G protein-coupled receptor class C, group 6, member A (GPRC6A) [112], a widely expressed GPCR that functions importantly in many diseases ranging from metabolic syndrome to cancer [113,114]. This protein is a class C GPCR with a large N-terminal extracellular domain (ECD), which contains a Venus-flytrap (VFT) domain and a cysteine-rich domain (CRD) [4]. The VFT domain is for ligand binding, and the CRD domain is for signal transfer [112].
It was observed that the ECD domain of GPRC6A consists of nine sequons [112]. Only seven asparagine residues carry N-glycans. Five of them are in the VFT domain, and Asn555 and Asn567 are located in the CRD [112]. The VFT domain also has two conserved cysteines (Cys122 and Cys131), whereas the CRD domain has nine conserved cysteines, eight of which form intra-CRD DBs [113]. Through analysis of different mutants by SDS-PAGE, it was found that Asn555 is important for protein surface expression and that Asn567 regulates receptor function. Furthermore, from the studies of two cysteines, Cys122 and Cys131, C131 contributed to the formation of a homodimer through an intermolecular disulfide bridge [112], and Cys122 contributed to the interdomain DB between VFT and CRD [115]. Mutation of C131A abolished the intermolecular DB and homodimer formation but did not impair receptor surface expression and its function, whereas mutation of C122A was responsible for the lowered signal response (40%) and higher (50%) surface expression [112]. This result suggested that the C122A mutation causes certain conformational changes. Not only is Cys122 next to Asn121, but the DB between CRD and VFT domains can also be largely shaped by the seven N-glycans carried by these two domains. It is likely that NG plays a role in the potential conformation changes or intermolecular DB formation; however, no experiments or discussion were presented on the relationships between NG and cysteine disulfide bridges or cysteines in the paper.
Another study explored the role of the conserved cysteines and NG sites among all alphaherpesviruses such as herpes simplex virus 1 (HSV-1) in virus production and membrane fusion by single- and double-site directed mutagenesis [116]. Glycoprotein K (gK) is a conserved virion protein in all alphaherpesviruses [117]. The N-terminal extracellular domain of gK is important for HSV-1 to enter neurons via axonal termini. This domain contains two conserved NG sites at Asn48 and Asn58 and four conserved cysteines for two potential disulfide pairs of Cys37–Cys114 and Cys82–Cys243 according to single-cysteine mutation and computational modeling [116].
It was found that viruses lacking Asn58 or lacking both sites (Asn48, Asn58) had enhanced fusion [116]. Interestingly, deletion of Cys37 or Cys114 led to a gK-null phenotype of few plaques, whereas mutation of Cys82 or Cys243 caused enhanced cell fusion. The authors provided an extensive discussion on the potential interactions between NG and DB on the basis of the known studies and hypothesized that the removal of NG at Asn58 could displace the DB formation, as the deletion of the Cys82–Cys243 disulfide recapitulated a similar fusion phenotype of Asn58A. However, the authors did not further verify this hypothesis, such as examining the presence of DBs through gel shift assays, labeling assays for free thiols, or MS characterization. Therefore, the authors in the end did not entail the specific relationship more than stating the presence of “a potentially important relationship” [116].
Related to the ongoing COVID-19 pandemic, the immunogen SARS-CoV-2 spike protein and its endogenous binding target ACE2 are both heavily glycosylated with numerous DBs. The SARS-CoV-2 S protein has a total of 22 sequons that to various extents are all glycosylated [118,119,120,121,122,123,124,125], seven O-glycosylations [118,125], and 40 cysteines with 15 DBs [118]. Similarly, ACE2 was mapped to have seven NG sites [36,125], one O-glycosylation [125], and four DBs [126,127]. According to mutations, molecular dynamics simulations of protein structures, and sequence alignment studies, eliminating certain DBs or NG on both ACE2 and SARS-CoV-2 S proteins can alter binding affinity to each other and change virus infectivity. For example, Cys480–Cys488 is considered the most important pair in the receptor-binding domain (RBD) of SARS-CoV-2 S proteins, and this pair participates in binding to the N-terminal of the host receptor that forms a stable SARS-COV-2 and ACE2 complex [126,127,128]. In addition, Cys133–Cys141 of ACE2 is responsible for making the loop at dimer interference [76,128] and is predicted to be crucial for making interactions with the spike protein of SARS-CoV-2 [127]. Deletion of Asn90 glycosylation of ACE2 increased the binding to S proteins, while removal of Asn322 of ACE2 decreased virus binding and infection [125,129]. From the perspective of SARS-CoV-2 S protein, the Ser309 neutralizing antibody binds Asn234 glycosylated RBD [32], and double mutations of N165A/N234A [35] and N331Q/N343Q [53] in S protein both reduced the binding between the immunogen and the receptor. Despite the extensive and rapid studies of NG and DBs in S proteins and ACE2 in the past 2 years, no studies have examined the relationship between DBs and NG in these two proteins. This phenomenon clearly indicates the severe understudy in this important field.

8. Common Methods

Successful studies of the relationships between DB and NG relied on suitable tools. Table 2 and Table 3 summarize common methods used in studies of NG and DB, respectively.
Table
Table 2. Summary of methodologies for the identification and structural analysis of N-glycosylation in proteins.
Table 2. Summary of methodologies for the identification and structural analysis of N-glycosylation in proteins.
NG detectionStaining procedures [130]
  • Resolve protein on SDS-PAGE and stain the gel for glycoproteins
Affinity-based methods [130]
  • Saccharide-binding protein (lectin-based)
  • Enzyme-based methods
  • Antibody-based methods
NMR spectroscopy [131,132]
X-ray crystallography [133]
Circular dichroism (CD) spectroscopy [64]
NG structural analysisRequires N-glycan removal prior to further analysis which can be achieved byChromatography
  • Enzymatic removal [130,134]
  • PNGase F
  • Endo-H and peptide: N-glycanase [67]
  • Chemical removal [130]
  • β-Elimination
  • Alkaline borohydride [135]
  • Hydrazinolysis
  • Weak anion exchange (WAX) [136]
  • Gel filtration
  • High-performance anion-exchange chromatography with pulsed amperometric detection (HPAEC-PAD) [137]
  • Normal-phase high-performance liquid chromatography (NP-HPLC) [138]
  • Reverse-phase HPLC (RP-HPLC) [139]
  • Mass spectrometry [140,141,142,143,144,145,146]
  • MALDI-MS, ESI-MS, or LC–ESI-MS [147]
  • LC–MS/MS [148]
  • Targeted MS/MS [149]
NG functional analysisChemical tools: inhibitors of glycosyltransferases and glycosidases (in vivo) [150]
  • Tunicamycin
  • Plant alkaloids: australine, castanospermine [151], deoxynojirimycin [151], deoxymannojirimycin, kifunensine, swainsonine, and mannostatin A
Physical tools: adjust temperature, ATP, pH, etc.
Site-directed mutagenesis
Genetic glyco-engineering [152]
  • Involves introduction of heterologous glycosylation machinery or inactivation of endogenous enzymes.
Table
Table 3. Summary of the methodologies for the detection and analysis of disulfide bonds in proteins.
Table 3. Summary of the methodologies for the detection and analysis of disulfide bonds in proteins.
Quantify the amount of unbound cysteine residuesChemical labeling and spectroscopic detection [153]
  • Ellman assay
  • N-(1-pyrenyl)maleimide (NPM) labeling
Reduction methodsReducing enzymes [153]
  • 2-Mercaptoethanol (ME)
  • Dithiothreitol (DTT)
  • Tris(2-carboxyethyl)phosphine (TCEP)
  • Tris(2-hydroxyethyl)phosphine (THP)
Detection/Analysis of DBEdman degradation sequencing [154]
NMR spectroscopy [155,156]
X-ray crystallography [157]
2-Nitro-5-thiosulfobenzoate (NTSB) assay [158,159]
  • Electrophoretic methods [153,160]
  • Capillary electrophoresis sodium dodecyl sulfate (CE-SDS)
  • Nonreducing SDS polyacrylamide gel electrophoresis (SDS-PAGE) [160,161]
  • Diagonal gel electrophoresis [162]
Mass spectrometry approaches:
Front-end separation [153,163,164,165,166,167,168,169]		Mass spectrometry approaches:
Fragmentation types
  • LC–MS/MS
  • LC–ESI-MS/MS
  • ETD-MS/MS
  • ESI-MS/MS
  • MS/MS/MS
  • Activated ion ETD (AI-ETD) [170,171]
  • CID [172,173]
  • HCD [174]
  • EThcD [175,176]
  • Ultraviolet photodissociation (UVPD)–MS [177]
Detect structural changesPartial proteolysis by enzymes such as trypsin and pepsin
Functional assays
  • Epitope tags such as haemagglutinin, hexahistidine, V5, FLAG (visualized using antibodies)
  • Biotin tags
Site-directed mutagenesis
For both modifications, conventional analytical methods include NMR [155,156], X-ray crystallography [157], cryoEM, CD for structure analysis, Edman degradation [154] and mass spectrometry (MS) for sequencing analysis, and electrophoresis for protein migration mobility analysis [153,160]. Gel shift assay by electrophoresis is a readily accessible and effective analytical method widely employed to study both modifications. Electrophoretic methods such as SDS-PAGE and capillary electrophoresis under reducing and nonreducing conditions are simple assays for primary analysis of the overall DBs in a protein. By comparing the differential electrophoretic mobility, researchers can deduce the presence of DBs. In particular, diagonal electrophoresis, which conducts sequential nonreducing and reducing electrophoresis in two orthogonal dimensions of the same sample, allows easy identification of DBs [162]. For NG, enzymes and chemical removal of sugar moieties can be identified by mobility shifts in SDS-PAGE. Due to the size of N-glycans, their multiplicity can also be resolved by SDS-PAGE from the corresponding ladder-shaped protein bands. Combined with pulse-chasing using isotopes such as [35S]Met, the kinetics of the formation, processing, maturation, and degradation of these modifications are often monitored by the gel shift assay.
