# Characterisation of N-glycans in the epithelial-like tissue of the rat cochlea

## Abstract

Membrane proteins (such as ion channels, transporters, and receptors) and secreted proteins are essential for cellular activities. N-linked glycosylation is involved in stability and function of these proteins and occurs at Asn residues. In several organs, profiles of N-glycans have been determined by comprehensive analyses. Nevertheless, the cochlea of the mammalian inner ear, a tiny organ mediating hearing, has yet to be examined. Here, we focused on the stria vascularis, an epithelial-like tissue in the cochlea, and characterised N-glycans by liquid chromatography with mass spectrometry. This hypervascular tissue not only expresses several ion transporters and channels to control the electrochemical balance in the cochlea but also harbours different transporters and receptors that maintain structure and activity of the organ. Seventy-nine N-linked glycans were identified in the rat stria vascularis. Among these, in 55 glycans, the complete structures were determined; in the other 24 species, partial glycosidic linkage patterns and full profiles of the monosaccharide composition were identified. In the process of characterisation, several sialylated glycans were subjected sequentially to two different alkylamidation reactions; this derivatisation helped to distinguish α2,3-linkage and α2,6-linkage sialyl isomers with mass spectrometry. These data should accelerate elucidation of the molecular architecture of the cochlea.

## Introduction

Cellular and tissue functions are precisely and dynamically controlled by a variety of membrane-integral proteins such as receptors, ion channels, and transporters. More than 50% of these proteins are glycosylated1. This post-transcriptional modification also occurs in the majority of secreted proteins that mediate the cross-talk among cells2. Glycosylation affects Asn residues (N-glycans) or Ser/Thr residues (O-glycans). Recent studies highlighted roles of different N-glycans not only in the processes related to protein stability and trafficking but also in the modulation of actions of membrane proteins3,4. Therefore, characterisation of glycan types expressed in each tissue or organ is crucial for elucidation of molecular architectures underlying vital phenomena in various organisms.

Although structures of N-glycans in serum and several organs including the brain, lungs, and kidneys have been comprehensively analysed5,6,7,8, those in the cochlea of the mammalian inner ear, a small organ of a few millimetres in size, have not yet been sufficiently profiled. In the cochlea, the stria vascularis, an epithelial-like tissue composed of marginal, intermediate, and basal cells, contains numerous capillaries; therefore, it carries a variety of substances including hormones, metabolites, glucose, and even externally applied drugs, from blood to itself and other tissues9,10,11. These actions are likely to be mediated by a considerable number of organic transporters; besides, receptors for growth factors and hormones are expressed in strial cells12,13,14,15. Strial K+ channels and K+ uptake transporters maintain a high [K+] of 150 mM and a highly positive potential of +80 mV in an extracellular fluid, endolymph; these electrochemical milieus contribute to the maintenance of hearing (Fig. 1a)16,17,18. Other endolymphatic properties such as volume, osmolarity, and pH may be balanced by a variety of ion channels and transporters in the stria12,19,20. In addition, marginal cells seem to secrete a few protein types that can be involved in the development of the cochlea21,22. Overall, it is plausible that the strial membrane protein networks described above are collectively crucial for cochlear function. In the present study, we focused on the stria vascularis and profiled the structures of its N-glycans, which potentially regulate activities of the membrane and secreted proteins. Our method combining three high performance liquid chromatography (HPLC) types and different modes of multi-stage mass spectrometry (MSn) identified 79 different N-glycan species and characterised their structures.

## Results

### Verification of purification of the stria vascularis dissociated from the cochlea

The stria vascularis is enriched with capillaries and is tightly attached to a neighbouring tissue, the spiral ligament, in the lateral cochlear wall (Fig. 1a). We first perfused rats systemically with saline to remove blood from the stria vascularis and then carefully isolated this tissue from the lateral wall (Fig. 1b–d; see also ‘Methods’). Nevertheless, we were concerned about contamination with the ligament in the samples. We therefore decided to evaluate the purity of the samples. Total-RNA samples extracted from the isolated stria vascularis and spiral ligament from 8–10 cochleae (4–5 rats) were independently analysed by quantitative PCR (qPCR) with primers for the four genes that encode the proteins specific to each tissue (Fig. 2). This series of assays was repeated three times with different batches of cochleae. The stria vascularis is separated from endolymph and the spiral ligament by marginal and basal cells, respectively (Fig. 2a). Our qPCR assays (Fig. 2b) showed that mRNA of Clchannel β-subunit barttin (Bsnd), which is exclusively expressed in marginal cells23, was abundant in the samples of the stria but was only moderately detectable in those of the ligament. Similar results were obtained with the primers specific for claudin 11 (Cldn11), a component of tight junction strands in basal cells24,25. We next performed assays with primers for a K+,Cl-cotransporter KCC3 (slc12a6) and transcription factor Brn-4 (pou3f4), both of which are present in the ligament but absent in the stria vascularis26,27. The amounts of mRNAs of the two genes were negligible in the samples of the stria but well detectable in those of the ligament. These tendencies were observed in all the three series of experiments (Fig. 2b). The observations described above confirmed not only the purity of the strial samples but also the reliability of our isolation technique.

### Detection and characterisation of glycans in the stria vascularis

We next characterised the profile of glycans in the stria vascularis. The strial tissues dissociated from 102 cochleae (51 rats) were combined into one batch. The sample was lyophilised and chemically treated in accordance with the process described in the ‘Methods’ section. The following workflow was carried out by multiple methods as shown in Fig. 3a, and the numbers of strial glycans extracted or characterised by each method are illustrated in Fig. 3b. In this series of experiments, crude pyridylaminated (PA)-glycans from the samples were initially subjected to diethylaminoethyl (DEAE) anion exchange HPLC (Fig. 3a). This method fractionates N-glycans in accordance with the number of the attached sialic acid residues. As shown in Fig. 4a, in the stria vascularis, non-sialic glycans (N) were the most abundant. Smaller amounts of the mono- and di-sialic glycans (classes A1 and A2, respectively) were also detected in the samples. Careful observations unveiled a weak but significant signal of tri- and tetra-sialylated classes (A3 and A4, respectively). A peak between N and A1 signals stemmed primarily from non-glycan materials that persisted during sample processing7,28. Then, the five fractions (N, A1–A4) were separately collected and assayed by reversed-phase HPLC, which evaluates hydrophobicity of samples (Figs 3 and 4b). Numerous peaks were obtained in this assay; in this context, the eluates within the initial ~10 min were likely to contain chemical reagents including pyridylamine and its derivatives28, and therefore they were omitted for further analyses. We measured the areas of all the individual peaks and found that the fifth fraction in the non-sialic class (N-5) was the most abundant species. On the basis of this observation, a fraction whose area exceeded 2% of that of the N-5 fraction was assumed to be significant. According to this criterion, we re-evaluated all the data obtained by reversed-phase HPLC (Fig. 3a). Consequently, 27 fractions from class N, 24 fractions from class A1, 27 fractions from class A2, 21 fractions from class A3, and eight fractions from the A4 class were collected as presented in Fig. 4b (a total of 107 fractions; see also Fig. 3b). Then, each of these 107 fractions was subjected one by one to size fractionation HPLC, which analyses molecular size of the samples (Fig. 3a; for raw chromatograms, see Supplementary Fig. S1). Each fraction separated with this procedure should be composed of a sole glycan type. Areas of the individual peaks were again determined; the most abundant was a species that was derived from the N-5 fraction extracted by reversed-phase HPLC (N-5 as is). In the products of the size fractionation HPLC, the fraction whose area exceeded 2% of that of the N-5 fraction was assumed to be significant. Of note, in some cases, from the fraction separated by the reversed-phase HPLC, multiple peaks were obtained in the analysis of the size fractionation HPLC; these products were sub-numbered with reference to their elution time (Table 1 and Supplementary Fig. S1 and Tables S1 and S2). As a consequence, at least 88 glycan species were isolated from the strial samples (Fig. 3b and Supplementary Fig. S1).

