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Journal of Experimental Botany logoLink to Journal of Experimental Botany
. 2020 May 29;71(18):5414–5424. doi: 10.1093/jxb/eraa236

Expression of a fungal exo-β-1,3-galactanase in Arabidopsis reveals a role of type II arabinogalactans in the regulation of cell shape

Yoshihisa Yoshimi 1,2, Katsuya Hara 1, Mami Yoshimura 1, Nobukazu Tanaka 3,4, Takumi Higaki 5, Yoichi Tsumuraya 1, Toshihisa Kotake 1,6,✉
Editor: Simon Turner7
PMCID: PMC7501824  PMID: 32470141

We developed a new system that causes specific degradation of type II arabinogalactans by dexamethasone-inducible expression of a fungal exo-β-1,3-galactanase in Arabidopsis, producing severe tissue disorganization in the hypocotyl and cotyledons.

Keywords: Arabidopsis, arabinogalactan-protein, exo-β-1, 3-galactanase, extracellular proteoglycan, fungal enzyme, inducible expression system, Irpex lacteus, tissue disorganization, type II arabinogalactan

Abstract

Arabinogalactan-proteins (AGPs) are a family of plant extracellular proteoglycans implicated in many physiological events. AGP is decorated with type II arabinogalactans (AGs) consisting of a β-1,3-galactan backbone and β-1,6-galactan side chains, to which other sugars are attached. Based on the fact that a type II AG-specific inhibitor, β-Yariv reagent, perturbs growth and development, it has been proposed that type II AGs participate in the regulation of cell shape and tissue organization. However, the mechanisms by which type II AGs participate have not yet been established. Here, we describe a novel system that causes specific degradation of type II AGs in Arabidopsis, by which a gene encoding a fungal exo-β-1,3-galactanase that specifically hydrolyzes β-1,3-galactan backbones of type II AGs is expressed under the control of a dexamethasone-inducible promoter. Dexamethasone treatment increased the galactanase activity, leading to a decrease in Yariv reagent-reactive AGPs in transgenic Arabidopsis. We detected the typical oligosaccharides released from type II AGs by Il3GAL in the soluble fraction, demonstrating that Il3GAL acted on type II AG in the transgenic plants. Additionally, this resulted in severe tissue disorganization in the hypocotyl and cotyledons, suggesting that the degradation of type II AGs affected the regulation of cell shape.

Introduction

Type II arabinogalactans (AGs) are plant-specific glycans generally found as the carbohydrate component of the extracellular proteoglycans called arabinogalactan-proteins (AGPs). In several plants, they have also been detected as side chains of pectin rhamnogalacturonan I and as a secreted polysaccharide in cell walls (Ponder and Richards, 1997; Mohnen, 2008; Caffall and Mohnen, 2009). Although the structures of type II AGs are diverse, depending on plant species, tissue, and developmental stage (Tsumuraya et al., 1988), they universally consist of a β-1,3-galactan backbone and β-1,6-galactan side chains, to which l-Ara and other additional sugars such as GlcA, 4-O-methyl-GlcA (4-O-Me-GlcA), and l-Fuc are attached (Tryfona et al., 2012; Tan et al., 2013). These features distinguish type II AGs from type I AGs which have a β-1,4-galactan backbone (Mohnen, 2008). Because type II AGs can be detected in angiosperms, gymnosperms, ferns, mosses, and liverworts, they have been expected to have important functions throughout the plant kingdom (Jermyn and Yeow, 1975; Clarke et al., 1978).

The participation of type II AGs in various physiological processes has been shown in studies using a specific inhibitor, β-Yariv reagent, which is a phenylazo compound with β-glucosyl or β-galactosyl residues at its termini specifically binding to β-1,3-galactan (Yariv et al., 1962; Kitazawa et al., 2013). In tobacco (Nicotiana tabacum) suspension-cultured cells, treatment with β-Yariv reagent causes extreme cell bulging together with disorganization and depolymerization of cortical microtubules (CMTs) (Sardar et al., 2006). It also strongly inhibits apical cell expansion in the moss Physcomitrella patens (Lee et al., 2005). On the other hand, this does not exclude the possibility that the phenotypes observed in plants treated with β-Yariv reagent are caused, at least in part, by secondary effects of this phenylazo compound, because β-Yariv reagent forms an insoluble precipitate with type II AGs and AGPs in cell walls (Olmos et al., 2017).

Several Arabidopsis (Arabidopsis thaliana) AGP mutants exhibit altered cell shape and tissue disorganization. The salt-overly sensitive5 (sos5)/fasciclin-like agp4 (fla4) mutant, which has a defect in an AGP core protein with fasciclin-like domains, shows root swelling and reduced root growth when treated with a high concentration of NaCl, while it does not show these phenotypes under normal conditions (Shi et al., 2003). Nevertheless, with >80 AGP genes in Arabidopsis, gene redundancy makes it difficult to understand the physiological functions and importance of AGPs based on the study of Arabidopsis knockout lines (Borner et al., 2003; Ma et al., 2017).

It is probable that type II AGs contain physiologically important ‘epitopes’ to participate in various physiological events in plants. In Torenia foumieri, 4-O-Me-GlcA-1,6-Gal (MeGlcAGal), a non-reducing terminal structure of type II AGs, has been shown to function as a signaling factor during fertilization (Mizukami et al., 2016). This signaling factor, called AMOR, confers on pollen tubes the competency to respond to ovular attractant LURE peptides for pollen tube guidance. However, since type II AGs are widely observed in other tissues and organs including the hypocotyl and roots in plants, it is likely that AGs have other distinct biological functions.

As a novel approach in the investigation of the physiological importance and exploration of molecular functions of AGPs, we developed a dexamethasone (Dex)-inducible system for in vivo specific degradation of AG sugar chains using exo-β-1,3-galactanase, a fungal enzyme that causes drastic degradation of type II AGs by hydrolyzing their β-1,3-galactan backbones (Tsumuraya et al., 1990; Kotake et al., 2009). With this system, we observed severe tissue disorganization in the hypocotyl and cotyledons of transgenic Arabidopsis when the degradation of type II AG was induced by treatment with Dex (Aoyama and Chua, 1997), indicating that type II AG plays an essential role in cell morphology.

Materials and methods

Materials

The β-1,3-galactan substrate for exo-β-1,3-galactanase from Ilpex lacteus (Il3GAL) was prepared from gum arabic (Acacia senegal; Sigma-Aldrich Japan, Tokyo, Japan) by Smith degradation as described previously (Goldstein et al., 1956; Kitazawa et al., 2013). Radish root and leaf AGPs were extracted and purified from radish (Raphanus sativus L.) as described previously (Shimoda et al., 2014; Inaba et al., 2015). The polyclonal antibody raised against a partial sequence of Il3GAL, GGGDQTYSYTDTKI, was purchased from Eurofins Genomics (Tokyo, Japan). The polyclonal antibody serum from rabbit was subjected to ammonium sulfate precipitation, and the 20–40% saturated fraction was used for western blotting.