X-ray analysis of N-glycosylation can be challenging due to the heterogenous glycoforms that impede diffraction-quality crystallization. Nevertheless, the 3D structures of N-glycans in glycoproteins have been growing in PDB [178]. Various methods have been explored, including engineering the host cell glycosylation machinery to produce homogenous N-glycan-modified proteins for X-ray crystallography [133]. Many NMR methods have been developed to study the structure of N-glycans, intact N-glycoproteins, N-glycoprotein complexes, and model N-glycosylated peptides [131,132]. Synthetic model glycopeptides have unique advantages in terms of forming well-defined sequences and structures to interrogate their conformational effect in great detail under NMR [132]. In particular, the relations between NG and DBs have been characterized using synthetic model peptides, such as those derived from nicotinic acetylcholine receptor and prion protein [12,58]. In addition, MS has also recently been developed to decipher glycoprotein complex interactions through N-glycans, in which various glycoforms can be examined individually [179].
For molecular engineering, mutagenesis is another common method that is widely used to accurately pinpoint the site of modifications and to study the structural and functional consequence upon complete, permanent, and selective removal of some or all of these PTMs. The most frequently used mutagenesis is single-amino-acid substitution, even though deletion of one or a chain of amino acids exists. It is worth mentioning the choice of amino-acid replacements. Commonly, cysteines are mutated to alanines (A) or serines (S), whereas asparagines are replaced by aspartic (D) and glutamic acids (E) or glutamines (Q), even though some studies replaced threonine (T)/serine (S) in the sequons to abolish NG.
Chemical removal or tagging of DBs and NG is also frequently employed to identify their presence and functions. For DBs, reducing agents can be used to disrupt the covalent bond, and thiol-reactive chemical groups can modify the free thiols to distinguish them from those that are occupied by DBs. Either a gel shift assay or MS can be employed downstream to identify changes in these chemical perturbations. Chemical removal of NG can be catalyzed by enzymes. Using enzymatic selectivity, different glycans can be readily distinguished. For example, according to the degree of processing, N-glycans have three types, i.e., high mannose, complex, and hybrid N-glycans. Endoglycosidase (endo H) cannot cleave complex N-glycans, yet N-glycosidase F (PNGase F) can [134]. Therefore, the two enzymes are frequently used to delineate the type of N-glycans. Chemical removal can also be facilitated by small molecules, such as base-assisted beta-elimination and hydrazinolysis [130], which are less selective than enzymatic reactions.
For structural characterization upon changes by DBs and NG, in addition to the instrumental approaches mentioned above, several biochemical approaches have also been developed. First, enzymes, particularly peptidase/protease, have been used to examine the overall structures of proteins. Both trypsin and pepsin were used to assess the compactness of the protein folding according to digestion efficiency. Second, for specific epitopes of a protein, antibodies were developed for rapid and specific recognition.
In addition to the above in vitro analysis methods, in vivo tools to interrogate the pathways in the formation and processing of the two PTMs were made available. A selective perturbation to the pathways can be achieved through molecularly engineered knockout, knockdown, or knock-in of a particular enzyme or chaperone. Targeted changes can also be elicited through pharmacological inhibition by small molecules. Less selective conditions, such as dithiothreitol (DTT) and 2-mercaptoethanol (2-ME) treatments, were also used to induce a global reduction of all DBs in vivo.
One important aspect of characterizing the relationships between NG and DBs is to examine the kinetics of protein maturation in the secretory pathway, as well as the kinetics of enzymatic reactions that regulate NG and DB formation and processing. Due to the migration shift in the gel after the formation of N-glycans and DBs, the protein maturation kinetics have often been examined by pulse-chase gel-shift assays. Regarding the kinetics of glycoenzymes with oxidoreductase activities, available studies are very limited. Historically, radioisotope labeling was used to probe enzymatic reactions in vitro to build predictive models for N-glycosylation [180,181]. Later, the MS characterization of glycans with and without stable isotope labeling was adopted for safer measurements [182,183,184]. Recently, targeted MS was developed to quantify the kinetics of stable isotope-labeled glycopeptides for more accurate modeling, in which not only the rates of glycan synthesis/processing but also the amino-acid sequences around glycosylation sites were monitored for “cell, enzyme, and glycosylation” site-specific analysis [23].
Among all the techniques, we would like to highlight MS in the characterization of the two modifications. With the advent of modern instrumentation, the method measures the mass of peptides down to sub-ppm accuracy and attomole sensitivity. The instrument holds promise for sequencing, i.e., structurally resolved, complex biological samples including all proteins, peptides, nucleic acids, carbohydrates, lipids, and metabolites within [151]. It has been playing ever increasingly important roles in deconvoluting the structures of proteins, including their DBs and glycosylation. In recent years, the application of the technique has been moved from studying one protein at a time to studying a sub-proteome by enrichment through a native moiety or chemical tagging. For example, glycoproteins and glycopeptides can be enriched by lectins or hydrophilic metals, charcoal, organic sorbents, or chemical bonding to sorbents through hydrazone and boronic acid diesters and subsequently analyzed by MS for identification, quantification, or structural interpretation [185,186,187]. Similarly, the thiol group has been a conventional substrate for MS analysis either at the individual protein level or at the proteome level using methods such as ICAT [188]. With both label- and label-free quantitation rapidly developing, MS characterization holds the potential both for steady-state analyses and for kinetic interrogations in modeling biological processes. Several reviews are available that summarize the field of MS characterization in either DBs [166,188] or NG [185,186,187].

9. Final Remarks

It is widely accepted that both NG and BDs can affect the folding, maturation, trafficking, and degradation of host proteins; however, how to effectively control and engineer these PTMs in individual proteins for disease prevention and treatments, respectively, remains in its infancy. Unlike existing reviews on the mechanisms of enzymes functioning in NG and DB formation pathways, our study focused on the relationships of the two PTMs discovered in individual proteins. After reviewing more than 500 papers that investigated both modifications in one protein, we noticed that most studies only mapped their positions or studied their functions separately. Fewer than 100 articles have experimentally addressed the relationships between the two PTMs. We summarized the studied proteins in Table 1.
From the intriguing cooperation observed between N-glycoenzymes and oxidoreductases in the ER, it is envisaged that close relationships between NG and DBs are anticipated to widely exist in membrane and secreted proteins. Compared to the total human proteins annotated in UniProt with DBs and NGs, the proteins in Table 1 comprise less than 2%. As a result, for the most studied STT3B and STT3A substrate preferences, their complete responsive sites in all substrate proteins are still elusive. A recent discovery-based study carried out by proteomics on STT3A and STT3B substrate pools uncovered some interesting proteins [75] that could not be explained by the known mechanisms. During CNX/CRT-chaperoned N-glycoprotein folding, oxidoreductases are involved. It is known that there are ERp57 obligate and ERp57 facultative substrates [189]. ERp72 was discovered to be the alternative enzyme that acts on facultative substrates in the absence of ERp57; however, it is unclear how the obligate and facultative substrates are determined in vivo. For other complexes, such as EDEMs in ERAD, their protein substrates are just starting to emerge.
Even though relatively few proteins have been studied on the mutual relations between NG and DBs as exemplified in Figure 4, they are important disease biomarkers and therapeutic targets. Understanding the function and regulation of these PTMs is, therefore, critically important in disease treatment and prevention. Most of the studies used mutagenesis to remove one or both PTMs for structural and functional effects; however, a few studies introduced novel PTMs into proteins to engineer protein-based drugs/vaccines for better stability and efficacy [48,190,191]. In addition, knowledge obtained from studying these modifications can help researchers gain insights into early disease diagnosis and prevention [50,58].
Due to the diverse structures possessed by individual proteins and the complex relationships, it is important to examine the entire sub-proteome to gain comprehensive knowledge. The current intriguing interactions between the two PTMs derived from model proteins should serve as an encouraging start for an exciting field. We believe that the MS-led new generation of high-throughput high-accuracy analyses can quickly move this field forward. Lastly, we hope that this review will encourage future studies to investigate the relationship between NG and DBs and to better disclose their hidden linkages in the remaining 98% of the proteins for novel insights into their structural and functional roles.

Author Contributions

B.S. conceived the idea; T.B. and R.K. (SARS-CoV-2 related) performed the literature search; T.B. analyzed the results; D.P. generated Figure 3; T.B., R.K. (SARS-CoV-2 related) and B.S. wrote; and everyone reviewed the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

This research received no external funding.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Acknowledgments

This work was supported by the National Sciences and Engineering Research Council of Canada, RGPIN06073 (B.S), the Canada Foundation of Innovation (B.S.), the British Columbia Knowledge Development Fund (B.S.), and the Simon Fraser University work study program (T.B., R.K. and D.P.).