All the 88 glycans were subjected to liquid chromatography with positive ion mode electrospray ionisation mass spectrometry (LC-ESI-MS) and MS2 analyses (Fig. 3). In the former, because the original samples extracted through reversed-phase HPLC were analysed, multiple peaks that showed different glycan types were detected in the spectra in many cases (Supplementary Fig. S2). Elution profiles of the products in the size fractionation HPLC enabled us to roughly predict the molecular mass of each eluted glycan29. On the basis of this information, among the fractions obtained in the MS analysis, the ones that represented the aforementioned 88 glycans were selected and then examined with MS2 (Supplementary Fig. S2). This series of experiments revealed that in 75 glycans, the reducing ends consist of Man3GlcNAc2, the core structure of N-glycans (Table 1 and Supplementary Tables S1 and S2)30. We additionally identified Man2GlcNAc2 and its mono-fucosylated derivative, both of which are also categorised into the N-linked type (Table 1 and Supplementary Tables S1 and S2)30,31. These 77 N-glycans were subjected to further analyses (Fig. 3b). On the other hand, 11 glycans, which did not contain Man3GlcNAc2, Man2GlcNAc2, or its mono-fucosylated derivative, were characterised as follows (Supplementary Fig. S2 and Table S3). Four glycans (A2-1, A2-3, A3-3, and A4-1) were found to bear reducing ends composed of N-acetylgalactosamine and therefore they manifested themselves as the O-linked type. Five species (A2-2-1, A2-2-2, A2-4, A2-5, and A4-2) were likely to be degradation products of some original glycans. As for each remainder (N-11-2 and N-14-1), the molecular mass predicted from the signals of the size fractionation HPLC could not be explained by the MS data.

In general, when a glycan is analysed with LC-ESI-MS and MS2, the spectra provide monosaccharide composition and partial glycosidic linkage patterns. This information, on some occasions, allows us to predict multiple structure types of the glycan. Next, to determine the detailed profiles of the 77 N-linked glycans obtained from the stria vascularis, we attempted to use their R and S values29,32 (Fig. 3a). These indexes stem from measured elution time of each glycan in reversed-phase HPLC and that in size fractionation HPLC, respectively29,32 (see ‘Methods’). In addition, 194 standard glycans, which are available from commercial or other resources, have been examined by the two HPLC types, and their R and S values (Rstd and Sstd) can be obtained from the literature7,28 (Supplementary Table S4). With these values, we proceeded to the following four steps for each of the 77 N-glycans from the stria vascularis. Firstly, among the 194 standard glycans, species that have structure(s) identical to a predicted one or multiple structure(s) of a strial glycan were identified. Secondly, the R and S values obtained from the HPLCs’ data of the strial glycan (Rstria and Sstria; see above) were compared to set(s) of the Rstd and Sstd values of the standard glycan(s) assigned at the first step. Thirdly, error factors (error Rstd and error Sstd) between the values of the strial glycan and those of each of the corresponding standard glycans were calculated by means of the formulas:

$${\rm{error}}\,{{\rm{R}}}_{{\rm{std}}}=|\frac{{{\rm{R}}}_{{\rm{stria}}}-{{\rm{R}}}_{{\rm{std}}}}{{{\rm{R}}}_{{\rm{std}}}}|\times 100$$
(1)

and

$${\rm{error}}\,{{\rm{S}}}_{{\rm{std}}}=|\frac{{{\rm{S}}}_{{\rm{stria}}}-{{\rm{S}}}_{{\rm{std}}}}{{{\rm{S}}}_{{\rm{std}}}}|\times 100$$
(2)

Finally, we assigned the standard glycan, which provided both error factors of <5, to the strial glycan. In accordance with these criteria, the structures of 42 strial glycans were determined, as presented in Table 1 and Supplementary Tables S1 and S2 (see also Fig. 3b and Supplementary Table S5). Nevertheless, among these glycans, the assignment of A3-18 [NeuAc3Gal3GlcNAc3Man3FucGlcNAc2 (333N-TRF6)] may not be correct because the information on standard glycans that have more than two sialyl residues is limited.

Next, the rest of the strial N-linked glycans (35 species; see Fig. 3b) were analysed via the following four steps (Fig. 3a). Firstly, even for each of these glycans, the composition and partial linkage patterns were determined by the LC-ESI-MS and MS2 analyses (Supplementary Fig. S2); on the basis of these data, we extracted one or multiple constituent(s) that could also be identified in the library of 194 standard glycans (see Supplementary Table S4). Secondly, Rstd and Sstd values of these assigned constituent(s) were combined with ‘partial elution times’ of the remaining residues. These indexes are the values that are derived and obtained from the types and linkage patterns of the residues in accordance with the ‘empirical additivity rule’7. Collectively, in these two processes, we could not only predict structure(s) of a strial glycan but also calculate the R and S values (i.e. Rcalc and Scalc, respectively). Furthermore, in some cases, multiple linkage patterns were predictable for one strial glycan; therefore, different sets of Rcalc and Scalc values were available. Thirdly, error factors (error Rcalc and error Scalc) between the R and S values of the strial glycan (i.e. aforementioned Rstria and Sstria values) and each set of the Rcalc and Scalc values were obtained via the following equations:

$${\rm{error}}\,{{\rm{R}}}_{{\rm{calc}}}=|\frac{{{\rm{R}}}_{{\rm{stria}}}-{{\rm{R}}}_{{\rm{calc}}}}{{{\rm{R}}}_{{\rm{calc}}}}|\times 100$$
(3)

and

$${\rm{error}}\,{{\rm{S}}}_{{\rm{calc}}}=|\frac{{{\rm{S}}}_{{\rm{stria}}}-{{\rm{S}}}_{{\rm{calc}}}}{{{\rm{S}}}_{{\rm{calc}}}}|\times 100$$
(4)

Finally, we concluded that a candidate that showed two error factors of <5 corresponds to the strial glycan. This series of assays determined the structures of 14 strial glycans (Fig. 3b, Table 1, and Supplementary Tables S1, S2 and S5).

In summary, in the stria vascularis, we identified the complete structures of 55 N-linked glycans and assigned partial structures (along with full profiles of the monosaccharide composition) to the other 24 species (Fig. 3b, Table 1, and Supplementary Tables S1 and S2). As for A3-13 species that belongs to the latter category, the molecular mass determined by positive ion mode MALDI-QIT-TOF MS after SALSA differed by 1095.49 Da from the molecular mass indicated by the combination of LC-ESI-MS and MS2 (Supplementary Figs S2S4 and Table S6); this marked inconsistency cannot be explained by any effects of alkylamidation of the three sialic acid residues. Accordingly, the derivatised sample was next profiled by negative ion mode MALDI-TOF-MSn, as described below (also see Fig. 3).