Preparation of recombinant Il3GAL and point-mutated rIl3GAL

Il3GAL (accession number AB461394) was cloned in a previous study (Kotake et al., 2009). To generate the point-mutated Il3GAL (Il3GAL-PM) gene, the point mutation E102A that replaces the conserved Glu with Ala was introduced by PCR using the primers Il3GAL-PM-F and Il3GAL-PM-R (see Supplementary Table S1 at JXB online). For expression in Pichia pastoris, the Il3GAL and Il3GAL-PM fragments were subcloned into pPICZαC plasmid (Invitrogen, Waltham, MA, USA). The methylotrophic P. pastoris (Pichia yeast) strain KM71H (Invitrogen) was then transformed by electroporation with the constructs, Il3GAL/pPICZαC or Il3GAL-PM/pPICZαC. The transformants were selected based on zeocine resistance and cultured in YPG medium containing 1% (w/v) yeast extract, 2% (w/v) peptone, and 1% (w/v) glycerol at 30 °C with shaking at 90 rpm for 2 d. The cells were collected by centrifugation at 1500 g for 5 min, washed with ice-cold water, and suspended in 50 ml of YP medium containing 1% (w/v) yeast extract and 2% (w/v) peptone. The expression of recombinant enzymes was induced by 1% (v/v) methanol, and the yeast was cultured for another 5 d with addition of 1% (v/v) methanol each day. After centrifugation at 1500 g for 5 min, the supernatant was collected as crude enzyme. The recombinant Il3GAL (rIl3GAL) and recombinant Il3GAL-PM (rIl3GAL-PM) were purified from crude enzyme solution by size exclusion chromatography and ion-exchange chromatography as described previously (Kotake et al., 2009). The purity of rIl3GAL and rIl3GAL-PM was examined by SDS–PAGE (Laemmli, 1970).

Generation of transgenic plants and Dex treatment

Arabidopsis ecotype Columbia (Col-0) was used in the present study. The cDNA for the Il3GAL or Il3GAL-PM sequence without the part corresponding to its signal peptide was PCR amplified using KOD2 DNA polymerase (Toyobo, Tokyo, Japan) and the set of primers, Il3GAL-F+BamHI and Il3GAL-R+SpeI (Supplementary Table S1) (Kotake et al., 2009). The cDNA sequence corresponding to the signal sequence of Arabidopsis AGP4 (At5g10430) was PCR amplified with the primers AtAGP4-F+XhoI and AtAGP4-R+BamHI (Supplementary Table S1). These two fragments were fused using the BamHI site. The resulting fragment, AGP4 signal sequence–Il3GAL, was subcloned between the XhoI and SpeI sites of pTA7001 (Aoyama and Chua, 1997). To generate Dex::Il3GAL and Dex::Il3GAL-PM plants, the gene constructs were introduced into Arabidopsis by agrobacterium-mediated (Rhizobium radiobacter, EHA105 strain) transformation (Clough and Bent, 1998). Transformants were selected using Murashige and Skoog (MS) medium (Murashige and Skoog, 1962) containing 20 µg ml–1 hygromycin B and 50 µg ml–1 carbenicillin. The hygromycin B-resistant seedlings were isolated as individual transgenic lines. For the present study, five independent transgenic lines (#1, 2, 3, 4, and 5) for Dex::Il3GAL plants and nine independent transgenic lines (#1, 2, 3, 4, 5, 6, 7, 8, and 9) for Dex::Il3GAL-PM plants were obtained. Homozygous plants of the T3 generation were used in all experiments. Plants were grown at 22 °C under continuous light. For the analysis of galactanase activity, the plants were first grown on MS agar medium for 2 weeks, then treated with a solution containing 10 μM Dex and 0.1% DMSO for 2 d. As the negative control, plants were treated with 0.1% DMSO solution. To observe phenotypes, Arabidopsis seeds were sown on MS agar medium containing 0.1, 1, or 10 μM Dex, and the plants were grown for a week.

Semi-quantitative analysis of Il3GAL mRNAs

The relative expression level of Il3GAL in Dex::Il3GAL plants was estimated by semi-quantitative reverse transcription–PCR (RT–PCR). Total RNA was extracted from Arabidopsis seedlings treated with Dex for 0.5, 1, 3, 6, 12, or 24 h with an Isogen kit (Nippon Gene, Tokyo, Japan). Single-stranded cDNA was synthesized from total RNA using oligo(dT)12–18 primer. A set of specific primers, Il3GAL-QPCR-F and Il3GAL-QPCR-R (Supplementary Table S1), for Il3GAL was designed using the Primer3 program (http://bioinfo.ut.ee/primer3-0.4.0/). As the internal control, the expression level of ACTIN2 (At3g18780) was measured with a set of specific primers, ACT2-RTP-F and ACT2-RTP-R (Supplementary Table S1). The PCR was performed with a SYBR Premix Ex Taq kit (Takara Bio Inc., Otsu, Japan) under the following conditions: 10 s denaturing at 95 °C, 30 s annealing at 60 °C, and 20 s amplification at 72 °C, 40 cycles.

Measurement of galactanase activity in transgenic plants

The galactanase activity of rIl3GAL and rIl3GAL-PM was measured with a reaction mixture containing 1 mg ml–1 β-1,3-galactan prepared from gum arabic, 50 mM sodium acetate buffer (pH 5.0), and rIl3GAL and rIl3GAL-PM at 37 °C. The reducing sugars were measured colorimetrically by the neocuproine method (Dygert et al., 1965). One unit of enzyme activity is capable of producing 1 µmol of reducing power from the substrate per minute.

To measure the galactanase activity in the transgenic plants, the seedlings of Dex::Il3GAL and Dex::Il3GAL-PM plants treated with 10 μM Dex were ground in 20 mM sodium acetate buffer (pH 5.0) with a mortar and pestle and centrifuged at 10 000 g. The resulting supernatant was collected as the soluble fraction. The pellet was resuspended in the same buffer containing 1 M NaCl at 4 °C for 1 h and then centrifuged. The resulting supernatant was collected as the cell wall-bound fraction. The galactanase activity of soluble and cell wall-bound fractions was measured using 1 mg ml–1 β-1,3-galactan as substrate as described above.

Western blotting

Il3GAL and Il3GAL-PM proteins induced by treatment with Dex in the transgenic Arabidopsis were detected by western blotting. As Il3GAL and Il3GAL-PM fused with the signal peptide of Arabidopsis AGP4 are designed to be secreted to cell walls in the transgenic plants, these proteins can be collected in the soluble fraction. Two-week-old plants treated with 10 μM Dex and 0.1% DMSO for 2 d were ground with a pestle in 20 mM sodium acetate buffer (pH 5.0). After centrifugation at 10 000 g, the supernatant was collected and subjected to SDS–PAGE. The Il3GAL protein in the gel was transferred to a polyvinylidene difluoride membrane and then detected with anti-Il3GAL antibody (rabbit IgG) as the primary antibody (1:2000 dilution) and a horseradish peroxidase-conjugated anti-rabbit IgG antibody (GE Healthcare Life Sciences, Chicago, IL, USA) as the secondary antibody (1:10 000 dilution). Chemi Doc XRS (Bio-Rad, Tokyo, Japan) was used to detect chemiluminescence.