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Adams, B.M.; Oster, M.E.; Hebert, D.N. Protein Quality Control in the Endoplasmic Reticulum. Protein J. 2019, 38, 317–329. [Google Scholar] [CrossRef] [PubMed]
  2. Grek, C.; Townsend, D.M. Protein Disulfide Isomerase Superfamily in Disease and the Regulation of Apoptosis. Endoplasmic Reticulum Stress Dis. 2014, 1, 4–17. [Google Scholar] [CrossRef] [PubMed]
  3. Reily, C.; Stewart, T.J.; Renfrow, M.B.; Novak, J. Glycosylation in health and disease. Nat. Rev. Nephrol. 2019, 15, 346–366. [Google Scholar] [CrossRef] [PubMed]
  4. UniProt Consortium, T. UniProt: The universal protein knowledgebase. Nucleic Acids Res. 2018, 46, 2699. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Braakman, I.; Hoover-Litty, H.; Wagner, K.R.; Helenius, A. Folding of influenza hemagglutinin in the endoplasmic reticulum. J. Cell Biol. 1991, 114, 401–411. [Google Scholar] [CrossRef]
  6. Chen, W.; Helenius, J.; Braakman, I.; Helenius, A. Cotranslational folding and calnexin binding during glycoprotein synthesis. Proc. Natl. Acad. Sci. USA 1995, 92, 6229–6233. [Google Scholar] [CrossRef] [Green Version]
  7. Hebert, D.N.; Zhang, J.X.; Chen, W.; Foellmer, B.; Helenius, A. The number and location of glycans on influenza hemagglutinin determine folding and association with calnexin and calreticulin. J. Cell Biol. 1997, 139, 613–623. [Google Scholar] [CrossRef]
  8. Wakabayashi, K.; Nakagawa, H.; Tamura, A.; Koshiba, S.; Hoshijima, K.; Komada, M.; Ishikawa, T. Intramolecular disulfide bond is a critical check point determining degradative fates of ATP-binding cassette (ABC) transporter ABCG2 protein. J. Biol. Chem. 2007, 282, 27841–27846. [Google Scholar] [CrossRef] [Green Version]
  9. Patel, C.; Saad, H.; Shenkman, M.; Lederkremer, G.Z. Oxidoreductases in Glycoprotein Glycosylation, Folding, and ERAD. Cells 2020, 9, 2138. [Google Scholar] [CrossRef]
  10. Chang, V.T.; Crispin, M.; Aricescu, A.R.; Harvey, D.J.; Nettleship, J.E.; Fennelly, J.A.; Yu, C.; Boles, K.S.; Evans, E.J.; Stuart, D.I.; et al. Glycoprotein structural genomics: Solving the glycosylation problem. Structure 2007, 15, 267–273. [Google Scholar] [CrossRef] [Green Version]
  11. Hanson, S.R.; Culyba, E.K.; Hsu, T.L.; Wong, C.H.; Kelly, J.W.; Powers, E.T. The core trisaccharide of an N-linked glycoprotein intrinsically accelerates folding and enhances stability. Proc. Natl. Acad. Sci. USA 2009, 106, 3131–3136. [Google Scholar] [CrossRef] [Green Version]
  12. O’Connor, S.E.; Pohlmann, J.; Imperiali, B.; Saskiawan, I.; Yamamoto, K. Probing the effect of the outer saccharide residues of N-linked glycans on peptide conformation. J. Am. Chem. Soc. 2001, 123, 6187–6188. [Google Scholar] [CrossRef]
  13. Jitsuhara, Y.; Toyoda, T.; Itai, T.; Yamaguchi, H. Chaperone-like functions of high-mannose type and complex-type N-glycans and their molecular basis. J. Biochem. 2002, 132, 803–811. [Google Scholar] [CrossRef] [PubMed]
  14. Kimura, N.; Uchida, M.; Nishimura, S.; Yamaguchi, H. Promotion of polypeptide folding by interactions with Asn-Glycans. J. Biochem. 1998, 124, 857–862. [Google Scholar] [CrossRef] [PubMed]
  15. Rickert, K.W.; Imperiali, B. Analysis of the conserved glycosylation site in the nicotinic acetylcholine receptor: Potential roles in complex assembly. Chem. Biol. 1995, 2, 751–759. [Google Scholar] [CrossRef] [Green Version]
  16. Matsusaki, M.; Kanemura, S.; Kinoshita, M.; Lee, Y.H.; Inaba, K.; Okumura, M. The Protein Disulfide Isomerase Family: From proteostasis to pathogenesis. Biochim. Et Biophys. Acta. Gen. Subj. 2020, 1864, 129338. [Google Scholar] [CrossRef]
  17. Robinson, P.J.; Bulleid, N.J. Mechanisms of Disulfide Bond Formation in Nascent Polypeptides Entering the Secretory Pathway. Cells 2020, 9, 1994. [Google Scholar] [CrossRef]
  18. Shrimal, S.; Cherepanova, N.A.; Gilmore, R. Cotranslational and posttranslocational N-glycosylation of proteins in the endoplasmic reticulum. Semin. Cell Dev. Biol. 2015, 41, 71–78. [Google Scholar] [CrossRef] [Green Version]
  19. Fu, J.; Gao, J.; Liang, Z.; Yang, D. PDI-regulated disulfide bond formation in protein folding and biomolecular assembly. Molecules 2021, 26, 171. [Google Scholar] [CrossRef]
  20. Labunskyy, V.M.; Hatfield, D.L.; Gladyshev, V.N. The Sep15 protein family: Roles in disulfide bond formation and quality control in the endoplasmic reticulum. IUBMB Life 2007, 59, 1–5. [Google Scholar] [CrossRef] [Green Version]
  21. Segawa, H.; Inakawa, A.; Yamashita, T.; Taira, H. Functional analysis of individual oligosaccharide chains of Sendai virus hemagglutinin-neuraminidase protein. Biosci. Biotechnol. Biochem. 2003, 67, 592–598. [Google Scholar] [CrossRef] [PubMed]
  22. Chen, J.Z.; Settembre, E.C.; Aoki, S.T.; Zhang, X.; Bellamy, A.R.; Dormitzer, P.R.; Harrison, S.C.; Grigorieff, N. Molecular interactions in rotavirus assembly and uncoating seen by high-resolution cryo-EM. Proc. Natl. Acad. Sci. USA 2009, 106, 10644–10648. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Arigoni-Affolter, I.; Scibona, E.; Lin, C.W.; Bruhlmann, D.; Souquet, J.; Broly, H.; Aebi, M. Mechanistic reconstruction of glycoprotein secretion through monitoring of intracellular N-glycan processing. Sci. Adv. 2019, 5, eaax8930. [Google Scholar] [CrossRef] [Green Version]
  24. Pace, N.J.; Weerapana, E. Diverse functional roles of reactive cysteines. ACS Chem. Biol. 2013, 8, 283–296. [Google Scholar] [CrossRef] [PubMed]
  25. Ohtsubo, K.; Marth, J.D. Glycosylation in cellular mechanisms of health and disease. Cell 2006, 126, 855–867. [Google Scholar] [CrossRef] [Green Version]
  26. Fewell, S.W.; Travers, K.J.; Weissman, J.S.; Brodsky, J.L. The action of molecular chaperones in the early secretory pathway. Annu. Rev. Genet. 2001, 35, 149–191. [Google Scholar] [CrossRef]
  27. Bolmstedt, A.; Hemming, A.; Flodby, P.; Berntsson, P.; Travis, B.; Lin, J.P.; Ledbetter, J.; Tsu, T.; Wigzell, H.; Hu, S.L.; et al. Effects of mutations in glycosylation sites and disulphide bonds on processing, CD4-binding and fusion activity of human immunodeficiency virus envelope glycoproteins. J. Gen. Virol. 1991, 72 Pt 6, 1269–1277. [Google Scholar] [CrossRef]
  28. Zhu, Q.; Kao, L.; Azimov, R.; Abuladze, N.; Newman, D.; Kurtz, I. Interplay between disulfide bonding and N-glycosylation defines SLC4 Na+-coupled transporter extracellular topography. J. Biol. Chem. 2015, 290, 5391–5404. [Google Scholar] [CrossRef] [Green Version]
  29. Haniu, M.; Horan, T.; Arakawa, T.; Le, J.; Katta, V.; Hara, S.; Rohde, M.F. Disulfide structure and N-glycosylation sites of an extracellular domain of granulocyte-colony stimulating factor receptor. Biochemistry 1996, 35, 13040–13046. [Google Scholar] [CrossRef]
  30. Dekker, J.; Strous, G.J. Covalent oligomerization of rat gastric mucin occurs in the rough endoplasmic reticulum, is N-glycosylation-dependent, and precedes initial O-glycosylation. J. Biol. Chem. 1990, 265, 18116–18122. [Google Scholar] [CrossRef]
  31. Yi, L.; Bozkurt, G.; Li, Q.; Lo, S.; Menon, A.K.; Wu, H. Disulfide Bond Formation and N-Glycosylation Modulate Protein-Protein Interactions in GPI-Transamidase (GPIT). Sci. Rep. 2017, 8, 45912. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  32. Vlahos, C.J.; Wilhelm, O.G.; Hassell, T.; Jaskunas, S.R.; Bang, N.U. Disulfide pairing of the recombinant kringle-2 domain of tissue plasminogen activator produced in Escherichia coli. J. Biol. Chem. 1991, 266, 10070–10072. [Google Scholar] [CrossRef]
  33. Allen, S.; Naim, H.Y.; Bulleid, N.J. Intracellular folding of tissue-type plasminogen activator. Effects of disulfide bond formation on N-linked glycosylation and secretion. J. Biol. Chem. 1995, 270, 4797–4804. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Cruz, M.A.; Handin, R.I.; Wise, R.J. The interaction of the von Willebrand factor-A1 domain with platelet glycoprotein Ib/IX. The role of glycosylation and disulfide bonding in a monomeric recombinant A1 domain protein. J. Biol. Chem. 1993, 268, 21238–21245. [Google Scholar] [CrossRef]
  35. Marti, T.; Rosselet, S.J.; Titani, K.; Walsh, K.A. Identification of disulfide-bridged substructures within human von Willebrand factor. Biochemistry 1987, 26, 8099–8109. [Google Scholar] [CrossRef] [PubMed]
  36. McKinnon, T.A.; Goode, E.C.; Birdsey, G.M.; Nowak, A.A.; Chan, A.C.; Lane, D.A.; Laffan, M.A. Specific N-linked glycosylation sites modulate synthesis and secretion of von Willebrand factor. Blood 2010, 116, 640–648. [Google Scholar] [CrossRef] [Green Version]