### Examples of structural analysis of strial N-glycans

In some cases, analysis of glycans with R and S values reveals the linkage patterns that cannot be addressed with mass spectrometry alone. Representative cases are A1-3-2 and A1-4-2 species, which were characterised with LC-ESI-MS and MS2 analyses and the Rstd and Sstd values (Fig. 5 and see Fig. 3). A difference in structure between these two strial N-glycans was limited to the linkage pattern of a single sialic acid residue (Table 1 and Supplementary Tables S1 and S2). In the MS spectrum, the A1-3-2 species was detected as a peak at m/z 985.59 [M + 2 H]2+ (Fig. 5a). This glycan was separated by MS2 into six remarkable fragments; HexHexNAc (m/z 366.17 [M + H]+), NeuAcHexHexNAc (m/z 657.37 [M + H]+), NeuAcHex2HexNAc (m/z 819.41 [M + H]+), NeuAcHex5HexNAc3-PA (m/z 904.44 [M + 2H]2+), Hex4HexNAc-PA (m/z 1151.70 [M + H]+), and Hex5HexNAc2-PA (m/z 1313.70 [M + H]+; Fig. 5a and Supplementary Table S7). These observations implied that species A1-3-2 is NeuAcGalGlcNAcMan5GlcNAc2 (mN-LnM5). At this stage, it remained uncertain whether the glycan is 3N-LnM5 that has an α2,3-linked sialic acid residue or 6N-LnM5 that contains an α2,6-linked sialic acid residue. Such prediction was also the case for A1-4-2 species (Fig. 5b). Rstd and Sstd values of 3N-LnM5 are 60.7 and 6.9, respectively, whereas those of 6N-LnM5 are 56.6 and 7.4, respectively (Supplementary Table S4). Each set of these values was compared to Rstria and Sstria values of the two strial glycans (Fig. 5c). Calculation of error Rstd and Sstd values using equations (1) and (2) and the aforementioned criterion revealed that A1-3-2 and A1-4-2 species are 6N-LnM5 and 3N-LnM5, respectively, as shown in Fig. 5c,d (see also Table 1 and Supplementary Tables S1 and S2).

The next example is a strial glycan whose structure was characterised with the Rcalc and Scalc values (Fig. 6). As illustrated in Fig. 6a, the A1-8-1 species was detected as a marked signal at m/z 896.39 [M + 2 H]2+ in the LC-ESI-MS spectra. Analysis of this fraction in MS2 mode detected five significant peaks, each of which corresponded to HexHexNAc (m/z 366.26 [M + H]+), NeuAcHexHexNAc (m/z 657.31 [M + H]+), Hex2HexNAc2dHex-PA (m/z 973.60 [M + H]+), Hex3HexNAc2dHex-PA (m/z 1135.69 [M + H]+), or Hex4HexNAc3dHex-PA (m/z 1500.83 [M + H]+; Fig. 6a and Supplementary Table S7). Accordingly, fraction A1-8-1 was likely to be made up of NeuAcGalGlcNAcMan3FucGlcNAc2, i.e. mN-MOF6. Regarding the structure of this glycan, four candidates can be proposed because isomers of NeuAcGalGlcNAcMan3GlcNAc2 (MOF6) exist (MO1F6 and MO2F6; Supplementary Table S4) and a galactose residue in each isomer can bind to a sialic acid with α2,3-linkage (3N-MO1F6 or 3N-MO2F6) or with α2,6-linkage (6N-MO1F6 or 6N-MO2F6). For 3N-MO1F6 and 3N-MO2F6, Rstd and Sstd values were available (Supplementary Table S4). Comparison of each pair of these values with Rstria and Sstria values of A1-8-1 indicated that none of the sets of error Rstd and Sstd values satisfied the criterion ‘<5’ as depicted in Fig. 6b [see equations (1) and (2)]. To assign the strial glycan to 6N-MO1F6 or 6N-MO2F6, we obtained their Rcalc and Scalc values via equations (3) and (4) because of a lack of their Rstd and Sstd values (for details, see Fig. 6c). On the basis of calculated error Rcalc and Scalc values and the aforementioned criterion, the A1-8-1 species is potentially 6N-MO1F6 but not 6N-MO2F6 (Fig. 6c,d).

In the experiment shown in Fig. 7, SALSA derivatisation was necessary to clarify the sialyl linkage (see Fig. 3). Species A2-24, which was initially found to possess two sialic acid residues in the HPLC assays (Fig. 4), appeared as a signal at m/z 1326.40 [M + 2 H]2+ in the LC-ESI-MS spectra (Fig. 7a). This parent ion was next separated by MS2 analysis into six major moieties, which were detected as the signals at m/z 657.38 [M + H]+ (NeuAcHexHexNAc), m/z 819.14 [M + H]+ (NeuAcHex2HexNAc), m/z 1176.77 [M + H]+ (Hex2HexNAc3dHex-PA), m/z 1541.23 [M + H]+ (Hex3HexNAc5dHex-PA), m/z 1703.80 [M + H]+ (Hex4HexNAc4dHex-PA), and m/z 1994.90 [M + H]+ (NeuAcHex4HexNAc4dHex-PA; Fig. 7a and Supplementary Table S7). These observations predicted NeuAc2Gal2GlcNAc3Man3FucGlcNAc2 (dN-BIBsF6 or dN-TRF6-1G) as the structure of the A2-24 glycan; in this situation, the linkage pattern between three N-acetylglucosamine residues in antenna structures and two mannose residues in the core structure remained obscure (Fig. 7a and Supplementary Table S7). Moreover, each of the two sialic acid residues can bind to any one of the two galactose residues in the antenna structures. These unresolved issues stem from unavailability of Rcalc and Scalc values owing to a lack of partial elution times related to the N-acetylglucosamines and sialic acid residues. Therefore, the linkage patterns of sialic acid residues were analysed with the combination of SALSA and positive ion mode MALDI-QIT-TOF MS (see Fig. 3). The spectrum showed a clear-cut peak at m/z 2755.11 [M + Na]+ (Fig. 7b; and see Supplementary Fig. S3 and Table S6). The monoisotopic m/z [M + Na]+ value of the A2-24 species without SALSA was calculated on the basis of the data from the LC-ESI-MS and MS2 analyses and was found to be 2672.97 (Fig. 7b). The mass difference (82.14 Da) between these two fractions matched molecular mass of two iPAs (single iPA; 41.06 Da). Accordingly, it was concluded that the glycan carries two α2,6-linked sialic acid residues (Fig. 7c, Table 1, and Supplementary Tables S1 and S2; see also Supplementary Table S6).