Quantification of type II AGs

Plants treated with Dex were ground in 50 mM MOPS-KOH buffer (pH 6.5) and boiled for 30 min. After centrifugation, the supernatant was collected as the hot water (HW)-soluble fraction. The amount of type II AGs in the HW-soluble fraction was determined by radial gel diffusion assay with a gel containing 40 µg ml–1 β-Gal-Yariv, 150 mM sodium chloride, 0.02% (w/v) sodium azide, and 1% (w/v) agarose (van Holst and Clarke, 1985).

Detection and identification of oligosaccharides

For the analysis of action of recombinant enzymes expressed in Pichia yeast, rIl3GAL and rIl3GAL-PM were reacted with 1 mg ml–1 AGPs from radish leaves in 50 mM sodium acetate buffer (pH 5.0) at 37 °C. Released Gal and oligosaccharides were derivatized with p-aminobenzoic acid ethyl ester (ABEE; Wako, Osaka, Japan) (Matsuura and Imaoka, 1988), and detected by HPLC as previously described (Yoshimi et al., 2017). ABEE-labeled isomaltooligosaccharides (IMOs) were used as molecular makers for the elution positions (Konishi et al., 2007).

For the identification of type II AG-derived oligosaccharides in the transgenic plants, the soluble fraction was prepared from 230–500 mg of Dex::Il3GAL and Dex::Il3GAL-PM plants grown on MS agar medium containing 10 μM Dex. Oligosaccharides included in the soluble fraction were labeled with ABEE and detected by HPLC as described above. ABEE-labeled oligosaccharides were further digested with α-l-arabinofuranosidase from Aspergillus niger (Arafase) from Megazyme and/or recombinant β-glucuronidase from Aspergillus niger expressed in P. pastoris (GlcAase) as described previously (Konishi et al., 2008).

The standard oligosaccharides were prepared and purified as previously described (Shimoda et al., 2014). AGPs from radish roots were first hydrolyzed into oligosaccharides with 80 mU of rIl3GAL and 80 mU of recombinant endo-β-1,3-galactanase from Neurospora crassa (rNcEn3GAL), which were expressed in P. pastoris, at 37 °C overnight (Yoshimi et al., 2017). The resulting hydrolysate including oligosaccharides was applied to a Sephadex G-100 column to remove polysaccharides. The oligosaccharides were fractionated into neutral and acidic oligosaccharide fractions by anion exchange chromatography using a DEAE-cellulose (SERVA, Heidelberg, Germany) column (HCO3–, 2.2×8 cm). The neutral and acidic fractions were desalted by DOWEX 50Wx8 (Dow Chemical Company, Midland, MI, USA) and lyophilized.

Preparation of cross-sections and observation by SEM

Preparation of cross-sections was performed as described previously with minor modifications (Nitta et al., 2009; Abedi et al., 2018). Briefly, 7-day-old seedlings treated with Dex were pre-fixed in 2% glutaraldehyde in 0.1 M sodium phosphate buffer (pH 7.4) at room temperature for 2 h and at 4 °C overnight. After rinsing in the buffer, seedlings were post-fixed in the buffer containing 2% OsO4 on ice for 2 h and then dehydrated in a graded ethanol series. The post-fixed samples were substituted with an ethanol:propylene oxide mixture (1:1, v/v) once and with propylene oxide twice, then embedded in EPOK 812 resin (Oken Shoji, Tokyo, Japan). Semi ultra-thin sections (~500 nm in thickness) were cut with a glass knife on an Ultracut N ultramicrotome (Reichert Technologies, Depew, NY, USA) and stained by dipping in 0.01% (w/v) toluidine blue O solution for a minute followed by gentle removal of the stain.

For SEM observation, pre-fixed samples were lyophilized with a FDC10 freezer and FD6510 freeze dryer (SUN Technologies, Alpharetta GA, USA), and sputter-coated with platinum. The samples were visualized using a JSM 5610 scanning elctron microscope (JEOL, Tokyo, Japan) at an accelerating voltage of 5 kV.

Results

Properties of exo-β-1,3-galactanase, Il3GAL, and its point-mutated form in vitro

Although their structures are diverse and heterogeneous, almost all type II AGs have a β-1,3-galactan backbone in common. Exo-β-1,3-galactanase, Il3GAL, is a fungal enzyme from I. lacteus, which specifically hydrolyzes the β-1,3-galactan backbones of type II AGs (Tsumuraya et al., 1990; Kotake et al., 2009). Il3GAL differs from plant endogenous enzymes such as β-galactosidase and α-l-arabinofuranosidase (Kotake et al., 2005, 2006), as it causes drastic degradation of type II AGs by hydrolyzing the β-1,3-galactan backbone irrespective of the β-1,6-galactan side chains (Fig. 1). As the result of action by Il3GAL, type II AGs are hydrolyzed into oligosaccharides derived from the β-1,6-galactan side chains (Tsumuraya et al., 1990; Tryfona et al., 2012; Inaba et al., 2015). In the present study, in vivo specific degradation by Il3GAL introduced into Arabidopsis was examined. Since, however, it was conceivable that the presence of Il3GAL itself generated stress in the plants, because Il3GAL is a fungal protein, we compared the effect with a negative control, Il3GAL-PM, which has the mutation E102A at its conserved residue (Fig. 2A) (Ichinose et al., 2005; Kotake et al., 2009). To confirm the loss of activity of Il3GAL-PM, rIl3GAL and rIl3GAL-PM were prepared by expression in Pichia yeast (Fig. 2B). The rIl3GAL expressed in Pichia yeast appeared as two bands with relative molecular masses of 54 kDa and 49 kDa on SDS–PAGE, which is larger than that (45 520 Da) predicted from the amino acid sequence. This can be explained as we have shown in a previous study that the apparent molecular mass of rIl3GAL shifts to 45 kDa after removal of N-glycans, and we conclude that the protein bands observed here are indeed rIl3GAL in different states of N-glycosylation (Gemmill and Trimble, 1999; Kotake et al., 2009; Strasser,S 2016)

Fig. 1.

Fig. 1.

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Model structure of type II AG and action of Il3GAL. A model structure of type II AG is shown. Il3GAL, represented by an arrowhead, hydrolyzes β-1,3-galactan backbones irrespective of β-1,6-galactan side chains from non-reducing terminal residues, which results in drastic breakdown of type II AGs, releasing various oligosaccharides derived from the side chains. l-Araf, l-arabinofuranose.

Fig. 2.

Fig. 2.

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Enzymatic activity of rIl3GAL and rIl3GAL-PM. (A) Point mutation in the catalytic site of Il3GAL. The Glu residue was replaced with Ala to generate rIl3GAL-PM. (B) The purity of recombinant proteins. The rIl3GAL and rIl3GAL-PM proteins were examined by SDS–PAGE. Proteins in the gel were stained with Coomassie Brilliant Blue R-250. Arrows indicate rIl3GAL and rIl3GAL-PM. (C) Galactanase activity. The activity of recombinant enzymes was measured using β-1,3-galactan as substrate. Data are mean values ±SD (n=3 technical replicates). (D) Released oligosaccharides from radish leaf AGPs by the action of rIl3GAL or rIl3GAL-PM. Enzymatic hydrolysis products were derivatized with ABEE and detected by HPLC. Arrows indicate oligosaccharides as follows: a, Gal; b, MeGlcAGal; c, Gal2; d, l-Ara-β-1,6-Gal2; e, MeGlcAGal2; f, Gal3; g, AraGal3. Asterisks indicate oligosaccharides released from type II AGs but not assigned. The elution positions of glucose and IMOs with degree of polymerization (DP) 2–6 are indicated on the top.