  37. Feng, W.; Huth, J.R.; Norton, S.E.; Ruddon, R.W. Asparagine-linked oligosaccharides facilitate human chorionic gonadotropin beta-subunit folding but not assembly of prefolded beta with alpha. Endocrinology 1995, 136, 52–61. [Google Scholar] [CrossRef]
  38. Feng, W.; Matzuk, M.M.; Mountjoy, K.; Bedows, E.; Ruddon, R.W.; Boime, I. The asparagine-linked oligosaccharides of the human chorionic gonadotropin beta subunit facilitate correct disulfide bond pairing. J. Biol. Chem. 1995, 270, 11851–11859. [Google Scholar] [CrossRef] [Green Version]
  39. Moriwaki, T.; Suganuma, N.; Furuhashi, M.; Kikkawa, F.; Tomoda, Y.; Boime, I.; Nakata, M.; Mizuochi, T. Alteration of N-linked oligosaccharide structures of human chorionic gonadotropin beta-subunit by disruption of disulfide bonds. Glycoconj. J. 1997, 14, 225–229. [Google Scholar] [CrossRef]
  40. Kuglstatter, A.; Stihle, M.; Neumann, C.; Muller, C.; Schaefer, W.; Klein, C.; Benz, J. Structural differences between glycosylated, disulfide-linked heterodimeric Knob-into-Hole Fc fragment and its homodimeric Knob-Knob and Hole-Hole side products. Protein Eng. Des. Sel. PEDS 2017, 30, 649–656. [Google Scholar] [CrossRef]
  41. Lipari, F.; Herscovics, A. Role of the cysteine residues in the alpha1,2-mannosidase involved in N-glycan biosynthesis in Saccharomyces cerevisiae. The conserved Cys340 and Cys385 residues form an essential disulfide bond. J. Biol. Chem. 1996, 271, 27615–27622. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  42. Flahaut, M.; Pfister, C.; Rossier, B.C.; Firsov, D. N-Glycosylation and conserved cysteine residues in RAMP3 play a critical role for the functional expression of CRLR/RAMP3 adrenomedullin receptor. Biochemistry 2003, 42, 10333–10341. [Google Scholar] [CrossRef]
  43. Walker, A.K.; Soo, K.Y.; Levina, V.; Talbo, G.H.; Atkin, J.D. N-linked glycosylation modulates dimerization of protein disulfide isomerase family A member 2 (PDIA2). FEBS J. 2013, 280, 233–243. [Google Scholar] [CrossRef] [PubMed]
  44. Vidal, S.; Mottet, G.; Kolakofsky, D.; Roux, L. Addition of high-mannose sugars must precede disulfide bond formation for proper folding of Sendai virus glycoproteins. J. Virol. 1989, 63, 892–900. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. McGinnes, L.W.; Morrison, T.G. Disulfide bond formation is a determinant of glycosylation site usage in the hemagglutinin-neuraminidase glycoprotein of Newcastle disease virus. J. Virol. 1997, 71, 3083–3089. [Google Scholar] [CrossRef] [Green Version]
  46. Pitt, J.J.; Da Silva, E.; Gorman, J.J. Determination of the disulfide bond arrangement of Newcastle disease virus hemagglutinin neuraminidase. Correlation with a beta-sheet propeller structural fold predicted for paramyxoviridae attachment proteins. J. Biol. Chem. 2000, 275, 6469–6478. [Google Scholar] [CrossRef] [Green Version]
  47. Daniels, R.; Kurowski, B.; Johnson, A.E.; Hebert, D.N. N-linked glycans direct the cotranslational folding pathway of influenza hemagglutinin. Mol. Cell 2003, 11, 79–90. [Google Scholar] [CrossRef]
  48. Thornlow, D.N.; Macintyre, A.N.; Oguin, T.H.; Karlsson, A.B.; Stover, E.L.; Lynch, H.E.; Sempowski, G.D.; Schmidt, A.G. Altering the Immunogenicity of Hemagglutinin Immunogens by Hyperglycosylation and Disulfide Stabilization. Front. Immunol. 2021, 12, 737973. [Google Scholar] [CrossRef]
  49. Suzuki, S.; Furuhashi, M.; Suganuma, N. Additional N-glycosylation at Asn(13) rescues the human LHbeta-subunit from disulfide-linked aggregation. Mol. Cell. Endocrinol. 2000, 160, 157–163. [Google Scholar] [CrossRef]
  50. Naessens, S.; De Zaeytijd, J.; Syx, D.; Vandenbroucke, R.E.; Smeets, F.; Van Cauwenbergh, C.; Leroy, B.P.; Peelman, F.; Coppieters, F. The N-terminal p.(Ser38Cys) TIMP3 mutation underlying Sorsby fundus dystrophy is a founder mutation disrupting an intramolecular disulfide bond. Hum. Mutat. 2019, 40, 539–551. [Google Scholar] [CrossRef] [Green Version]
  51. Arolas, J.L.; Broder, C.; Jefferson, T.; Guevara, T.; Sterchi, E.E.; Bode, W.; Stocker, W.; Becker-Pauly, C.; Gomis-Ruth, F.X. Structural basis for the sheddase function of human meprin beta metalloproteinase at the plasma membrane. Proc. Natl. Acad. Sci. USA 2012, 109, 16131–16136. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  52. Ishmael, S.S.; Ishmael, F.T.; Jones, A.D.; Bond, J.S. Protease domain glycans affect oligomerization, disulfide bond formation, and stability of the meprin A metalloprotease homo-oligomer. J. Biol. Chem. 2006, 281, 37404–37415. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  53. Liu, T.; Qian, W.J.; Gritsenko, M.A.; Camp, D.G., 2nd; Monroe, M.E.; Moore, R.J.; Smith, R.D. Human plasma N-glycoproteome analysis by immunoaffinity subtraction, hydrazide chemistry, and mass spectrometry. J. Proteome Res. 2005, 4, 2070–2080. [Google Scholar] [CrossRef] [Green Version]
  54. McCormick, L.M.; Urade, R.; Arakaki, Y.; Schwartz, A.L.; Bu, G. Independent and cooperative roles of N-glycans and molecular chaperones in the folding and disulfide bond formation of the low-density lipoprotein (LDL) receptor-related protein. Biochemistry 2005, 44, 5794–5803. [Google Scholar] [CrossRef] [PubMed]
  55. Zelcer, N.; Hong, C.; Boyadjian, R.; Tontonoz, P. LXR regulates cholesterol uptake through Idol-dependent ubiquitination of the LDL receptor. Science 2009, 325, 100–104. [Google Scholar] [CrossRef] [Green Version]
  56. Asker, N.; Axelsson, M.A.; Olofsson, S.O.; Hansson, G.C. Dimerization of the human MUC2 mucin in the endoplasmic reticulum is followed by a N-glycosylation-dependent transfer of the mono- and dimers to the Golgi apparatus. J. Biol. Chem. 1998, 273, 18857–18863. [Google Scholar] [CrossRef] [Green Version]
  57. Bell, S.L.; Xu, G.; Khatri, I.A.; Wang, R.; Rahman, S.; Forstner, J.F. N-linked oligosaccharides play a role in disulphide-dependent dimerization of intestinal mucin Muc2. Biochem. J. 2003, 373, 893–900. [Google Scholar] [CrossRef] [Green Version]
  58. Bosques, C.J.; Imperiali, B. The interplay of glycosylation and disulfide formation influences fibrillization in a prion protein fragment. Proc. Natl. Acad. Sci. USA 2003, 100, 7593–7598. [Google Scholar] [CrossRef] [Green Version]
  59. Beggah, A.T.; Jaunin, P.; Geering, K. Role of glycosylation and disulfide bond formation in the beta subunit in the folding and functional expression of Na, K-ATPase. J. Biol. Chem. 1997, 272, 10318–10326. [Google Scholar] [CrossRef] [Green Version]
  60. Laughery, M.D.; Todd, M.L.; Kaplan, J.H. Mutational analysis of alpha-beta subunit interactions in the delivery of Na, K-ATPase heterodimers to the plasma membrane. J. Biol. Chem. 2003, 278, 34794–34803. [Google Scholar] [CrossRef] [Green Version]
  61. Clogston, C.L.; Boone, T.C.; Crandall, B.C.; Mendiaz, E.A.; Lu, H.S. Disulfide structures of human interleukin-6 are similar to those of human granulocyte colony stimulating factor. Arch. Biochem. Biophys. 1989, 272, 144–151. [Google Scholar] [CrossRef]
  62. May, L.T.; Shaw, J.E.; Khanna, A.K.; Zabriskie, J.B.; Sehgal, P.B. Marked cell-type-specific differences in glycosylation of human interleukin-6. Cytokine 1991, 3, 204–211. [Google Scholar] [CrossRef]
  63. Orita, T.; Oh-eda, M.; Hasegawa, M.; Kuboniwa, H.; Esaki, K.; Ochi, N. Polypeptide and carbohydrate structure of recombinant human interleukin-6 produced in Chinese hamster ovary cells. J. Biochem. 1994, 115, 345–350. [Google Scholar] [CrossRef] [PubMed]
  64. Roman-Sosa, G.; Karger, A.; Kraatz, F.; Aebischer, A.; Wernike, K.; Maksimov, P.; Lillig, C.H.; Reimann, I.; Brocchi, E.; Keller, M.; et al. The amino terminal subdomain of glycoprotein Gc of Schmallenberg virus: Disulfide bonding and structural determinants of neutralization. J. Gen. Virol. 2017, 98, 1259–1273. [Google Scholar] [CrossRef]
  65. Mohd Yusuf, S.N.; Bailey, U.M.; Tan, N.Y.; Jamaluddin, M.F.; Schulz, B.L. Mixed disulfide formation in vitro between a glycoprotein substrate and yeast oligosaccharyltransferase subunits Ost3p and Ost6p. Biochem. Biophys. Res. Commun. 2013, 432, 438–443. [Google Scholar] [CrossRef] [Green Version]
  66. Schulz, B.L.; Stirnimann, C.U.; Grimshaw, J.P.; Brozzo, M.S.; Fritsch, F.; Mohorko, E.; Capitani, G.; Glockshuber, R.; Grutter, M.G.; Aebi, M. Oxidoreductase activity of oligosaccharyltransferase subunits Ost3p and Ost6p defines site-specific glycosylation efficiency. Proc. Natl. Acad. Sci. USA 2009, 106, 11061–11066. [Google Scholar] [CrossRef] [Green Version]