The final case is species A3-13 whose characterisation required more complicated analyses (Fig. 8; see also Fig. 3). This strial glycan, which was originally found to have three sialic acid residues by the analyses with three different HPLC types (see Fig. 4a), appeared as a peak at m/z 1160.29 [M + 3 H]3+ in the LC-ESI-MS spectra (Supplementary Fig. S4). Subsequent MS2 analysis detected signals at m/z 844.17 and m/z 1120.01 and predicted that both of these molecular fragments contained a pseudo-Lewis X structure, i.e. GalNAc(GlcNAc)Fuc (Supplementary Table S7). These results suggested that the A3-13 glycan is NeuAc3GalNAc2GalGlcNAc3Fuc2Man3FucGlcNAc2 [trN-d(LdnF)-mLn-M3F6] whose molecular mass is 3477.30 Da. On the other hand, when the sample separated by reversed-phase HPLC was processed with SALSA and assayed with positive ion mode MALDI-QIT-TOF MS, the A3-13 species was detected as a strong peak at m/z 2403.8 [M-H + 2Na]+ (Fig. 8a). This observation indicated that molecular mass of this glycan is 2381.8 Da. The difference between the mass values obtained in these two series of analyses was not explained by SALSA derivatisation. To more precisely profile the A3-13 glycan, we carried out the following experiments. Firstly, the corresponding fraction isolated via reversed-phase HPLC was subjected to negative ion mode MALDI-QIT-TOF MS without SALSA. This analysis identified a signal at m/z 2316.8 [M-H] (Fig. 8b). Then, the original sample was treated with SALSA and assayed by the same MS type, visualizing a peak at m/z 2357.9 [M-H] (Fig. 8c). The difference of 41.1 Da in molecular mass between these two deprotonated ions [M-H] is identical to molecular mass of one iPA (41.06 Da). Accordingly, species A3-13 is likely to contain an α2,6-linked sialic acid residue. Of note, in the MS spectrum of the A3-13 sample without SALSA (Fig. 8b), two other peaks at m/z 2338.8 [M-H] and at m/z 2236.9 [M-H] were detected. The former is likely to represent addition of Na+ to the original glycan observed as the peak at m/z 2316.8 [M-H]. This result indicates that the A3-13 species remained to be deprotonated even when an acidic functional group included in this glycan was neutralised by Na+ binding; in other words, this glycan has multiple acidic functional groups. In addition, even though a sialic acid in the A3-13 species was neutralised by SALSA, this glycan remained to be a deprotonated form [M-H] in negative ion mode MALDI-QIT-TOF MS (Fig. 8c). Taken together, the A3-13 species is likely to harbour at least one acidic functional group that is different from carboxyl group of the sialic acid. In this context, in the MS spectrum obtained from the sample without SALSA (Fig. 8b), the peak at m/z 2236.9 [M-H] was smaller by approximately 80 Da than the native signal of A3-13 species (m/z 2316.8 [M-H]) and the difference is consistent with molecular mass of a sulphate group or a phosphate group. Accordingly, it is plausible that this strial glycan consists of NeuAcGalNAc2GlcNAc2Man3FucGlcNAc2 [6N-BI(dLdn1,2)F6)] (molecular mass: 2237.86) to which either acidic functional group is attached. Furthermore, with MS2 mode we analysed the SALSA-treated fraction, which was detected as a product at m/z 2357.9 [M-H] in negative ion mode MALDI-QIT-TOF MS (Fig. 8c; and see Fig. 3). As shown in Fig. 8d, three marked peaks were detected; the one at m/z 2025.7 [M-H] should result from neutral loss of single iPA-bound sialic acid in the parent ion. Additional lack of one and two HexNAc residue(s) (203.08 Da for one) is likely to result in the other two peaks at m/z 1822.6 [M-H] and m/z 1619.6 [M-H], respectively. The latter seems to represent a glycan of GalNAcGlcNAcMan3FucGlcNAc2 (LdnM3F6) that is sulphated or phosphorylated (Supplementary Table S7). Analysis of this fraction with MS3 assay produced multiple signals (Fig. 8e); difference in molecular mass between a fragment at m/z 1174.3 [M-H] and the parent ion (m/z 1619.6 [M-H]) was likely due to loss of the PA-bound GlcNAc and Fuc at the reducing end. Moreover, it seems probable that the fragment at m/z 971.2 [M-H] was produced by deletion of one HexNAc residue (203.08 Da) from the glycan detected at m/z 1174.3 [M-H] whereas the moiety at m/z 485.1 [M-H] resulted from additional loss of three Hex residues (Fig. 8e). The value of m/z 485.1 [M-H] can be accounted for by molecular mass of GalNAcGlcNAc (406.16 Da) that is modified by a sulphate group or a phosphate group (~80 Da; Fig. 8e). According to the literature34, Gal and HexNAc in N-glycans can be sulphated but not phosphorylated (but see ‘Discussion’). Therefore, we concluded that the functional group in GalNAcGlcNAc is likely to be a sulphate group. Next, the aforementioned fraction with m/z 485.1 [M-H] (GalNAcGlcNAc) was analysed with MS4 and a peak at m/z 282.0 [M-H] was detected in the spectrum (Fig. 8f). This m/z value seems to represent a combination of the mass of a sulphate group (79.96 Da) and that of GalNAc; alternatively, it may denote GlcNAc (203.08 Da; Supplementary Table S7). It is only logical that a sulphate group is attached to the non-reducing terminus of a glycan35; this modification should be the case for the strial A3-13 glycan comprising NeuAcGalNAc2GlcNAc2Man3FucGlcNAc2 [6N-BI(dLdn1,2)F6] (Fig. 8g). This conclusion means no inconsistency for the signal detected at m/z 1160.29 in ESI-MS and MS2 spectra (Fig. 8h and also see Supplementary Fig. S2) when this fraction served as a doubly protonated ion [M + 2 H]2+ instead of a triply protonated form [M + 3 H]3+ that was initially predicted.

### Profiles of strial N-glycans

We finally categorised all the 79 strial N-linked glycans in accordance with their structural profiles as follows. Major vertebrate N-glycans can be categorised into three groups, i.e. high-mannose, complex, and hybrid types, all of which have a common core glycan chain of Man3GlcNAc2. Each type has a different additional sequence as follows30. Firstly, in the high-mannose type, the core is coupled to chains of various lengths composed purely of mannose residues. Secondly, the complex type harbours ‘antennae’ that are initiated by N-acetylglucosaminyltransferases and contain a different combination of other monosaccharides such as N-acetylglucosamine, galactose, fucose, N-acetylgalactosamine, and sialic acid30. Thirdly, in the hybrid type, the chain(s) of only mannose(s) (i.e. high-mannose-type residues) and the complex-type ‘antennae’ are both bound to the core. In addition to these three groups, some strial glycans belong to paucimannose species (Man1–4GlcNAc2Fuc0–1), which does not contain more than four mannoses and any antenna structures (Table 1 and Supplementary Tables S1 and S2)30,31. This type is common in invertebrates and plants but was recently detected in vertebrates as well31,36,37. The 79 strial N-glycans were subjected to this categorisation, and we present in Fig. 9a their amounts normalised to the amount of fraction N-5 (Man6GlcNAc2, i.e. M6). On the basis of this characterisation, we obtained the proportion of each of the four structural types among the 79 glycans. As illustrated in Fig. 9b, the high-mannose type was the most abundant and accounted for 38.1% of the total amount of strial glycans. Complex and hybrid types represented 34.8% and 21.0%, respectively. The least abundant variety was the paucimannose type, which represented 5.8% of the total. As mentioned above, in N-16-2 (GalGlcNAcHexNAc3Man3GlcNAc2), it was unclear whether each of the three HexNAc residues that constitute some non-reducing ends is GlcNAc or GalNAc (Table 1 and Supplementary Tables S1 and S2). Therefore, we could not conclude whether this glycan belongs to the hybrid or complex type. On the other hand, it seems probable that N-21-2 belongs to the complex type, owing to the identified monosaccharide composition at the non-reducing ends (see Table 1 and Supplementary Tables S1 and S2). Sialylation can occur in the hybrid or complex type but not in the high-mannose or paucimannose type38. In the stria vascularis, 43.6% of the total amount of N-glycans had single or multiple sialic acid residues; complex and hybrid types constituted 25.4% and 18.2%, respectively (Fig. 9c). Finally, core fucosylation was detected in 28.4% of the total amount of N-glycans, i.e. 2.6%, 23.3%, and 2.4% were the paucimannose type, complex type, and hybrid type of glycans, respectively (Fig. 9d).

## Discussion

The cochlear stria vascularis, which is essential for hearing, has affinity for some lectin types such as concanavalin A, ulex europaeus agglutinin I, and wheat germ agglutinin39,40,41. Although these observations indicate that this tissue expresses different glycan types, the detailed profile remains unclear. In the present study, a combination of different analytical approaches detected 79 N-linked glycans in the stria vascularis and determined their relative amount (Table 1, Fig. 9a, and Supplementary Tables S1 and S2). In this process, we identified the complete structures of 55 strial glycans and determined partial glycosidic linkage patterns and full monosaccharide composition in the other 24 glycans (Fig. 3b). To our knowledge, such detailed analysis of sugar chains in the stria has not been carried out to date.

The method composed of three HPLC types and LC-ESI-MS is relatively simple and is also used for different samples to analyse their glycans7,28. Nonetheless, this approach seems to have limitations; in particular, it cannot perfectly distinguish sialyl linkage isomers in some cases. In the present study, we additionally treated a few samples with SALSA and clearly distinguished α2,3-linked and α2,6-linked sialic acid residues by mass spectrometry (Figs 3, 7 and 8). Accordingly, the workflow combining this derivatisation and MSn as described in Fig. 3 is an effective and sensitive procedure for characterisation of glycan structures.