While rIl3GAL exhibited strong hydrolytic activity (13.3 U mg–1 protein) towards β-1,3-galactans, releasing various β-1,6-galactooligosaccharides derived from side chains from radish leaf AGPs, rIl3GAL-PM did not show measurable activity (<0.001 U mg–1 protein), resulting in no released oligosaccharide from radish leaf AGPs in vitro (Fig. 2C, D).

In vivo degradation of type II AGs by means of a fungal enzyme

Using the Il3GAL gene, we accomplished the specific degradation of type II AGs in vivo under the control of a Dex-inducible promoter in Arabidopsis. To ensure the secretion of Il3GAL in muro, the signal sequence of Il3GAL was replaced with that of Arabidopsis AGP4 (Supplementary Fig. S1). We designated the transgenic Arabidopsis Dex::Il3GAL.

In Dex::Il3GAL plants, the galactanase activity toward β-1,3-galactan rapidly increased under treatment in a dose-dependent manner, whereas no increase was observed in the wild type (WT) (Fig. 3A; Supplementary Fig. S2), indicating that galactanase activity could be regulated by Dex concentration. In fact, the expression of the Il3GAL gene occurred within 1 h after Dex treatment and reached a maximum at 24 h (Fig. 3B). Western blot analysis using antibody raised against an Il3GAL peptide also confirmed that Il3GAL protein was produced by Dex treatment in the transgenic plants (Fig. 3C).

Fig. 3.

Fig. 3.

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Il3GAL expression induced by Dex in planta. (A) Galactanase activity in Dex::Il3GAL plants treated with Dex. Dex::Il3GAL and Dex::Il3GAL-PM plants were first grown in the absence of Dex for 2 weeks and then treated with 10 µM Dex for 2 d. The negative controls were treated with 0.1% DMSO solution for 2 d. Values indicate the total activity obtained from the soluble and wall-bound fractions. F.W., fresh weight. Data are mean values ±SD (n=3 biological replicates). Asterisks indicate significant differences between plants with and without Dex treatment (Student’s t-test, *P<0.05; **P<0.01). (B) Induction of the Il3GAL gene. Dex::Il3GAL #2 plants grown in the absence of Dex were treated with 10 µM Dex for 0.5, 1, 3, 6, 12, 24, and 48 h. The expression level of Il3GAL was determined by semi-quantitative RT–PCR. The values are shown as expression levels relative to ACTIN2. Data are mean values ±SD (n=3 biological replicates). (C) Detection of Il3GAL and Il3GAL-PM. Il3GAL and Il3GAL-PM proteins in the soluble fraction were detected by western blotting using anti-Il3GAL antibody. The arrow indicates Il3GAL or Il3GAL-PM protein.

On the other hand, in Dex::Il3GAL-PM transgenic plants, galactanase activity was almost unchanged from that of the WT, and, as was expected, they did not show increased activity after Dex treatment (Fig. 3A). The weak activity observed probably resulted from endogenous β-galactosidases (Kotake et al., 2005). Accumulation of Il3GAL and Il3GAL-PM proteins was confirmed immunologically, indicating that Dex::Il3GAL-PM plants were suitable as a negative control (Fig. 3C).

Degradation of AGP in transgenic plants

To evaluate the degree of type II AG degradation, a radial gel diffusion assay with β-Yariv reagent was performed. As β-Yariv reagent binds to any β-1,3-galactan backbone that is larger than β-1,3-galactopentaose (Kitazawa et al., 2013), β-Yariv reactivity can be used to estimate the amount of β-1,3-galactans in the samples. The soluble fraction, which includes most AGPs, was prepared from Dex::Il3GAL plants and subjected to Yariv assay (Fig. 4A). In Dex::Il3GAL plants #1 and #2 grown in the presence of Dex, the amount of β-Yariv reagent-reactive (β-Yariv-reactive) AGPs was drastically reduced (42% and 72%, respectively, were lost compared with the amount in plants grown in the absence of Dex), whereas Dex::Il3GAL-PM and WT plants did not show a significant change under Dex treatment (Fig. 4B).

Fig. 4.

Fig. 4.

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Degradation of type II AGs in muro. (A) β-Yariv-reactive type II AGs in the transgenic plants. A radial gel diffusion assay with β-Yariv reagent was performed with the soluble fraction. Representative results for WT, Dex::Il3GAL #2 and #3, and Dex::Il3GAL-PM #2 and #3 are shown here. (B) Estimated amount of type II AGs. The area of the halo formed by β-Yariv-reactive type II AGs was calculated and plotted. Data are mean values ±SD (n=3 biological replicates). Asterisks indicate significant differences between amounts with and without Dex treatment (Student’s t-test, *P<0.05; **P<0.01).

While plant endogenous glycoside hydrolases including β-galactosidase and α-l-arabinofuranosidase only act on non-reducing terminal residues of type II AGs releasing monosaccharides, Il3GAL causes dramatic degradation by directly hydrolyzing the β-1,3-galactan backbone, which releases the oligosaccharides from side chains. In order to confirm that the enzyme functioned in transgenic plants, we measured oligosaccharides by HPLC. In the soluble fraction of Dex::Il3GAL plants treated with Dex, we identified an accumulation of specific oligosaccharides typical for type II AGs, such as β-1,6-galactotriose (Gal3), 4-O-Me-GlcA-β-1,6-Gal2 (MeGlcAGal2), l-arabinosyl-Gal3 (AraGal3), and 4-O-Me-GlcA-β-1,6-Gal3 (MeGlcAGal3) (Fig. 5A) (Tryfona et al., 2012; Tan et al., 2013; Shimoda et al., 2014). In addition to these neutral and acidic oligosaccharides, we detected at least six non-assigned oligosaccharides that were susceptible to β-glucuronidase and/or α-l-arabinofuranosidase digestion, indicating that β-glucuronidated or α-l-arabinosylated oligosaccharides, which are also typically found in type II AG, were released in the transgenic plants (Fig. 5B; Supplementary Fig. S3). Because these AG-specific oligosaccharides were not observed in either WT or Dex::Il3GAL-PM plants with Dex treatment, or in Dex::Il3GAL plants without Dex treatment, we conclude that they must have been liberated as a result of the hydrolysis of type II AGs by Il3GAL.

Fig. 5.

Fig. 5.