  67. Ohgomori, T.; Nanao, T.; Morita, A.; Ikekita, M. Asn54-linked glycan is critical for functional folding of intercellular adhesion molecule-5. Glycoconj. J. 2012, 29, 47–55. [Google Scholar] [CrossRef]
  68. Zhang, H.; Casasnovas, J.M.; Jin, M.; Liu, J.H.; Gahmberg, C.G.; Springer, T.A.; Wang, J.H. An unusual allosteric mobility of the C-terminal helix of a high-affinity alphaL integrin I domain variant bound to ICAM-5. Mol. Cell 2008, 31, 432–437. [Google Scholar] [CrossRef] [Green Version]
  69. Kondo, J.; Shibata, H.; Miura, S.; Yamakawa, A.; Sato, K.; Higuchi, Y.; Shukunami, C.; Hiraki, Y. A functional role of the glycosylated N-terminal domain of chondromodulin-I. J. Bone Miner. Metab. 2011, 29, 23–30. [Google Scholar] [CrossRef] [Green Version]
  70. Hoffman, R.C.; Andersen, H.; Walker, K.; Krakover, J.D.; Patel, S.; Stamm, M.R.; Osborn, S.G. Peptide, disulfide, and glycosylation mapping of recombinant human thrombopoietin from ser1 to Arg246. Biochemistry 1996, 35, 14849–14861. [Google Scholar] [CrossRef]
  71. Kato, T. Protein characteristics of thrombopoietin. Stem Cells 1996, 14 (Suppl. S1), 139–147. [Google Scholar] [CrossRef] [PubMed]
  72. Diop, N.K.; Hrycyna, C.A. N-Linked glycosylation of the human ABC transporter ABCG2 on asparagine 596 is not essential for expression, transport activity, or trafficking to the plasma membrane. Biochemistry 2005, 44, 5420–5429. [Google Scholar] [CrossRef] [PubMed]
  73. Wakabayashi-Nakao, K.; Tamura, A.; Furukawa, T.; Nakagawa, H.; Ishikawa, T. Quality control of human ABCG2 protein in the endoplasmic reticulum: Ubiquitination and proteasomal degradation. Adv. Drug Deliv. Rev. 2009, 61, 66–72. [Google Scholar] [CrossRef]
  74. Fischer, F.; Molinari, M.; Bodendorf, U.; Paganetti, P. The disulphide bonds in the catalytic domain of BACE are critical but not essential for amyloid precursor protein processing activity. J. Neurochem. 2002, 80, 1079–1088. [Google Scholar] [CrossRef] [PubMed]
  75. Cherepanova, N.A.; Venev, S.V.; Leszyk, J.D.; Shaffer, S.A.; Gilmore, R. Quantitative glycoproteomics reveals new classes of STT3A- and STT3B-dependent N-glycosylation sites. J. Cell Biol. 2019, 218, 2782–2796. [Google Scholar] [CrossRef] [Green Version]
  76. Cherepanova, N.A.; Shrimal, S.; Gilmore, R. Oxidoreductase activity is necessary for N-glycosylation of cysteine-proximal acceptor sites in glycoproteins. J. Cell Biol. 2014, 206, 525–539. [Google Scholar] [CrossRef] [Green Version]
  77. Ruiz-Canada, C.; Kelleher, D.J.; Gilmore, R. Cotranslational and posttranslational N-glycosylation of polypeptides by distinct mammalian OST isoforms. Cell 2009, 136, 272–283. [Google Scholar] [CrossRef] [Green Version]
  78. Rius, M.; Sala, L.; Chillaron, J. The role of N-glycans and the C-terminal loop of the subunit rBAT in the biogenesis of the cystinuria-associated transporter. Biochem. J. 2016, 473, 233–244. [Google Scholar] [CrossRef]
  79. Ivanenkov, V.V.; Meller, J.; Kirley, T.L. Characterization of disulfide bonds in human nucleoside triphosphate diphosphohydrolase 3 (NTPDase3): Implications for NTPDase structural modeling. Biochemistry 2005, 44, 8998–9012. [Google Scholar] [CrossRef]
  80. Qiu, Z.; Hobman, T.C.; McDonald, H.L.; Seto, N.O.; Gillam, S. Role of N-linked oligosaccharides in processing and intracellular transport of E2 glycoprotein of rubella virus. J. Virol. 1992, 66, 3514–3521. [Google Scholar] [CrossRef] [Green Version]
  81. Alhamidi, M.; Kjeldsen Buvang, E.; Fagerheim, T.; Brox, V.; Lindal, S.; Van Ghelue, M.; Nilssen, O. Fukutin-related protein resides in the Golgi cisternae of skeletal muscle fibres and forms disulfide-linked homodimers via an N-terminal interaction. PLoS ONE 2011, 6, e22968. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  82. Pal, A.; Kraetzner, R.; Gruene, T.; Grapp, M.; Schreiber, K.; Gronborg, M.; Urlaub, H.; Becker, S.; Asif, A.R.; Gartner, J.; et al. Structure of tripeptidyl-peptidase I provides insight into the molecular basis of late infantile neuronal ceroid lipofuscinosis. J. Biol. Chem. 2009, 284, 3976–3984. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  83. Wujek, P.; Kida, E.; Walus, M.; Wisniewski, K.E.; Golabek, A.A. N-glycosylation is crucial for folding, trafficking, and stability of human tripeptidyl-peptidase I. J. Biol. Chem. 2004, 279, 12827–12839. [Google Scholar] [CrossRef] [Green Version]
  84. Chen, R.; Jiang, X.; Sun, D.; Han, G.; Wang, F.; Ye, M.; Wang, L.; Zou, H. Glycoproteomics analysis of human liver tissue by combination of multiple enzyme digestion and hydrazide chemistry. J. Proteome Res. 2009, 8, 651–661. [Google Scholar] [CrossRef]
  85. Guhaniyogi, J.; Sohar, I.; Das, K.; Stock, A.M.; Lobel, P. Crystal structure and autoactivation pathway of the precursor form of human tripeptidyl-peptidase 1, the enzyme deficient in late infantile ceroid lipofuscinosis. J. Biol. Chem. 2009, 284, 3985–3997. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  86. Wollscheid, B.; Bausch-Fluck, D.; Henderson, C.; O’Brien, R.; Bibel, M.; Schiess, R.; Aebersold, R.; Watts, J.D. Mass-spectrometric identification and relative quantification of N-linked cell surface glycoproteins. Nat. Biotechnol. 2009, 27, 378–386. [Google Scholar] [CrossRef] [Green Version]
  87. Koch, M.; Stronge, V.S.; Shepherd, D.; Gadola, S.D.; Mathew, B.; Ritter, G.; Fersht, A.R.; Besra, G.S.; Schmidt, R.R.; Jones, E.Y.; et al. The crystal structure of human CD1d with and without alpha-galactosylceramide. Nat Immunol 2005, 6, 819–826. [Google Scholar] [CrossRef]
  88. Vallee, F.; Lipari, F.; Yip, P.; Sleno, B.; Herscovics, A.; Howell, P.L. Crystal structure of a class I alpha1,2-mannosidase involved in N-glycan processing and endoplasmic reticulum quality control. EMBO J. 2000, 19, 581–588. [Google Scholar] [CrossRef] [Green Version]
  89. Borg, N.A.; Wun, K.S.; Kjer-Nielsen, L.; Wilce, M.C.; Pellicci, D.G.; Koh, R.; Besra, G.S.; Bharadwaj, M.; Godfrey, D.I.; McCluskey, J.; et al. CD1d-lipid-antigen recognition by the semi-invariant NKT T-cell receptor. Nature 2007, 448, 44–49. [Google Scholar] [CrossRef]
  90. Honer, J.; Niemeyer, K.M.; Fercher, C.; Diez Tissera, A.L.; Jaberolansar, N.; Jafrani, Y.M.A.; Zhou, C.; Caramelo, J.J.; Shewan, A.M.; Schulz, B.L.; et al. TorsinA folding and N-linked glycosylation are sensitive to redox homeostasis. Biochim. Et Biophys. Acta. Mol. Cell Res. 2021, 1868, 119073. [Google Scholar] [CrossRef]
  91. Kustedjo, K.; Bracey, M.H.; Cravatt, B.F. Torsin A and its torsion dystonia-associated mutant forms are lumenal glycoproteins that exhibit distinct subcellular localizations. J. Biol. Chem. 2000, 275, 27933–27939. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  92. Scott, D.C.; Schekman, R. Role of Sec61p in the ER-associated degradation of short-lived transmembrane proteins. J. Cell Biol. 2008, 181, 1095–1105. [Google Scholar] [CrossRef] [PubMed]
  93. Nakahara, M.; Koyama, T.; Nakazawa, F.; Nishio, M.; Shibamiya, A.; Hirosawa, S. Gradually glycosylated protein C mutants (Arg178Gln and Cys331Arg) are degraded by proteasome after mannose trimming. Thromb Haemost 2004, 92, 1284–1290. [Google Scholar] [CrossRef] [PubMed]
  94. Zhao, Y.; Zhang, Q.; Yuan, L.; Zhang, R.; Li, L. N-glycosylation and dimerization regulate the PtrMAN6 enzyme activity that may modulate generation of oligosaccharide signals. Plant Signal Behav. 2013, 8, e26956. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  95. Gardner, T.G.; Kearse, K.P. Modification of the T cell antigen receptor (TCR) complex by UDP-glucose:glycoprotein glucosyltransferase. TCR folding is finalized convergent with formation of alpha beta delta epsilon gamma epsilon complexes. J. Biol. Chem. 1999, 274, 14094–14099. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  96. Jia, W.; Lu, Z.; Fu, Y.; Wang, H.P.; Wang, L.H.; Chi, H.; Yuan, Z.F.; Zheng, Z.B.; Song, L.N.; Han, H.H.; et al. A strategy for precise and large scale identification of core fucosylated glycoproteins. Mol Cell Proteom. 2009, 8, 913–923. [Google Scholar] [CrossRef] [Green Version]
  97. Thaysen-Andersen, M.; Mysling, S.; Hojrup, P. Site-specific glycoprofiling of N-linked glycopeptides using MALDI-TOF MS: Strong correlation between signal strength and glycoform quantities. Anal. Chem. 2009, 81, 3933–3943. [Google Scholar] [CrossRef]
  98. Frank, M.; Walker, R.C.; Lanzilotta, W.N.; Prestegard, J.H.; Barb, A.W. Immunoglobulin G1 Fc domain motions: Implications for Fc engineering. J. Mol. Biol. 2014, 426, 1799–1811. [Google Scholar] [CrossRef] [Green Version]