A possible application of the glycan library obtained here is to complement other studies as follows. Mumps virus infects the stria vascularis and causes deafness42. In vitro experiments show that neuraminidase in the virus strongly binds unbranched-type NeuAc-Gal-Glucose or NeuAc-Gal-GlcNAc that have the α2,3 sialyl linkage in glycans43. Nevertheless, whether proteins in the stria vascularis harbour either sugar chain has remained elusive. In our list of 79 strial glycans (Table 1 and Supplementary Tables S1 and S2), the latter binding site is included in glycan A1-18-1. This evidence reinforces the current theory about the route of mumps infection and may contribute to elucidation of the pathological process of the deafness. Further comparison of the strial glycan structures shown in this study with different experimental results may expand the repertoire of uses of the library.

In the analysis of glycan A3-13, we concluded that the functional group in GalNAcGlcNAc is a sulphate group (Figs 3 and 8; Supplementary Fig. S2). Nevertheless, a possibility of phosphorylation instead of the sulphation cannot be ruled out completely. In O-glycans, LacdiNAc, which is composed of two HexNAc residues, can be phosphorylated44,45. The same modification may be identified in HexNAc of N-glycans by further study.

Although the methodologies shown in this work are effective at analysing glycan structures, they have several limitations. The first issue is related to liberation of sugar chains from glycoproteins (see ‘Methods’). Anhydrous hydrazine employed in our experiments can extract more divergent glycans regardless of their structures and protein types, as compared to enzymes including peptide N-glycosidase F. Nevertheless, the hydrazinolysis can cleave acyl groups from monosaccharides constituting glycans. Therefore, we re-N-acetylated the samples with acetic anhydride46. These procedures and modifications also affect all the sialic acid residues and prevent us from determining individual types such as N-acetyl, N-glycolyl, and O-acetyl derivatives.

The second limitation lies in the procedure for purification of strial glycans. Trifluoroacetic acid is commonly used to elute acidic glycans from a graphite carbon cartridge loaded with samples47. The reagent is strongly acidic. If the eluates will be next concentrated for some reason, then increased acidification may degrade sugar chains. In this study, the amount of tissues of the stria vascularis was expected to be small (see Fig. 1d), and therefore the samples were processed in a vacuum concentrator. To avoid excess acidification, we added no trifluoroacetic acid but instead ammonium acetate to elution buffer (final concentration: 50 mM), as described in the literature7 (see ‘Methods’). It is noteworthy that the increased salt concentration accelerates a release of numerous glycans from the cartridge but may be ineffective for collection of some highly acidic types.

Thirdly, because 194 standard glycans we used are primarily of the human or zebrafish type, extrapolation of these glycan data to rat strial glycans should be addressed carefully. Moreover, as presented in Fig. 3b, the structures of 24 strial N-glycans could not be completely determined by means of our procedures. To completely resolve these issues, analyses of the samples treated multiple times with different exoglycosidases by mass spectrometry or HPLC48,49 may be useful. This series of assays would require a considerable amount of a sample, and therefore this series was not incorporated here into the workflow for analysis of glycans from the stria vascularis, a tiny tissue (see Fig. 1d). In this context, further experiments may be necessary to validate our procedures.

## Methods

### Isolation of the stria vascularis

All the animal experiments were conducted in compliance with the protocol reviewed by the Institutional Animal Care and Use Committee, were approved by the President of Niigata University (Niigata Univ. Res. 215-2), and were compliant with the ARRIVE guidelines50. Male BN/SsNSIc rats (7 weeks old, 140–180 g; SLC, Hamamatsu, Japan) were used (64 rats total). All the animals were anaesthetised by intraperitoneal injection of sodium pentobarbital (0.5 ml per rat; Nembutal; Abbott, IL, USA). After deep anaesthesia was confirmed by the toe pinch, corneal reflexes, and respiratory rate, in each rat, the heart was surgically exposed and cold saline (100 ml) was infused systemically through the left ventricle (drainage; right atrium). Then, the cochleae were dissected from the temporal bone (Fig. 1b) and washed in the chilled standard solution consisting of NaCl, 140 mM; KCl, 5 mM; HEPES, 10 mM (pH 7.4); D-glucose, 10 mM; MgCl2, 1 mM; CaCl2, 1 mM; and cOmplete Protease Inhibitor Cocktail (1 tablet per 50 ml; Roche, Basel, Switzerland).

The stria vascularis and spiral ligament were isolated under a stereo-microscope as follows. Firstly, the cochlea was sagittally divided using a sharp scalpel, and the bony lateral wall, which contains the stria vascularis and spiral ligament, was manually separated from the organ of Corti and cochlear axis with fine tweezers (Fig. 1c). Secondly, the lateral cochlear wall consisting of the stria and ligament was detached from the bony wall, and the stria, which is identified by brown pigmentation of intermediate cells51 (Fig. 1c), was carefully peeled away from the ligament with a 27-gauge needle (Fig. 1d). Thirdly, the isolated tissues were gently washed with the standard solution. Five to eight pieces of the stria vascularis and ligament (length: 200–1300 μm) were obtained from one cochlea. Samples of respective tissues from 8–10 cochleae were collected in 1.5 ml microtubes and centrifuged at 11432 × g for 1 min at 4 °C (KITMAN-18; TOMY, Tokyo, Japan). After removal of the supernatant, the samples were frozen in liquid nitrogen and stored at −80 °C until use.

### qPCR analyses

Total-RNA samples were extracted from the stria vascularis and spiral ligament isolated from 8–10 cochleae using NucleoSpin RNA XS (TaKaRa Bio, Otsu, Japan). Concentration and quality of RNA were estimated on a 2100 BioAnalyzer (Agilent, Santa Clara, CA, USA); samples whose RNA integrity number exceeded 7.0 were admitted to subsequent experiments. The RNA was processed with Moloney Murine Leukaemia Virus (M-MULV) reverse transcriptase (Invitrogen, Carlsbad, CA). Real-time qPCR was carried out on a LightCycler Nano System (Roche). Expression levels of transcripts of four genes, i.e. Slc12a6 (GenBank accession No. NM_001109630), Pou3f4 (NM_017252), Bsnd (NM_138979), and Cldn11 (NM_053457), which encode KCC3, Brn-4, barttin, and claudin 11, respectively, were compared between the stria vascularis and spiral ligament. The primer sequences have been described in our earlier work12. All the experiments were conducted in duplicate. Quantitative data from PCR with each set of primers were obtained with reference to an internal control gene: glyceraldehyde 3-phosphate dehydrogenase (Gapdh; GenBank accession No. NM_017008). The cDNA template resulting from 5 ng of total RNA was used for the assessment of expression of Slc12a6, Pou3f4, Bsnd, and Cldn11 and that from 1 ng of total RNA was tested for Gapdh. This series of assays was carried out three times with different batches of cochlea samples: 26 cochleae from 13 rats were analysed in total. Each gene expression level was displayed as mean ± SE (n = 3), and differences between the stria vascularis and spiral ligament were evaluated by two-tailed Student’s t test.