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Identification of oligosaccharides liberated from type II AGs in vivo. (A) Chromatogram of detected oligosaccharides liberated from type II AGs by the action of Il3GAL. The oligosaccharides in the soluble fraction were derivatized with ABEE and detected by HPLC. Arrows indicate liberated oligosaccharides as follows: e, MeGlcAGal2; f, Gal3; g, AraGal3; h, MeGlcAGal3; i, Gal4; j, MeGlcA-β-1,6-Gal4; k, β-1,6-galactopentaose. Asterisks indicate oligosaccharides released from type II AGs but not assigned. The elution positions of glucose and IMOs with DP 2–8 are indicated on the top. (B) Enzymatic digestion of AG oligosaccharides. The labeled oligosaccharides were digested with GlcAase (+GlcAase), Arafase (+Arafase), or both enzymes (+GlcAase +Arafase). The elution positions of β-1,6-galactooligosaccharides and MeGlcA-β-1,6-galactooligosaccharides are shown in Supplementary Fig. S3.

Tissue disorganization in the hypocotyl

Four out of five lines of Dex::Il3GAL plants (#1–#3 and #5) showed abnormal morphology in hypocotyls and cotyledons when grown on MS agar medium containing 0.1–10 μM Dex under light conditions (Fig. 6; Supplementary Fig. S4). Under dark conditions, the elongation of etiolated hypocotyls was also significantly decreased (11–56%) in all lines of the Dex-treated Dex::Il3GAL plants (Supplementary Fig. S5). Consistent with the galactanase activity, the abnormal morphology was enhanced by increased concentrations of Dex in the growth medium. Observation by SEM revealed extreme bulging of some epidermal cells of the hypocotyl (Fig. 6I). In the cross-sections of hypocotyls of #2 plants, abnormally large cells were found not only in the epidermis, but also in the cortex and endodermis, resulting in severe tissue disorganization in the hypocotyl, while no abnormally enlarged cells were observed in the vascular tissues (Fig. 6H). Because WT and Dex::Il3GAL-PM plants did not show any change under Dex treatment, it can be assumed that the degradation of type II AGs was the cause of these distinctive phenotypes (Fig. 6A–F, J–L). These results therefore indicate that the type II AGs play an important role in regulation of the cell morphology. The differences in appearance and varying extent of disorganization in the phenotypes of transgenic lines may result from different expression patterns and levels of Il3GAL.

Fig. 6.

Fig. 6.

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Tissue disorganization in the transgenic plants. WT plants treated with Dex (A–C), Dex::Il3GAL plants grown without Dex (D–F), Dex::Il3GAL plants treated with Dex(G–I), and Dex::Il3GAL-PM plants treated with Dex (J–L) were observed. Plants were grown on MS agar medium containing 0.1 μM Dex for 7 d under continuous light before analysis. (A, D, G, J) Stereoscope images of seedlings. Scale bar=1 mm. Plants treated with different Dex concentrations are shown in Supplementary Fig. S4. (B, E, H, K) Cross-sections of the middle region of the hypocotyl stained with toluidine blue O. Scale bar=100 µm. Ep, epidermis; Co, cortex; En, endodermis. (C, F, I, L) SEM images of hypocotyls. Scale bar=100 μm.

Effect of exogenous application of type II AG oligosaccharides

We considered the possibility that cell bulging and tissue disorganization were caused by accumulation of Gal or oligosaccharides released from type II AGs by the action of Il3GAL. It has been reported that a high concentration of monomeric Gal inhibits cell elongation (Yamamoto et al., 1988; Dörmann and Benning, 1998; Rösti et al., 2007). In order to examine whether the Gal and oligosaccharides produced by the action of Il3GAL caused the growth defects, we prepared a hydrolysate of Arabidopsis AGP by rIl3GAL in vitro and applied it to WT plants growing in MS medium. However, the application of hydrolysate did not mimic the tissue disorganization phenotypes of Dex::Il3GAL plants (Supplementary Fig. S6). This suggests that the reduced amount of type II AGs, rather than the released oligosaccharides, caused the tissue disorganization.

Discussion

Specific degradation of type II AGs in vivo

Type II AGs are the second most complex polysaccharides after pectin rhamnogalacturonan II in plants. Type II AGs mainly consist of Gal and l-Ara, but also possess other sugars such as GlcA, 4-O-Me-GlcA, l-Fuc, l-Rha, and Xyl, which differ depending on plant species, tissue, and age (Tsumuraya et al., 1988). Heterogeneous carbohydrate structures make functional analysis difficult. In AGPs from radish, wheat (Triticum aestivum L.), and pear (Pyrus communis L), the length of β-1,6-galactan side chains varies from one to >20 (Tryfona et al., 2010; Shimoda et al., 2014; Tsumuraya et al., 2019). Therefore, in the past, the specific in vitro fragmentation of type II AGs into oligosaccharides using microbial hydrolases such as exo-β-1,3-galactanase and endo-β-1,6-galactanase has been an effective approach to obtain structural information (Tryfona et al., 2010, 2012; Shimoda et al., 2014; Inaba et al., 2015).

The present study is the first attempt to achieve specific degradation of type II AGs in vivo. Il3GAL is quite specific to β-1,3-galactan, as it never acts on glycans including carboxymethyl-curdlan (β-1,3-glucan), β-1,4-galactan, pectic arabinan, and xylan (Tsumuraya et al., 1990; Kotake et al., 2009). Therefore, it is unlikely that Il3GAL induced by Dex hydrolyzed glycans other than type II AGs in Dex::Il3GAL plants. We found that in some of these plants, the amount of β-Yariv-reactive type II AGs decreased to as little as 30%. On the other hand, this observation indicates that ~30% of type II AGs remained and were not hydrolyzed by Il3GAL. It is probable that in some tissues the expression of Il3GAL gene was not induced by Dex treatment. It is also possible that some of the type II AGs were resistant to hydrolysis by Il3GAL. In a previous study, we have observed that rIl3GAL expressed in Pichia yeast had weak activity toward gum arabic (acacia gum), which contains β-1,3-galactans highly substituted with short β-1,6-galactan side chains (Kotake et al., 2009). Type II AGs having such a structure, if present, would not be hydrolyzed in vivo by Il3GAL.

Inhibitory effect of type II AG degradation in planta

It has been suggested that type II AGs are implicated in a wide range of physiological processes in plants (Park et al., 2003; Lee et al., 2005). However, most information about the physiological importance of type II AGs so far comes from studies using β-Yariv reagent and/or Arabidopsis knockout lines. Our system instead works by specific and controlled degradation of type II AGs in vivo. Several phenotypes we observed, including cell bulging and tissue disorganization, were similar to those of Arabidopsis roots treated with β-Yariv reagent and the knockout fla4/sos5 mutant under salt stress (Willats and Knox, 1996; Shi et al., 2003), indicating that the Dex treatment caused inhibition of AGP functions in Dex::Il3GAL plants. In addition, severe tissue disorganization in the hypocotyl and cotyledons, which has not been reported in AGP mutants under normal conditions, was observed in Dex::Il3GAL plants. The reason for this may well be that the drastic degradation of type II AGs occurred not only in surface tissues but also in tissues such as the cortex and endodermis. Indeed, in Dex::Il3GAL #2 plants, ~70% of β-Yariv-reactive type II AGs were lost, which should lead to many kinds of AGPs losing their native functions. The present study also shows the practical advantage of the Dex-inducible system, because this system allows controlled analysis of the influence of Il3GAL expression, which causes severe and lethal phenotypes when fully unleashed.