  99. Vance, B.A.; Bennett, M.J.; Ward, Y.; Gress, R.G.; Kearse, K.P. Distinct but dispensable N-glycosylation of human CD69 proteins. Arch. Biochem. Biophys. 1999, 368, 214–220. [Google Scholar] [CrossRef]
  100. Vance, B.A.; Wu, W.; Ribaudo, R.K.; Segal, D.M.; Kearse, K.P. Multiple dimeric forms of human CD69 result from differential addition of N-glycans to typical (Asn-X-Ser/Thr) and atypical (Asn-X-cys) glycosylation motifs. J. Biol. Chem. 1997, 272, 23117–23122. [Google Scholar] [CrossRef] [Green Version]
  101. Kang, S.J.; Cresswell, P. Calnexin, calreticulin, and ERp57 cooperate in disulfide bond formation in human CD1d heavy chain. J. Biol. Chem. 2002, 277, 44838–44844. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  102. Paduraru, C.; Spiridon, L.; Yuan, W.; Bricard, G.; Valencia, X.; Porcelli, S.A.; Illarionov, P.A.; Besra, G.S.; Petrescu, S.M.; Petrescu, A.J.; et al. An N-linked glycan modulates the interaction between the CD1d heavy chain and beta 2-microglobulin. J. Biol. Chem. 2006, 281, 40369–40378. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  103. Dick, T.P.; Bangia, N.; Peaper, D.R.; Cresswell, P. Disulfide bond isomerization and the assembly of MHC class I-peptide complexes. Immunity 2002, 16, 87–98. [Google Scholar] [CrossRef] [Green Version]
  104. Wearsch, P.A.; Peaper, D.R.; Cresswell, P. Essential glycan-dependent interactions optimize MHC class I peptide loading. Proc. Natl. Acad. Sci. USA 2011, 108, 4950–4955. [Google Scholar] [CrossRef] [Green Version]
  105. Mirazimi, A.; Svensson, L. Carbohydrates facilitate correct disulfide bond formation and folding of rotavirus VP7. J. Virol. 1998, 72, 3887–3892. [Google Scholar] [CrossRef] [Green Version]
  106. McGinnes, L.W.; Wilde, A.; Morrison, T.G. Nucleotide sequence of the gene encoding the Newcastle disease virus hemagglutinin-neuraminidase protein and comparisons of paramyxovirus hemagglutinin-neuraminidase protein sequences. Virus Res. 1987, 7, 187–202. [Google Scholar] [CrossRef]
  107. McGinnes, L.W.; Morrison, T.G. The role of the individual cysteine residues in the formation of the mature, antigenic HN protein of Newcastle disease virus. Virology 1994, 200, 470–483. [Google Scholar] [CrossRef]
  108. Mirza, A.M.; Sheehan, J.P.; Hardy, L.W.; Glickman, R.L.; Iorio, R.M. Structure and function of a membrane anchor-less form of the hemagglutinin-neuraminidase glycoprotein of Newcastle disease virus. J. Biol. Chem. 1993, 268, 21425–21431. [Google Scholar] [CrossRef]
  109. Kao, L.; Sassani, P.; Azimov, R.; Pushkin, A.; Abuladze, N.; Peti-Peterdi, J.; Liu, W.; Newman, D.; Kurtz, I. Oligomeric structure and minimal functional unit of the electrogenic sodium bicarbonate cotransporter NBCe1-A. J. Biol. Chem. 2008, 283, 26782–26794. [Google Scholar] [CrossRef] [Green Version]
  110. Hemming, A.; Bolmstedt, A.; Flodby, P.; Lundberg, L.; Gidlund, M.; Wigzell, H.; Olofsson, S.O. Cysteine 402 of HIV gp120 is essential for CD4-binding and resistance of gp120 to intracellular degradation. Arch. Virol. 1989, 109, 269–276. [Google Scholar] [CrossRef]
  111. Tschachler, E.; Buchow, H.; Gallo, R.C.; Reitz, M.S., Jr. Functional contribution of cysteine residues to the human immunodeficiency virus type 1 envelope. J. Virol. 1990, 64, 2250–2259. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  112. Norskov-Lauritsen, L.; Jorgensen, S.; Brauner-Osborne, H. N-glycosylation and disulfide bonding affects GPRC6A receptor expression, function, and dimerization. FEBS Lett. 2015, 589, 588–597. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  113. Pi, M.; Nishimoto, S.K.; Quarles, L.D. GPRC6A: Jack of all metabolism (or master of none). Mol. Metab. 2017, 6, 185–193. [Google Scholar] [CrossRef] [PubMed]
  114. Clemmensen, C.; Smajilovic, S.; Wellendorph, P.; Brauner-Osborne, H. The GPCR, class C, group 6, subtype A (GPRC6A) receptor: From cloning to physiological function. Br. J. Pharmacol. 2014, 171, 1129–1141. [Google Scholar] [CrossRef] [Green Version]
  115. Muto, T.; Tsuchiya, D.; Morikawa, K.; Jingami, H. Structures of the extracellular regions of the group II/III metabotropic glutamate receptors. Proc. Natl. Acad. Sci. USA 2007, 104, 3759–3764. [Google Scholar] [CrossRef] [Green Version]
  116. Rider, P.J.F.; Naderi, M.; Bergeron, S.; Chouljenko, V.N.; Brylinski, M.; Kousoulas, K.G. Cysteines and N-Glycosylation Sites Conserved among All Alphaherpesviruses Regulate Membrane Fusion in Herpes Simplex Virus 1 Infection. J. Virol. 2017, 91, e00873-17. [Google Scholar] [CrossRef] [Green Version]
  117. Neubauer, A.; Osterrieder, N. Equine herpesvirus type 1 (EHV-1) glycoprotein K is required for efficient cell-to-cell spread and virus egress. Virology 2004, 329, 18–32. [Google Scholar] [CrossRef] [Green Version]
  118. Zhang, S.; Go, E.P.; Ding, H.; Anang, S.; Kappes, J.C.; Desaire, H.; Sodroski, J. Analysis of glycosylation and disulfide bonding of wild-type SARS-CoV-2 spike glycoprotein. J. Virol. 2022, 96, e01626-21. [Google Scholar] [CrossRef]
  119. Brun, J.; Vasiljevic, S.; Gangadharan, B.; Hensen, M.; Chandran, A.V.; Hill, M.L.; Kiappes, J.L.; Dwek, R.A.; Alonzi, D.S.; Struwe, W.B.; et al. Analysis of SARS-CoV-2 spike glycosylation reveals shedding of a vaccine candidate. bioRxiv 2020. [Google Scholar] [CrossRef]
  120. Wang, D.; Baudys, J.; Bundy, J.L.; Solano, M.; Keppel, T.; Barr, J.R. Comprehensive Analysis of the Glycan Complement of SARS-CoV-2 Spike Proteins Using Signature Ions-Triggered Electron-Transfer/Higher-Energy Collisional Dissociation (EThcD) Mass Spectrometry. Anal. Chem. 2020, 92, 14730–14739. [Google Scholar] [CrossRef]
  121. Yao, H.; Song, Y.; Chen, Y.; Wu, N.; Xu, J.; Sun, C.; Zhang, J.; Weng, T.; Zhang, Z.; Wu, Z.; et al. Molecular Architecture of the SARS-CoV-2 Virus. Cell 2020, 183, 730–738.e13. [Google Scholar] [CrossRef]
  122. Sanda, M.; Morrison, L.; Goldman, R. N and O glycosylation of the SARS-CoV-2 spike protein. Anal. Chem. 2021, 93, 2003–2009. [Google Scholar] [CrossRef]
  123. Watanabe, Y.; Allen, J.D.; Wrapp, D.; McLellan, J.S.; Crispin, M. Site-specific glycan analysis of the SARS-CoV-2 spike. Science 2020, 369, 330–333. [Google Scholar] [CrossRef]
  124. Bangaru, S.; Ozorowski, G.; Turner, H.L.; Antanasijevic, A.; Huang, D.; Wang, X.; Torres, J.L.; Diedrich, J.K.; Tian, J.H.; Portnoff, A.D.; et al. Structural analysis of full-length SARS-CoV-2 spike protein from an advanced vaccine candidate. Science 2020, 370, 1089–1094. [Google Scholar] [CrossRef]
  125. Zhao, P.; Praissman, J.L.; Grant, O.C.; Cai, Y.; Xiao, T.; Rosenbalm, K.E.; Aoki, K.; Kellman, B.P.; Bridger, R.; Barouch, D.H.; et al. Virus-Receptor Interactions of Glycosylated SARS-CoV-2 Spike and Human ACE2 Receptor. Cell Host Microbe 2020, 28, 586–601 e586. [Google Scholar] [CrossRef]
  126. Hati, S.; Bhattacharyya, S. Impact of Thiol-Disulfide Balance on the Binding of Covid-19 Spike Protein with Angiotensin-Converting Enzyme 2 Receptor. ACS Omega 2020, 5, 16292–16298. [Google Scholar] [CrossRef]
  127. Singh, J.; Dhindsa, R.S.; Misra, V.; Singh, B. SARS-CoV2 infectivity is potentially modulated by host redox status. Comput. Struct. Biotechnol. J. 2020, 18, 3705–3711. [Google Scholar] [CrossRef]
  128. Lan, J.; Ge, J.; Yu, J.; Shan, S.; Zhou, H.; Fan, S.; Zhang, Q.; Shi, X.; Wang, Q.; Zhang, L.; et al. Structure of the SARS-CoV-2 spike receptor-binding domain bound to the ACE2 receptor. Nature 2020, 581, 215–220. [Google Scholar] [CrossRef] [Green Version]
  129. Mehdipour, A.R.; Hummer, G. Dual nature of human ACE2 glycosylation in binding to SARS-CoV-2 spike. Proc. Natl. Acad. Sci. USA 2021, 118, e2100425118. [Google Scholar] [CrossRef]
  130. Roth, Z.; Yehezkel, G.; Khalaila, I. Identification and Quantification of Protein Glycosylation. Int. J. Carbohydr. Chem. 2012, 2012, 640923. [Google Scholar] [CrossRef] [Green Version]
  131. Gimeno, A.; Valverde, P.; Arda, A.; Jimenez-Barbero, J. Glycan structures and their interactions with proteins. A NMR view. Curr. Opin. Struct. Biol. 2020, 62, 22–30. [Google Scholar] [CrossRef]
  132. Imperiali, B.; O’Connor, S.E. Effect of N-linked glycosylation on glycopeptide and glycoprotein structure. Curr. Opin. Chem. Biol. 1999, 3, 643–649. [Google Scholar] [CrossRef]
  133. Kozak, S.; Bloch, Y.; De Munck, S.; Mikula, A.; Bento, I.; Savvides, S.N.; Meijers, R. Homogeneously N-glycosylated proteins derived from the GlycoDelete HEK293 cell line enable diffraction-quality crystallogenesis. Acta Crystallogr. Sect. D Struct. Biol. 2020, 76, 1244–1255. [Google Scholar] [CrossRef]