### Preparation of pyridylaminated glycans from the stria vascularis

N-glycans were liberated from the strial glycoproteins by hydrazinolysis as described previously29. Pieces of strial tissues that were excised from 102 cochleae (51 rats) and stored separately in 14 tubes were combined in one tube. Next, the samples were lyophilised and heated at 100 °C for 10 h with 1 ml of anhydrous hydrazine (Tokyo Chemical Industry, Tokyo, Japan). After removal of this reagent by repeated evaporation, the glycans were re-N-acetylated with acetic anhydride in a saturated sodium bicarbonate solution and subsequently desalted by passing them through a Dowex 50Wx2 (H+) cation exchanger (Dow Chemicals, Midland, MI, USA). The samples were again lyophilised and then heated at 90 °C for 60 min with 20 µl of a pyridylamination reagent; this reagent was prepared by dissolving 2-aminopyridine (276 mg) in acetic acid (100 µl). Finally, they were heated at 80 °C for 35 min with 70 µl of a reducing reagent, which was a mixture of dimethylamine borate (50 mg), acetic acid (20 µl), and double-distilled water (12.5 µl). In this process, the glycans were tagged with a fluorophore, 2-aminopyridine52,53.

Pyridylaminated (PA)-glycans from the reaction mixture were purified as described elsewhere7,54. The reaction mixture was diluted with 0.15 ml of water and extracted twice using 1 ml of phenol:chloroform (1:1 v/v) to remove the excess reagents and contaminants. The water layer that contained the PA-glycans was purified by gel filtration on a column (1.5 × 18 cm, TSK-gel Toyopearl HW-40F, Tosoh, Tokyo, Japan) equilibrated with 10 mM ammonium acetate pH 6.0. After loading of the sample, the eluate between 10 and 25 ml was collected as the PA-glycan fraction. The PA-glycans were further purified using a graphite carbon cartridge (GL-Pak Carbograph 300 mg; GL Sciences Ltd, Tokyo, Japan). The salt concentration of the glycan mixture was adjusted to 50 mM with ammonium acetate, pH 6.0, and the mixture was loaded onto the cartridge. After a wash with 5 ml of 50 mM ammonium acetate, pH 6.0, the glycans were eluted with 5 ml of 60% acetonitrile in the ammonium acetate buffer. The eluate was concentrated by means of a vacuum concentrator and dried by lyophilisation.

Sample preparation described above was performed in accordance with MIRAGE guidelines55,56.

### HPLC

Three types of HPLC were carried out using a Waters Alliance Waters 2695 separation module and W2475 fluorescence detector (Waters, Milfold, MA) in accordance with MIRAGE guidelines55,56; the detailed information including the parameter settings are described below.

Firstly, the lyophilised strial PA glycans were dissolved in ultra-pure water and analysed at a flow rate of 1.0 ml/min by anion exchange HPLC combined with a TSKgel DEAE-5PW column (0.75 × 7.5 cm; Tosoh, Tokyo, Japan). The column was equilibrated with 0.7 mM aqueous ammonia, pH 9.0. After the samples were injected into the column, the concentration of ammonium acetate was increased linearly to 0.2 M between the time points 5 and 20 min, and then, was further elevated to 0.5 M during the following 10 min. The PA-glycans were detected on a fluorescence spectrophotometer at an excitation wavelength of 310 nm and an emission wavelength of 380 nm. By these procedures, the N-glycans were separated in accordance with the number of attached sialic acid residues, i.e. into fractions N, A1, A2, A3, and A4 (see Fig. 3a and the ‘Results’ section).

Secondly, each fraction (N, A1–A4) was subjected to reversed-phase HPLC, which involved a Cosmosil 5C18-P column (0.2 × 25 cm; Nacalai Tesque, Kyoto, Japan). The flow rate of the samples was 0.2 ml/min. The column was equilibrated with 100 mM triethylamine acetate, pH 4.0, containing 0.075% of 1-butanol. After injection of the sample, the 1-butanol concentration was increased linearly from 0.075% to 0.5% during 105 min. Negative charges of sialic acid residues interfere with separation of samples by reversed-phase HPLC; therefore, in our preparation, they were neutralised by triethylamine, an ion-pairing reagent that has both a positive charge and a hydrophobic moiety. This treatment sharpens the elution profile of acidic N-glycans7. The PA-glycans were detected at an excitation wavelength of 315 nm and an emission wavelength of 400 nm. Areas of all the individual peaks were measured separately32. The most abundant species was N-5. A peak whose area exceeded 2% of that of N-5 was considered significant; thus, 107 fractions were subjected to the next analysis.

Thirdly, the samples were processed by size fractionation HPLC involving a TSK gel Amide 80 column (0.46 × 7.5 cm; Tosoh, Tokyo, Japan) at a flow rate of 0.5 ml/min. The column was equilibrated with 50 mM ammonium formate, pH 4.4, containing 80% acetonitrile. After a sample was injected, acetonitrile concentration was decreased linearly from 80% to 65% during 5 min and then from 65% to 55% over the next 5 min, and finally from 55% to 30% during the subsequent 25 min. PA-glycans were detected using a fluorescence spectrophotometer at an excitation wavelength of 315 nm and an emission wavelength of 400 nm. The peak area of each glycan obtained by this HPLC was determined as follows. When multiple subfractions were extracted from a fraction of the reversed-phase HPLC, an area proportion of each subfraction was calculated. The area of the original fraction was multiplied by each proportion to determine areas of the subfractions. A glycan whose relative amount exceeded 2% of that of N-5 was considered significant; 88 species that satisfied this criterion were subjected to LC-ESI-MS and MS2 (see Fig. 3, Table 1, and Supplementary Tables S1, S2 and S3).

A glycan’s elution time obtained in reversed-phase HPLC was converted to Rstria by means of the reversed-phase scale, and that obtained in size fractionation HPLC was converted to Sstria with the glucose unit, as described elsewhere29,32.

### LC-ESI-MS and MS2 analysis

Mass-spectrometric analysis of PA-glycans was performed by positive-ion mode ESI-MS on an LTQ XL linear ion trap mass spectrometer coupled to a Dionex U3000 HPLC system (Thermo Scientific, San Jose, CA). The fractions isolated through reversed-phase HPLC were trapped on a Hypercarb guard cartridge column (1 × 10 mm; Thermo Scientific, Waltham, MA) for enrichment and separation from contaminants. The samples were eluted with 0.1% (v/v) formic acid in water and 0.5% formic acid in acetonitrile. The flow rate was 50 µl/min, and the gradient conditions were varied for different samples. MS2 analyses of PA-glycans were carried out by collision-induced dissociation in a data-dependent mode or with manually selected parent ion isolation. The peak intensities were extracted in the Mass+ + software ver. 2 (Shimadzu, Kyoto, Japan). All the MS and MS2 spectra are displayed in Supplementary Fig. S2.

Sample preparation and mass-spectrometric analyses described above were performed in accordance with MIRAGE guidelines55,56. Details of the HPLC, MS, and MS2 settings are given in Supplementary Table S8.