If the system presented in this study is to serve as a new tool in the study of the functions of type II AGs and AGPs, we need to consider to what extent the accumulation of Il3GAL protein induced by Dex treatment may have directly affected the phenotypes. Indeed, we observed a dwarf phenotype in one line (#6) of Dex::Il3GAL-PM plants out of nine lines (Supplementary Figs S4, S5). However, the severe tissue disorganization occurring in four lines (#1, #2, #3, and #5) of Dex::Il3GAL plants was not observed in any lines of Dex::Il3GAL-PM plants, suggesting that tissue disorganization resulted from the degradation of type II AGs by Il3GAL, rather than protein accumulation.

Participation of type II AGs in tissue organization

Plant cell shape is primarily determined by the orientation of cellulose microfibrils. Deposition of cellulose microfibrils involves CMTs, along which cellulose synthase complexes move within the plane of the plasma membrane. It is conceivable that the degradation of type II AGs influences the orientation and/or stabilization of CMTs. In fact, depolymerization and disorganization of CMTs together with cell bulging are caused by treatment with β-Yariv reagent in tobacco cultured cells (Sardar et al., 2006). Moreover, similar disorganization of CMTs and swelling were also reported in Arabidopsis roots treated with β-Yariv reagent for 24 h (Nguema-Ona et al., 2007). To examine the possibility that degradation of type II AGs affects CMTs, CMTs were observed in Dex::Il3GAL #2 plants by introducing a gene encoding microtubule-associated protein (MAP) 65-1 fused with green fluorescence protein (GFP) (Lucas et al., 2011; Soga et al., 2018). In a time course experiment, the change in the orientation of CMTs occurred along with that in cell shape 48 h after the Dex treatment (Supplementary Fig. S7). Although the degradation of type II AGs significantly influenced CMTs, the change in CMTs may have been brought about indirectly by the change in cell shape. We note that the change observed in CMTs in Dex::Il3GAL #2 plants was milder than that in Arabidopsis mutants impaired in the regulation of CMTs such as mor1 and clasp (Whittington et al., 2001; Ambrose et al., 2007, 2011).

In conclusion, we have developed a novel approach to achieve the specific degradation of type II AGs in vivo. Using this system, we were able to show that type II AGs are physiologically important and participate in the organization of hypocotyl and cotyledon tissues. Future studies will aim to identify the carbohydrate structure(s) responsible for these biologically relevant functions of type II AGs. It may well be that specific structures in type II AGs play important roles in cellulose synthesis. Because Il3GAL hydrolyzed the β-1,3-galactan backbone causing drastic overall degradation of type II AGs, the identification of the structures essential for the physiological function of type II AGs was not within the scope of the present study. Further approaches using other hydrolases that specifically act on type II AGs, including endo-β-1,6-galactanase and β-glucuronidase, will help to identify such important carbohydrate structures.

Supplementary data

Supplementary data are available at JXB online.

Table S1. List of primers used in this study.

Fig. S1. Gene constructs for the generation of Dex::Il3GAL and Dex::Il3GAL-PM plants.

Fig. S2. Dose-dependent increase in galactanase activity.

Fig. S3. The elution positions of standard β-1,6-galactooligo saccharides and MeGlcA-β-1,6-galactooligosaccharides.

Fig. S4. Phenotype of Dex::Il3GAL and Dex::Il3GAL-PM plants.

Fig. S5. Length of etiolated hypocotyls of Dex::Il3GAL and Dex::Il3GAL-PM plants.

Fig. S6. Effect of AG oligosaccharides liberated by rIl3GAL on seedlings

Fig. S7. Effects of degradation of type II AGs on CMTs.

eraa236_suppl_Supplementary_Material
Click here for additional data file. (925.1KB, pdf)

Acknowledgements

We thank Ms Kanae Koike for technical assistance and Professor Nam-Hai Chua for providing pTA7001 plasmid. We are also grateful to Dr Federico López Hernández for critical reading of the manuscript. This work was supported by MEXT KAKENHI Grant-in-Aid for Scientific Research on Innovative Areas ‘Plant-Structure Optimization Strategy’ to TK [no. 18H05495] and to TH [no. 18H05492], Grant-in-Aid for Scientific Research on Innovative Areas-Resource and technical support platforms for promoting research ‘Advanced Bioimaging Support’ to TH [no. 16H06280], Grant-in-Aid for Scientific Research to TK [no. 19K06702], and JSPS Grant-in-Aid for JSPS Fellows to YY [no. 16J05924].

Glossary

Abbreviations

ABEE

p-aminobenzoic acid ethyl ester

Arafase

α-l-arabinofuranosidase from Aspergillus niger

AG

arabinogalactan

AGP

arabinogalactan-protein

l-Araf

l-arabinofuranose

AraGal3

l-arabinosyl-β-1,6-galactotriose

CMT

cortical microtubule

Dex

dexamethasone

Gal2

β-1,6-galactobiose

Gal3

β-1,6-galactotriose

Gal4

β-1,6-galactotetraose

GFP

green fluorescence protein

GlcAase

recombinant β-glucuronidase from Aspergillus niger

Il3GAL

exo-β-1,3-galactanase from Irpex lacteus

IMO

isomaltooligosaccharide

4-O-MeGlcA

4-O-methyl-GlcA

MeGlcAGal

MeGlcA-β-1,6-Gal

MeGlcAGal2

MeGlcA-β-1,6-Gal2

MeGlcAGal3

MeGlcA-β-1,6-Gal3

MS

Murashige and Skoog

rIl3GAL

recombinant Il3GAL

rIl3GAL-PM

point-mutated rIl3GAL

rNcEn3GAL

recombinant endo-β-1,3-galactanase from Neurospora crassa

WT

wild-type.

Author contributions

YY, YT, and TK designed the research; YY, MY, KH, NT, and TK performed the research; YY, TH, YT, and TK analyzed the data; YY, TH, and TK wrote the paper.

Conflict of interest

The authors declare no conflict of interest.