  134. Freeze, H.H.; Kranz, C. Endoglycosidase and glycoamidase release of N-linked glycans. Curr. Protoc. Mol. Biol. 2010, 89, 17.13A.1–17.13A.25. [Google Scholar] [CrossRef] [Green Version]
  135. Kinsella, M.G.; Wight, T.N. Isolation and characterization of dermatan sulfate proteoglycans synthesized by cultured bovine aortic endothelial cells. J. Biol. Chem. 1988, 263, 19222–19231. [Google Scholar] [CrossRef]
  136. Guile, G.R.; Wong, S.Y.; Dwek, R.A. Analytical and preparative separation of anionic oligosaccharides by weak anion-exchange high-performance liquid chromatography on an inert polymer column. Anal. Biochem. 1994, 222, 231–235. [Google Scholar] [CrossRef]
  137. Townsend, R.R.; Hardy, M.R. Analysis of glycoprotein oligosaccharides using high-pH anion exchange chromatography. Glycobiology 1991, 1, 139–147. [Google Scholar] [CrossRef]
  138. Guile, G.R.; Rudd, P.M.; Wing, D.R.; Prime, S.B.; Dwek, R.A. A rapid high-resolution high-performance liquid chromatographic method for separating glycan mixtures and analyzing oligosaccharide profiles. Anal. Biochem. 1996, 240, 210–226. [Google Scholar] [CrossRef]
  139. Guile, G.R.; Harvey, D.J.; O’Donnell, N.; Powell, A.K.; Hunter, A.P.; Zamze, S.; Fernandes, D.L.; Dwek, R.A.; Wing, D.R. Identification of highly fucosylated N-linked oligosaccharides from the human parotid gland. Eur. J. Biochem. 1998, 258, 623–656. [Google Scholar] [CrossRef] [Green Version]
  140. Han, L.; Costello, C.E. Mass spectrometry of glycans. Biochem. Biokhimiia 2013, 78, 710–720. [Google Scholar] [CrossRef] [Green Version]
  141. Harvey, D.J. Matrix-assisted laser desorption/ionisation mass spectrometry of oligosaccharides and glycoconjugates. J. Chromatogr. A 1996, 720, 429–446. [Google Scholar] [CrossRef]
  142. Illiano, A.; Pinto, G.; Melchiorre, C.; Carpentieri, A.; Faraco, V.; Amoresano, A. Protein Glycosylation Investigated by Mass Spectrometry: An Overview. Cells 2020, 9, 1986. [Google Scholar] [CrossRef] [PubMed]
  143. Mechref, Y.; Novotny, M.V. Structural investigations of glycoconjugates at high sensitivity. Chem. Rev. 2002, 102, 321–369. [Google Scholar] [CrossRef]
  144. Sagi, D.; Kienz, P.; Denecke, J.; Marquardt, T.; Peter-Katalinic, J. Glycoproteomics of N-glycosylation by in-gel deglycosylation and matrix-assisted laser desorption/ionisation-time of flight mass spectrometry mapping: Application to congenital disorders of glycosylation. Proteomics 2005, 5, 2689–2701. [Google Scholar] [CrossRef] [PubMed]
  145. Zhang, H.; Li, X.J.; Martin, D.B.; Aebersold, R. Identification and quantification of N-linked glycoproteins using hydrazide chemistry, stable isotope labeling and mass spectrometry. Nat. Biotechnol. 2003, 21, 660–666. [Google Scholar] [CrossRef] [PubMed]
  146. Zhu, F.; Trinidad, J.C.; Clemmer, D.E. Glycopeptide Site Heterogeneity and Structural Diversity Determined by Combined Lectin Affinity Chromatography/IMS/CID/MS Techniques. J. Am. Soc. Mass Spectrom. 2015, 26, 1092–1102. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  147. Bloom, J.W.; Madanat, M.S.; Ray, M.K. Cell line and site specific comparative analysis of the N-linked oligosaccharides on human ICAM-1des454-532 by electrospray ionization mass spectrometry. Biochemistry 1996, 35, 1856–1864. [Google Scholar] [CrossRef]
  148. Bunkenborg, J.; Pilch, B.J.; Podtelejnikov, A.V.; Wisniewski, J.R. Screening for N-glycosylated proteins by liquid chromatography mass spectrometry. Proteomics 2004, 4, 454–465. [Google Scholar] [CrossRef]
  149. Ford, K.L.; Zeng, W.; Heazlewood, J.L.; Bacic, A. Characterization of protein N-glycosylation by tandem mass spectrometry using complementary fragmentation techniques. Front Plant Sci 2015, 6, 674. [Google Scholar] [CrossRef] [Green Version]
  150. Esko, J.D.; Bertozzi, C.; Schnaar, R.L. Chemical Tools for Inhibiting Glycosylation. In Essentials of Glycobiology, 3rd ed.; Varki, A., Cummings, R.D., Esko, J.D., Stanley, P., Hart, G.W., Aebi, M., Darvill, A.G., Kinoshita, T., Packer, N.H., Prestegard, J.H., et al., Eds.; Cold Spring Harbor: Huntington, NY, USA, 2015; pp. 701–712. [Google Scholar] [CrossRef]
  151. Wainwright, L.J.; Field, M.C. Quality control of glycosylphosphatidylinositol anchor attachment in mammalian cells: A biochemical study. Biochem. J. 1997, 321 Pt 3, 655–664. [Google Scholar] [CrossRef] [Green Version]
  152. Barolo, L.; Abbriano, R.M.; Commault, A.S.; George, J.; Kahlke, T.; Fabris, M.; Padula, M.P.; Lopez, A.; Ralph, P.J.; Pernice, M. Perspectives for Glyco-Engineering of Recombinant Biopharmaceuticals from Microalgae. Cells 2020, 9, 633. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  153. Weinfurtner, D. Analysis of Disulfide Bond Formation in Therapeutic Proteins. In Oxidative Folding of Proteins: Basic Principles, Cellular Regulation and Engineerining; Royal Society of Chemistry: London, UK, 2018; pp. 81–98. [Google Scholar] [CrossRef]
  154. Haniu, M.; Acklin, C.; Kenney, W.C.; Rohde, M.F. Direct assignment of disulfide bonds by Edman degradation of selected peptide fragments. Int. J. Pept. Protein Res. 1994, 43, 81–86. [Google Scholar] [CrossRef] [PubMed]
  155. Klaus, W.; Broger, C.; Gerber, P.; Senn, H. Determination of the disulphide bonding pattern in proteins by local and global analysis of nuclear magnetic resonance data. Application to flavoridin. J. Mol. Biol. 1993, 232, 897–906. [Google Scholar] [CrossRef] [PubMed]
  156. Sharma, D.; Rajarathnam, K. 13C NMR chemical shifts can predict disulfide bond formation. J. Biomol. NMR 2000, 18, 165–171. [Google Scholar] [CrossRef] [PubMed]
  157. Jones, T.A.; Kjeldgaard, M. Electron-density map interpretation. Methods Enzymol. 1997, 277, 173–208. [Google Scholar] [CrossRef]
  158. Damodaran, S. Estimation of disulfide bonds using 2-nitro-5-thiosulfobenzoic acid: Limitations. Anal. Biochem. 1985, 145, 200–204. [Google Scholar] [CrossRef]
  159. Thannhauser, T.W.; Konishi, Y.; Scheraga, H.A. Analysis for disulfide bonds in peptides and proteins. Methods Enzymol. 1987, 143, 115–119. [Google Scholar] [CrossRef]
  160. Aitken, A.; Learmonth, M. Quantitation of cysteine residues and disulfide bonds by electrophoresis. In The Protein Protocols Handbook; Walker, J.M., Ed.; Humana Press: Totowa, NJ, USA, 2009; pp. 1057–1062. [Google Scholar] [CrossRef]
  161. Hirose, M.; Takahashi, N.; Oe, H.; Doi, E. Analyses of intramolecular disulfide bonds in proteins by polyacrylamide gel electrophoresis following two-step alkylation. Anal. Biochem. 1988, 168, 193–201. [Google Scholar] [CrossRef]
  162. Saraswat, R.; McDonagh, B. Diagonal Electrophoresis for the Detection of Proteins Involved in Disulfide Bonds. Methods Mol. Biol. 2019, 1855, 279–286. [Google Scholar] [CrossRef]
  163. Chrisman, P.A.; Pitteri, S.J.; Hogan, J.M.; McLuckey, S.A. SO2-* electron transfer ion/ion reactions with disulfide linked polypeptide ions. J. Am. Soc. Mass Spectrom. 2005, 16, 1020–1030. [Google Scholar] [CrossRef] [Green Version]
  164. Cramer, C.N.; Haselmann, K.F.; Olsen, J.V.; Nielsen, P.K. Disulfide Linkage Characterization of Disulfide Bond-Containing Proteins and Peptides by Reducing Electrochemistry and Mass Spectrometry. Anal. Chem. 2016, 88, 1585–1592. [Google Scholar] [CrossRef] [PubMed]
  165. Gorman, J.J.; Wallis, T.P.; Pitt, J.J. Protein disulfide bond determination by mass spectrometry. Mass Spectrom. Rev. 2002, 21, 183–216. [Google Scholar] [CrossRef] [PubMed]
  166. Lakbub, J.C.; Shipman, J.T.; Desaire, H. Recent mass spectrometry-based techniques and considerations for disulfide bond characterization in proteins. Anal. Bioanal. Chem. 2018, 410, 2467–2484. [Google Scholar] [CrossRef]
  167. Tsai, P.; Chen, S.; Huang, S.Y. Mass spectrometry-based strategies for protein disulfide bond identification. Rev. Anal. Chem. 2013, 32, 257–268. [Google Scholar] [CrossRef]
  168. Wiesner, J.; Resemann, A.; Evans, C.; Suckau, D.; Jabs, W. Advanced mass spectrometry workflows for analyzing disulfide bonds in biologics. Expert Rev. Proteom. 2015, 12, 115–123. [Google Scholar] [CrossRef]
  169. Zhou, Y.; Dong, J.; Vachet, R.W. Electron transfer dissociation of modified peptides and proteins. Curr. Pharm. Biotechnol. 2011, 12, 1558–1567. [Google Scholar] [CrossRef]
  170. Sarbu, M.; Ghiulai, R.M.; Zamfir, A.D. Recent developments and applications of electron transfer dissociation mass spectrometry in proteomics. Amino Acids 2014, 46, 1625–1634. [Google Scholar] [CrossRef]