### SALSA and multiple MALDI-QIT-TOF mass spectrometry (MSn) analysis

Strial PA-glycan fractions obtained by reversed-phase HPLC were desalted by means of StageTip Carbon composed of Empore SPE carbon disks (Sigma-Aldrich, St. Louis, MO)33. The solvent was removed in vacuo. The glycans included in dried samples were derivatised in a linkage-specific manner in alkylamidation solutions containing iPA and MA33. The samples were dried and re-dissolved in 10 μl of ultra-pure and sterile water. After that, 1 μl of this solution was deposited on a 700 μm μ Focus MALDI plate (Hudson Surface Technology Inc., Old Tappan, NJ) and then mixed with 1 μl of a matrix solution. Composition of this solution is described in Supplementary Table S9. The plate was place on a 75 °C heat block for 1 min to accelerate solvent evaporation. On-plate PA-glycans were analysed by MALDI-QIT-TOF MS (AXIMA-Resonance, Shimadzu/Kratos, Manchester, UK) in positive or negative ion mode. MSn analyses were conducted by collision-induced dissociation with manually selected parent ion isolation. The peak intensities were extracted using Shimadzu Biotech Launchpad ver. 2.9.3 (Kratos Analytical Ltd., Manchester, UK). Of note, the A3-15-2 glycan that was detected as a sole type by HPLC analyses was found to be composed of two species, i.e. A3-15-2-1 and A3-15-2-2, by the procedure combining SALSA and positive ion mode MALDI-MS (Table 1 and Supplementary Fig. S3 and Tables S1, S2 and S6). Relative amounts of each of these two species were calculated via the following three steps. Firstly, as usually detected in the results of mass spectrometry experiments, careful observation revealed that the SALSA derivatised glycan in positive ion mode MALDI-QIT-TOF MS was composed of multiple isotopic peaks; the peaks within 6 Da from the m/z value of the onset of the initial peak were taken as significant signals. All the data points in these significant peaks were analysed, and a total peak intensity was obtained (see ‘MALDI-MS total peak intensity’ in Supplementary Table S2). Secondly, using this value, the proportion of each glycan (i.e. A3-15-2-1 or A3-15-2-2) in the parent fraction, A3-15-2 species, was calculated. Finally, the relative amount of the glycan was determined by multiplying the proportion by the parent’s amount normalised to N-5. With the same procedure, the relative amounts of A3-15-3-1 and A3-15-3-2 species were calculated (Table 1 and Supplementary Tables S1 and S2). Finally, to one glycan (A3-13), MSn analyses were then applied (Fig. 8 and Supplementary Fig. S3 and Table S6).

Sample preparation and mass spectrometry described above were carried out in accordance with MIRAGE guidelines55,56. Information on the MS and MSn settings is shown in Supplementary Table S9.

## Data Availability

All the data generated or analysed during this study are included in this published article or available from the corresponding author on reasonable request.

## References

1. 1.

Wong, C. H. Protein glycosylation: new challenges and opportunities. J. Org. Chem. 70, 4219–4225 (2005).

2. 2.

Apweiler, R., Hermjakob, H. & Sharon, N. On the frequency of protein glycosylation, as deduced from analysis of the SWISS-PROT database. Biochim. Biophys. Acta. 1473, 4–8 (1999).

3. 3.

Zhao, Y. Y. et al. Functional roles of N-glycans in cell signaling and cell adhesion in cancer. Cancer Sci. 99, 1304–1310 (2008).

4. 4.

Scott, H. & Panin, V. M. The role of protein N-glycosylation in neural transmission. Glycobiology. 24, 407–417 (2014).

5. 5.

Hashii, N. et al. Alteration of N‐glycosylation in the kidney in a mouse model of systemic lupus erythematosus: relative quantification of N‐glycans using an isotope‐tagging method. Immunology. 126, 336–345 (2009).

6. 6.

Satomaa, T. et al. Analysis of the human cancer glycome identifies a novel group of tumor-associated N-acetylglucosamine glycan antigens. Cancer Res. 69, 5811–5819 (2009).

7. 7.

Natsuka, S., Masuda, M., Sumiyoshi, W. & Nakakita, S. Improved method for drawing of a glycan map, and the first page of glycan atlas, which is a compilation of glycan maps for a whole organism. PLoS One. 9, e102219, https://doi.org/10.1371/journal.pone.0102219 (2014).

8. 8.

Ishii, A. et al. Developmental changes in the expression of glycogenes and the content of N-glycans in the mouse cerebral cortex. Glycobiology. 17, 261–276 (2007).

9. 9.

Wangemann, P. & Schacht, J. In The Cochlea (eds Dallos, P., Popper, A. N. & Fay, R. R.) 130–185 (Springer, 1996).

10. 10.

Shi, X. Pathophysiology of the cochlear intrastrial fluid-blood barrier (review). Hear Res. 338, 52–63 (2016).

11. 11.

Forrest, D. & Ng, L. In Hearing and Hormones (eds Bass, A. H., Sisneros, J. A., Popper, A. N. & Fay, R. R.) 163–189 (Springer, 2016).

12. 12.

Uetsuka, S. et al. Molecular architecture of the stria vascularis membrane transport system, which is essential for physiological functions of the mammalian cochlea. Eur. J. Neurosci. 42, 1984–2002 (2015).

13. 13.

More, S. S. et al. Role of the copper transporter, CTR1, in platinum-induced ototoxicity. J. Neurosci. 30, 9500–9509 (2010).

14. 14.

Malgrange, B. et al. Expression of growth factors and their receptors in the postnatal rat cochlea. Neurochem. Res. 23, 1133–1138 (1998).

15. 15.

Nishioka, R. et al. Expression of aquaporins and vasopressin type 2 receptor in the stria vascularis of the cochlea. Hear. Res. 260, 11–19 (2010).

16. 16.

Von Bekesy, G. Resting potentials inside the cochlear partition of the guinea pig. Nature. 169, 241–242 (1952).

17. 17.

v. Békésy, G. DC resting potentials inside the cochlear partition. J. Acoust. Soc. Am. 24, 72–76 (1952).

18. 18.

Smith, C. A., Lowry, O. H. & Wu, M. L. The electrolytes of the labyrinthine fluids. Laryngoscope. 64, 141–153 (1954).

19. 19.

Wangemann, P. In Auditory Trauma, Protection, and Repair (eds Schacht, J. & Fay, R. R.) 49–100 (Springer, 2008).

20. 20.

Ciuman, R. R. Stria vascularis and vestibular dark cells: characterisation of main structures responsible for inner-ear homeostasis, and their pathophysiological relations. J Laryngol Otol. 123, 151–162 (2009).

21. 21.

Qiao, L., Han, Y., Zhang, P., Cao, Z. & Qiu, J. Detection of atrial natriuretic peptide and its receptor in marginal cells and cochlea tissues from the developing rats. Neuroendocrinol. Lett. 32, 187–192 (2011).

22. 22.

Sanchez-Calderon, H. et al. RNA microarray analysis in prenatal mouse cochlea reveals novel IGF-I target genes: implication of MEF2 and FOXM1 transcription factors. PloS One. 5, e8699, https://doi.org/10.1371/journal.pone.0008699 (2010).

23. 23.

Estevez, R. et al. Barttin is a Cl channel beta-subunit crucial for renal Cl reabsorption and inner ear K+ secretion. Nature. 414, 558–561 (2001).

24. 24.

Gow, A. et al. Deafness in Claudin 11-null mice reveals the critical contribution of basal cell tight junctions to stria vascularis function. J. Neurosci. 24, 7051–7062 (2004).

25. 25.

Kitajiri, S. et al. Compartmentalization established by claudin-11-based tight junctions in stria vascularis is required for hearing through generation of endocochlear potential. J. Cell. Sci. 117, 5087–5096 (2004).

26. 26.

Minowa, O. et al. Altered cochlear fibrocytes in a mouse model of DFN3 nonsyndromic deafness. Science. 285, 1408–1411 (1999).

27. 27.

Boettger, T. et al. Loss of K-Cl co-transporter KCC3 causes deafness, neurodegeneration and reduced seizure threshold. EMBO J. 22, 5422–5434 (2003).

28. 28.

Hanzawa, K., Suzuki, N. & Natsuka, S. Structures and developmental alterations of N-glycans of zebrafish embryos. Glycobiology. 27, 228–245 (2017).

29. 29.

Natsuka, S. & Hase, S. Analysis of N- and O-glycans by pyridylamination. Methods Mol. Biol. 76, 101–113 (1998).

30. 30.

Stanley, P., Taniguchi, N. & Aebi, M. In Essentials of Glycobiology (eds Varki, A. et al.) 99–111 (Cold Spring Harbor Laboratory, 2015).

31. 31.

Sethi, M. K. & Fanayan, S. Mass spectrometry-based N-glycomics of colorectal cancer. Int. J. Mol. Sci. 16, 29278–29304 (2015).

32. 32.