References

  1. Abedi T, Khalil MFM, Koike K, Hagura Y, Tazoe Y, Ishida N, Kitamura K, Tanaka N. 2018. Expression of the human UDP-galactose transporter gene hUGT1 in tobacco plants’ enhanced plant hardness. Journal of Bioscience and Bioengineering 126, 241–248. [DOI] [PubMed] [Google Scholar]
  2. Ambrose C, Allard JF, Cytrynbaum EN, Wasteneys GO. 2011. A CLASP-modulated cell edge barrier mechanism drives cell-wide cortical microtubule organization in Arabidopsis. Nature Communications 2, 430. [DOI] [PMC free article] [PubMed] [Google Scholar]
  3. Ambrose JC, Shoji T, Kotzer AM, Pighin JA, Wasteneys GO. 2007. The Arabidopsis CLASP gene encodes a microtubule-associated protein involved in cell expansion and division. The Plant Cell 19, 2763–2775. [DOI] [PMC free article] [PubMed] [Google Scholar]
  4. Aoyama T, Chua NH. 1997. A glucocorticoid-mediated transcriptional induction system in transgenic plants. The Plant Journal 11, 605–612. [DOI] [PubMed] [Google Scholar]
  5. Borner GH, Lilley KS, Stevens TJ, Dupree P. 2003. Identification of glycosylphosphatidylinositol-anchored proteins in Arabidopsis. A proteomic and genomic analysis. Plant Physiology 132, 568–577. [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Caffall KH, Mohnen D. 2009. The structure, function, and biosynthesis of plant cell wall pectic polysaccharides. Carbohydrate Research 344, 1879–1900. [DOI] [PubMed] [Google Scholar]
  7. Clarke AE, Gleeson PA, Jermyn MA, Knox RB. 1978. Characterization and localization of β-lectins in lower and higher plants. Australian Journal of Plant Physiology 5, 707–722. [Google Scholar]
  8. Clough SJ, Bent AF. 1998. Floral dip: a simplified method for Agrobacterium-mediated transformation of Arabidopsis thaliana. The Plant Journal 16, 735–743. [DOI] [PubMed] [Google Scholar]
  9. Dörmann P, Benning C. 1998. The role of UDP-glucose epimerase in carbohydrate metabolism of Arabidopsis. The Plant Journal 13, 641–652. [DOI] [PubMed] [Google Scholar]
  10. Dygert S, Li LH, Florida D, Thoma JA. 1965. Determination of reducing sugar with improved precision. Analytical Biochemistry 13, 367–374. [DOI] [PubMed] [Google Scholar]
  11. Gemmill TR, Trimble RB. 1999. Overview of N- and O-linked oligosaccharide structures found in various yeast species. Biochimica et Biophysica Acta 1426, 227–237. [DOI] [PubMed] [Google Scholar]
  12. Goldstein IJ, Hay GW, Lewis BA, Smith F. 1956. Controlled degradation of polysaccharides by periodate oxidation, reduction, and hydrolysis. Methods in Carbohydrate Chemistry 5, 361–370. [Google Scholar]
  13. Ichinose H, Yoshida M, Kotake T, Kuno A, Igarashi K, Tsumuraya Y, Samejima M, Hirabayashi J, Kobayashi H, Kaneko S. 2005. An exo-β-1,3-galactanase having a novel β-1,3-galactan-binding module from Phanerochaete chrysosporium. Journal of Biological Chemistry 280, 25820–25829. [DOI] [PubMed] [Google Scholar]
  14. Inaba M, Maruyama T, Yoshimi Y, Kotake T, Matsuoka K, Koyama T, Tryfona T, Dupree P, Tsumuraya Y. 2015. l-Fucose-containing arabinogalactan-protein in radish leaves. Carbohydrate Research 415, 1–11. [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Jermyn MA, Yeow YM. 1975. A class of lectins present in the tissues of seed plants. Australian Journal of Plant Physiology 2, 501–531. [Google Scholar]
  16. Kitazawa K, Tryfona T, Yoshimi Y, et al. 2013. β-Galactosyl Yariv reagent binds to the β-1,3-galactan of arabinogalactan proteins. Plant Physiology 161, 1117–1126. [DOI] [PMC free article] [PubMed] [Google Scholar]
  17. Konishi T, Kotake T, Soraya D, Matsuoka K, Koyama T, Kaneko S, Igarashi K, Samejima M, Tsumuraya Y. 2008. Properties of family 79 β-glucuronidases that hydrolyze β-glucuronosyl and 4-O-methyl-β-glucuronosyl residues of arabinogalactan-protein. Carbohydrate Research 343, 1191–1201. [DOI] [PubMed] [Google Scholar]
  18. Konishi T, Kotake T, Tsumuraya Y. 2007. Chain elongation of pectic β-(1→4)-galactan by a partially purified galactosyltransferase from soybean (Glycine max Merr.) hypocotyls. Planta 226, 571–579. [DOI] [PubMed] [Google Scholar]
  19. Kotake T, Dina S, Konishi T, Kaneko S, Igarashi K, Samejima M, Watanabe Y, Kimura K, Tsumuraya Y. 2005. Molecular cloning of a β-galactosidase from radish that specifically hydrolyzes β-(1→3)- and β -(1→6)-galactosyl residues of Arabinogalactan protein. Plant Physiology 138, 1563–1576. [DOI] [PMC free article] [PubMed] [Google Scholar]
  20. Kotake T, Kitazawa K, Takata R, Okabe K, Ichinose H, Kaneko S, Tsumuraya Y. 2009. Molecular cloning and expression in Pichia pastoris of a Irpex lacteus exo-β-(1→3)-galactanase gene. Bioscience, Biotechnology, and Biochemistry 73, 2303–2309. [DOI] [PubMed] [Google Scholar]
  21. Kotake T, Tsuchiya K, Aohara T, Konishi T, Kaneko S, Igarashi K, Samejima M, Tsumuraya Y. 2006. An α-l-arabinofuranosidase/β-d-xylosidase from immature seeds of radish (Raphanus sativus L.). Journal of Experimental Botany 57, 2353–2362. [DOI] [PubMed] [Google Scholar]
  22. Laemmli UK. 1970. Cleavage of structural proteins during the assembly of the head of bacteriophage T4. Nature 227, 680–685. [DOI] [PubMed] [Google Scholar]
  23. Lee KJ, Sakata Y, Mau SL, Pettolino F, Bacic A, Quatrano RS, Knight CD, Knox JP. 2005. Arabinogalactan proteins are required for apical cell extension in the moss Physcomitrella patens. The Plant Cell 17, 3051–3065. [DOI] [PMC free article] [PubMed] [Google Scholar]
  24. Lucas JR, Courtney S, Hassfurder M, Dhingra S, Bryant A, Shaw SL. 2011. Microtubule-associated proteins MAP65-1 and MAP65-2 positively regulate axial cell growth in etiolated Arabidopsis hypocotyls. The Plant Cell 23, 1889–1903. [DOI] [PMC free article] [PubMed] [Google Scholar]
  25. Ma Y, Yan C, Li H, Wu W, Liu Y, Wang Y, Chen Q, Ma H. 2017. Bioinformatics prediction and evolution analysis of arabinogalactan proteins in the plant kingdom. Frontiers in Plant Science 8, 1–17. [DOI] [PMC free article] [PubMed] [Google Scholar]
  26. Matsuura F, Imaoka A. 1988. Chromatographic separation of asparagine-linked oligosaccharides labeled with an ultraviolet-absorbing compound, p-aminobenzoic acid ethyl. Glycoconjugate Journal 5, 13–26. [Google Scholar]