  171. Wu, S.L.; Jiang, H.; Hancock, W.S.; Karger, B.L. Identification of the unpaired cysteine status and complete mapping of the 17 disulfides of recombinant tissue plasminogen activator using LC-MS with electron transfer dissociation/collision induced dissociation. Anal. Chem. 2010, 82, 5296–5303. [Google Scholar] [CrossRef] [Green Version]
  172. Lakbub, J.C.; Clark, D.F.; Shah, I.S.; Zhu, Z.; Go, E.P.; Tolbert, T.J.; Desaire, H. Disulfide Bond Characterization of Endogenous IgG3 Monoclonal Antibodies Using LC-MS: An Investigation of IgG3 Disulfide-mediated Isoforms. Anal. Methods 2016, 8, 6046–6055. [Google Scholar] [CrossRef] [Green Version]
  173. Clark, D.F.; Go, E.P.; Toumi, M.L.; Desaire, H. Collision induced dissociation products of disulfide-bonded peptides: Ions result from the cleavage of more than one bond. J. Am. Soc. Mass Spectrom. 2011, 22, 492–498. [Google Scholar] [CrossRef] [Green Version]
  174. Olsen, J.V.; Macek, B.; Lange, O.; Makarov, A.; Horning, S.; Mann, M. Higher-energy C-trap dissociation for peptide modification analysis. Nat. Methods 2007, 4, 709–712. [Google Scholar] [CrossRef] [PubMed]
  175. Frese, C.K.; Altelaar, A.F.; van den Toorn, H.; Nolting, D.; Griep-Raming, J.; Heck, A.J.; Mohammed, S. Toward full peptide sequence coverage by dual fragmentation combining electron-transfer and higher-energy collision dissociation tandem mass spectrometry. Anal. Chem. 2012, 84, 9668–9673. [Google Scholar] [CrossRef] [PubMed]
  176. Liu, F.; van Breukelen, B.; Heck, A.J. Facilitating protein disulfide mapping by a combination of pepsin digestion, electron transfer higher energy dissociation (EThcD), and a dedicated search algorithm SlinkS. Mol. Cell Proteom. 2014, 13, 2776–2786. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  177. Agarwal, A.; Diedrich, J.K.; Julian, R.R. Direct elucidation of disulfide bond partners using ultraviolet photodissociation mass spectrometry. Anal. Chem. 2011, 83, 6455–6458. [Google Scholar] [CrossRef]
  178. Suga, A.; Nagae, M.; Yamaguchi, Y. Analysis of protein landscapes around N-glycosylation sites from the PDB repository for understanding the structural basis of N-glycoprotein processing and maturation. Glycobiology 2018, 28, 774–785. [Google Scholar] [CrossRef]
  179. Wu, D.; Struwe, W.B.; Harvey, D.J.; Ferguson, M.A.J.; Robinson, C.V. N-glycan microheterogeneity regulates interactions of plasma proteins. Proc. Natl. Acad. Sci. USA 2018, 115, 8763–8768. [Google Scholar] [CrossRef] [Green Version]
  180. Bendiak, B.; Ward, L.D.; Simpson, R.J. Proteins of the Golgi apparatus. Purification to homogeneity, N-terminal sequence, and unusually large Stokes radius of the membrane-bound form of UDP-galactose:N-acetylglucosamine beta 1-4galactosyltransferase from rat liver. Eur. J. Biochem. 1993, 216, 405–417. [Google Scholar] [CrossRef]
  181. Krambeck, F.J.; Betenbaugh, M.J. A mathematical model of N-linked glycosylation. Biotechnol. Bioeng. 2005, 92, 711–728. [Google Scholar] [CrossRef]
  182. Krambeck, F.J.; Bennun, S.V.; Andersen, M.R.; Betenbaugh, M.J. Model-based analysis of N-glycosylation in Chinese hamster ovary cells. PLoS ONE 2017, 12, e0175376. [Google Scholar] [CrossRef] [Green Version]
  183. Nakajima, K.; Ito, E.; Ohtsubo, K.; Shirato, K.; Takamiya, R.; Kitazume, S.; Angata, T.; Taniguchi, N. Mass isotopomer analysis of metabolically labeled nucleotide sugars and N- and O-glycans for tracing nucleotide sugar metabolisms. Mol. Cell Proteom. 2013, 12, 2468–2480. [Google Scholar] [CrossRef] [Green Version]
  184. North, S.J.; Huang, H.H.; Sundaram, S.; Jang-Lee, J.; Etienne, A.T.; Trollope, A.; Chalabi, S.; Dell, A.; Stanley, P.; Haslam, S.M. Glycomics profiling of Chinese hamster ovary cell glycosylation mutants reveals N-glycans of a novel size and complexity. J. Biol. Chem. 2010, 285, 5759–5775. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  185. Yang, Y.; Franc, V.; Heck, A.J.R. Glycoproteomics: A Balance between High-Throughput and In-Depth Analysis. Trends Biotechnol. 2017, 35, 598–609. [Google Scholar] [CrossRef] [PubMed]
  186. Thaysen-Andersen, M.; Packer, N.H. Advances in LC-MS/MS-based glycoproteomics: Getting closer to system-wide site-specific mapping of the N- and O-glycoproteome. Biochim. Biophys. Acta 2014, 1844, 1437–1452. [Google Scholar] [CrossRef]
  187. Sun, B.; Hood, L. Protein-centric proteomics analysis of membrane and plasma membrane proteins. J. Proteome Res. 2014, 13, 2705–2714. [Google Scholar] [CrossRef] [PubMed]
  188. Lennicke, C.; Rahn, J.; Heimer, N.; Lichtenfels, R.; Wessjohann, L.A.; Seliger, B. Redox proteomics: Methods for the identification and enrichment of redox-modified proteins and their applications. Proteomics 2016, 16, 197–213. [Google Scholar] [CrossRef]
  189. Solda, T.; Garbi, N.; Hammerling, G.J.; Molinari, M. Consequences of ERp57 deletion on oxidative folding of obligate and facultative clients of the calnexin cycle. J. Biol. Chem. 2006, 281, 6219–6226. [Google Scholar] [CrossRef] [Green Version]
  190. Watt, G.M.; Lund, J.; Levens, M.; Kolli, V.S.; Jefferis, R.; Boons, G.J. Site-specific glycosylation of an aglycosylated human IgG1-Fc antibody protein generates neoglycoproteins with enhanced function. Chem. Biol. 2003, 10, 807–814. [Google Scholar] [CrossRef] [Green Version]
  191. Mathys, L.; Balzarini, J. Several N-Glycans on the HIV Envelope Glycoprotein gp120 Preferentially Locate Near Disulphide Bridges and Are Required for Efficient Infectivity and Virus Transmission. PLoS ONE 2015, 10, e0130621. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. Distribution of species hosting proteins studied for N-glycosylation and disulfide bonds.
Figure 1. Distribution of species hosting proteins studied for N-glycosylation and disulfide bonds.
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Figure 2. Distribution of different relationships between the N-glycosylation and disulfide bonds in the literature examined.
Figure 2. Distribution of different relationships between the N-glycosylation and disulfide bonds in the literature examined.
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Figure 3. Schematic of the relative position between N-glycosylation and disulfide bonds and their relationship in the selected proteins discussed here. S4A4, UniProt ID of human SLC4 Na+-coupled transporter, NBCe1; CGB3, UniProt ID of human chorionic gonadotropin beta-subunit; 9HIV1, UniProt ID of human immunodeficiency virus envelope glycoprotein; CNMD, UniProt ID of human chondromodulin-1. Colors indicate different disulfide bond pairs. The N-glycan sign does not represent the actual sugar structure.
Figure 3. Schematic of the relative position between N-glycosylation and disulfide bonds and their relationship in the selected proteins discussed here. S4A4, UniProt ID of human SLC4 Na+-coupled transporter, NBCe1; CGB3, UniProt ID of human chorionic gonadotropin beta-subunit; 9HIV1, UniProt ID of human immunodeficiency virus envelope glycoprotein; CNMD, UniProt ID of human chondromodulin-1. Colors indicate different disulfide bond pairs. The N-glycan sign does not represent the actual sugar structure.
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Figure 4. Molecular pathophysiology of extracellular loop 3 of NBCe1-A caused by mutual relationships between N-glycosylation and disulfide bonds.
Figure 4. Molecular pathophysiology of extracellular loop 3 of NBCe1-A caused by mutual relationships between N-glycosylation and disulfide bonds.
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Bakshi, T.; Pham, D.; Kaur, R.; Sun, B. Hidden Relationships between N-Glycosylation and Disulfide Bonds in Individual Proteins. Int. J. Mol. Sci. 2022, 23, 3742. https://doi.org/10.3390/ijms23073742

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Bakshi T, Pham D, Kaur R, Sun B. Hidden Relationships between N-Glycosylation and Disulfide Bonds in Individual Proteins. International Journal of Molecular Sciences. 2022; 23(7):3742. https://doi.org/10.3390/ijms23073742

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Bakshi, Tania, David Pham, Raminderjeet Kaur, and Bingyun Sun. 2022. "Hidden Relationships between N-Glycosylation and Disulfide Bonds in Individual Proteins" International Journal of Molecular Sciences 23, no. 7: 3742. https://doi.org/10.3390/ijms23073742

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