Yanagida, K., Ogawa, H., Omichi, K. & Hase, S. Introduction of a new scale into reversed-phase high-performance liquid chromatography of pyridylamino sugar chains for structural assignment. J. Chromatogr. A. 800, 187–198 (1998).

33. 33.

Nishikaze, T. et al. Differentiation of sialyl linkage isomers by one-pot sialic acid derivatization for mass spectrometry-based glycan profiling. Anal. Chem. 89, 2353–2360 (2017).

34. 34.

Stanley, P. & Cummings, R. D. Structures Common to Different Glycans in Essentials ofGlycobiology (eds Varki, A. et al.) 161–178 (Cold Spring Harbor Laboratory, 2015).

35. 35.

Van den Eijnden, D. H., Neeleman, A. P., Bakker, H. & Van Die, I. Novel pathways in complex-type oligosaccharide synthesis. New vistas opened by studies in invertebrates in Glycoimmunology 2 (ed. Axford, J. S.) 3–7 (Springer, 1998).

36. 36.

Everest-Dass, A. V. et al. Comparative structural analysis of the glycosylation of salivary and buccal cell proteins: innate protection against infection by Candida albicans. Glycobiology. 22, 1465–1479 (2012).

37. 37.

Parker, B. L. et al. Site-specific glycan-peptide analysis for determination of N-glycoproteome heterogeneity. J. Proteome Res. 12, 5791–5800 (2013).

38. 38.

Slavin, J. Structure, nomenclature, and properties of carbohydrates. In Biochemical, Physiological & Molecular Aspects of Human Nutrition (eds Stipanuk, M. & Caudill, M.) 50–68 (Elsevier, 2012).

39. 39.

Sugiyama, S., Spicer, S. S., Munyer, P. D. & Schulte, B. A. Distribution of glycoconjugates in ion transport cells of gerbil inner ear. J. Histochem. Cytochem. 39, 425–434 (1991).

40. 40.

Yamashita, H. & Bagger-Sjoback, D. Expression of glycoconjugates in the human fetal cochlea. Acta Otolaryngol. 112, 628–634 (1992).

41. 41.

Khan, K. M., Sarfaraz, N. & Salim, Z. Lectin binding patterns in nonsensory regions of rat cochlea during postnatal development. J. Anat. 194(Pt 4), 497–504 (1999).

42. 42.

Cohen, B. E., Durstenfeld, A. & Roehm, P. C. Viral causes of hearing loss: a review for hearing health professionals. Trends Hear. 18, 1–17, https://doi.org/10.1177/2331216514541361 (2014).

43. 43.

Kubota, M. et al. Trisaccharide containingalpha2,3-linked sialic acid is a receptor for mumps virus. Proc. Natl. Acad. Sci. USA 113, 11579–11584 (2016).

44. 44.

Hirano, K., Matsuda, A., Shirai, T. & Furukawa, K. Expression of LacdiNAc groups on N-glycans among human tumors is complex. Biomed. Res. Int. 2014, 981627, https://doi.org/10.1155/2014/981627 (2014).

45. 45.

Breloy, I. et al. O-linked N,N’-diacetyllactosamine (LacdiNAc)-modified glycans in extracellular matrix glycoproteins are specifically phosphorylated at subterminal N-acetylglucosamine. J. Biol. Chem. 287, 18275–18286 (2012).

46. 46.

Yosizawa, Z., Sato, T. & Schmid, K. Hydrazinolysis of alpha-1-acid glycoprotein. Biochim. Biophys. Acta. 121, 417–420 (1966).

47. 47.

Packer, N. H., Lawson, M. A., Jardine, D. R. & Redmond, J. W. A general approach to desalting oligosaccharides released from glycoproteins. Glycoconj. J. 15, 737–747 (1998).

48. 48.

Wang, J. R. et al. A method to identify trace sulfated IgG N-glycans as biomarkers for rheumatoid arthritis. Nat. Commun. 8, 63, https://doi.org/10.1038/s41467-017-00662-w (2017).

49. 49.

Ritchie, G. et al. Identification of N-linked carbohydrates from severe acute respiratory syndrome (SARS) spike glycoprotein. Virology. 399, 257–269 (2010).

50. 50.

Kilkenny, C., Browne, W. J., Cuthill, I. C., Emerson, M. & Altman, D. G. Improving bioscience research reporting: The ARRIVE guidelines for reporting animal research. J. Pharmacol. Pharmacother. 1, 94–99 (2010).

51. 51.

Steel, K. P. & Barkway, C. Another role for melanocytes: their importance for normal stria vascularis development in the mammalian inner ear. Development. 107, 453–463 (1989).

52. 52.

Kuraya, N. & Hase, S. Release of O-linked sugar chains from glycoproteins with anhydrous hydrazine and pyridylamination of the sugar chains with improved reaction conditions. J. Biochem. 112, 122–126 (1992).

53. 53.

Hase, S., Ikenaka, T. & Matsushima, Y. Structure analyses of oligosaccharides by tagging of the reducing end sugars with a fluorescent compound. Biochem. Biophys. Res. Commun. 85, 257–263 (1978).

54. 54.

Natsuka, S., Hirohata, Y., Nakakita, S., Sumiyoshi, W. & Hase, S. Structural analysis of N-glycans of the planarian Dugesia japonica. FEBS J. 278, 452–460 (2011).

55. 55.

Struwe, W. B. et al. The minimum information required for a glycomics experiment (MIRAGE) project: sample preparation guidelines for reliable reporting of glycomics datasets. Glycobiology. 26, 907–910 (2016).

56. 56.

Kolarich, D. et al. The minimum information required for a glycomics experiment (MIRAGE) project: improving the standards for reporting mass-spectrometry-based glycoanalytic data. Mol. Cell. Proteomics. 12, 991–995 (2013).

57. 57.

Nin, F. et al. The endocochlear potential depends on two K+ diffusion potentials and an electrical barrier in the stria vascularis of the inner ear. Proc. Natl. Acad. Sci. USA 105, 1751–1756 (2008).

## Acknowledgements

This work was partially supported by the following research grants and funds: Grants-in-Aid for Scientific Research A 18H04062 (to H.H.), Grants-in-Aid for Young Scientists A 15H05683 (to F.N.), Grants-in-Aid for Young Scientists B 17K17736 (to Sei.S.), and Grants-in-Aid for Scientific Research on Innovative Areas ‘HD Physiology’ 25136704 (to F.N.) from the Ministry of Education, Culture, Sports, Science and Technology of Japan; AMED-CREST 18gm0810004h, AMED (to H.H.); a Grant for Promotion of Niigata University Research Projects 24A006 (to H.H.); grants from The Salt Science Research Foundation ## 1318 and 1549 (to F.N.); the Takeda Science Foundation (to F.N.); the Uehara Memorial Foundation (to F.N.); and Astellas Foundation for Research on Metabolic Disorders (to F.N.).

## Author information

H.H., S.N., F.N., A.H., S.T. and H.I. conceived of this work. S.N., K.H., S.U. and T.H. designed the experiments. Y.N. and S.U. extracted the samples and analysed them by qPCR. S.N., K.H. and Y.N. performed the HPLC and MS analyses. T.N., Sad.S., and E.M. carried out the SALSA and MSn analyses. S.N., Sei.S., T.N., Sad.S., K.H., Y.N., S.O. and E.M. analysed the experimental data. Y.N., Sei.S. and H.H. wrote the manuscript. All the authors reviewed and approved the final manuscript.

Correspondence to Hiroshi Hibino.

## Ethics declarations

### Competing Interests

The authors declare no competing interests.

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

## Rights and permissions

Reprints and Permissions

Nonomura, Y., Sawamura, S., Hanzawa, K. et al. Characterisation of N-glycans in the epithelial-like tissue of the rat cochlea. Sci Rep 9, 1551 (2019). https://doi.org/10.1038/s41598-018-38079-0