  27. Mizukami AG, Inatsugi R, Jiao J, et al. 2016. The AMOR arabinogalactan sugar chain induces pollen-tube competency to respond to ovular guidance. Current Biology: CB 26, 1091–1097. [DOI] [PubMed] [Google Scholar]
  28. Mohnen D. 2008. Pectin structure and biosynthesis. Current Opinion in Plant Biology 11, 266–277. [DOI] [PubMed] [Google Scholar]
  29. Murashige T, Skoog F. 1962. A revised medium for rapid growth and bio assay with tobacco tissue cultures. Physiologia Plantarum 15, 473–497. [Google Scholar]
  30. Nguema-Ona E, Bannigan A, Chevalier L, Baskin TI, Driouich A. 2007. Disruption of arabinogalactan proteins disorganizes cortical microtubules in the root of Arabidopsis thaliana. The Plant Journal 52, 240–251. [DOI] [PubMed] [Google Scholar]
  31. Nitta K, Nagayama K, Danev R, Kaneko Y. 2009. Visualization of BrdU-labelled DNA in cyanobacterial cells by Hilbert differential contrast transmission electron microscopy. Journal of Microscopy 234, 118–123. [DOI] [PubMed] [Google Scholar]
  32. Olmos E, García De La Garma J, Gomez-Jimenez MC, Fernandez-Garcia N. 2017. Arabinogalactan proteins are involved in salt-adaptation and vesicle trafficking in tobacco BY-2 cell cultures. Frontiers in Plant Science 8, 1092. [DOI] [PMC free article] [PubMed] [Google Scholar]
  33. Park MH, Suzuki Y, Chono M, Knox JP, Yamaguchi I. 2003. CsAGP1, a gibberellin-responsive gene from cucumber hypocotyls, encodes a classical arabinogalactan protein and is involved in stem elongation. Plant Physiology 131, 1450–1459. [DOI] [PMC free article] [PubMed] [Google Scholar]
  34. Ponder GR, Richards GN. 1997. Arabinogalactan from western larch, Part III: alkaline degradation revisited, with novel conclusions on molecular structure. Carbohydrate Polymers 34, 251–261. [Google Scholar]
  35. Rösti J, Barton CJ, Albrecht S, Dupree P, Pauly M, Findlay K, Roberts K, Seifert GJ. 2007. UDP-glucose 4-epimerase isoforms UGE2 and UGE4 cooperate in providing UDP-galactose for cell wall biosynthesis and growth of Arabidopsis thaliana. The Plant Cell 19, 1565–1579. [DOI] [PMC free article] [PubMed] [Google Scholar]
  36. Sardar HS, Yang J, Showalter AM. 2006. Molecular interactions of arabinogalactan proteins with cortical microtubules and F-actin in Bright Yellow-2 tobacco cultured cells. Plant Physiology 142, 1469–1479. [DOI] [PMC free article] [PubMed] [Google Scholar]
  37. Shi H, Kim Y, Guo Y, Stevenson B, Zhu JK. 2003. The Arabidopsis SOS5 locus encodes a putative cell surface adhesion protein and is required for normal cell expansion. The Plant Cell 15, 19–32. [DOI] [PMC free article] [PubMed] [Google Scholar]
  38. Shimoda R, Okabe K, Kotake T, Matsuoka K, Koyama T, Tryfona T, Liang HC, Dupree P, Tsumuraya Y. 2014. Enzymatic fragmentation of carbohydrate moieties of radish arabinogalactan-protein and elucidation of the structures. Bioscience, Biotechnology, and Biochemistry 78, 818–831. [DOI] [PubMed] [Google Scholar]
  39. Soga K, Yamazaki C, Kamada M, et al. 2018. Modification of growth anisotropy and cortical microtubule dynamics in Arabidopsis hypocotyls grown under microgravity conditions in space. Physiologia Plantarum 162, 135–144. [DOI] [PubMed] [Google Scholar]
  40. Strasser R. 2016. Plant protein glycosylation. Glycobiology 26, 926–939. [DOI] [PMC free article] [PubMed] [Google Scholar]
  41. Tan L, Eberhard S, Pattathil S, et al. 2013. An Arabidopsis cell wall proteoglycan consists of pectin and arabinoxylan covalently linked to an arabinogalactan protein. The Plant Cell 25, 270–287. [DOI] [PMC free article] [PubMed] [Google Scholar]
  42. Tryfona T, Liang HC, Kotake T, et al. 2010. Carbohydrate structural analysis of wheat flour arabinogalactan protein. Carbohydrate Research 345, 2648–2656. [DOI] [PubMed] [Google Scholar]
  43. Tryfona T, Liang HC, Kotake T, Tsumuraya Y, Stephens E, Dupree P. 2012. Structural characterization of Arabidopsis leaf arabinogalactan polysaccharides. Plant Physiology 160, 653–666. [DOI] [PMC free article] [PubMed] [Google Scholar]
  44. Tsumuraya Y, Mochizuki N, Hashimoto Y, Kovac P. 1990. Purification of an exo-β-(1→3)-d-galactanase of Irpex lacteus (Polyporus tulipiferae) and its action on arabinogalactan-proteins. Journal of Biological Chemistry 265, 7207–7215. [PubMed] [Google Scholar]
  45. Tsumuraya Y, Ogura K, Hashimoto Y, Mukoyama H, Yamamoto S. 1988. Arabinogalactan-proteins from primary and mature roots of radish (Raphanus sativus L.). Plant Physiology 86, 155–160. [DOI] [PMC free article] [PubMed] [Google Scholar]
  46. Tsumuraya Y, Ozeki E, Ooki Y, Yoshimi Y, Hashizume K, Kotake T. 2019. Properties of arabinogalactan-proteins in European pear (Pyrus communis L.) fruits. Carbohydrate Research 485, 107816. [DOI] [PubMed] [Google Scholar]
  47. van Holst GJ, Clarke AE. 1985. Quantification of arabinogalactan-protein in plant extracts by single radial gel diffusion. Analytical Biochemistry 148, 446–450. [DOI] [PubMed] [Google Scholar]
  48. Whittington AT, Vugrek O, Wei KJ, Hasenbein NG, Sugimoto K, Rashbrooke MC, Wasteneys GO. 2001. MOR1 is essential for organizing cortical microtubules in plants. Nature 411, 610–613. [DOI] [PubMed] [Google Scholar]
  49. Willats WG, Knox JP. 1996. A role for arabinogalactan-proteins in plant cell expansion: evidence from studies on the interaction of β-glucosyl Yariv reagent with seedlings of Arabidopsis thaliana. The Plant Journal 9, 919–925. [DOI] [PubMed] [Google Scholar]
  50. Yamamoto R, Inouhe M, Masuda Y. 1988. Galactose inhibition of auxin-induced growth of mono- and dicotyledonous plants. Plant Physiology 86, 1223–1227. [DOI] [PMC free article] [PubMed] [Google Scholar]
  51. Yariv J, Rapport MM, Graf L. 1962. The interaction of glycosides and saccharides with antibody to the corresponding phenylazo glycosides. The Biochemical Journal 85, 383–388. [DOI] [PMC free article] [PubMed] [Google Scholar]
  52. Yoshimi Y, Yaguchi K, Kaneko S, Tsumuraya Y, Kotake T. 2017. Properties of two fungal endo-β-1,3-galactanases and their synergistic action with an exo-β-1,3-galactanase in degrading arabinogalactan-proteins. Carbohydrate Research 453-454, 26–35. [DOI] [PubMed] [Google Scholar]

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Supplementary Materials

eraa236_suppl_Supplementary_Material
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