- freely available
Int. J. Mol. Sci. 2014, 15(6), 11030-11039; doi:10.3390/ijms150611030
Published: 18 June 2014
Abstract: Plant chitinases have been studied for their importance in the defense of crop plants from pathogen attacks and for their peculiar vacuolar sorting determinants. A peculiarity of the sequence of many family 19 chitinases is the presence of a C-terminal extension that seems to be important for their correct recognition by the vacuole sorting machinery. The 7 amino acids long C-terminal vacuolar sorting determinant (CtVSD) of tobacco chitinase A is necessary and sufficient for the transport to the vacuole. This VSD shares no homology with other CtVSDs such as the phaseolin’s tetrapeptide AFVY (AlaPheValTyr) and it is also sorted by different mechanisms. While a receptor for this signal has not yet been convincingly identified, the research using the chitinase CtVSD has been very informative, leading to the observation of phenomena otherwise difficult to observe such as the presence of separate vacuoles in differentiating cells and the existence of a Golgi-independent route to the vacuole. Thanks to these new insights in the endoplasmic reticulum (ER)-to-vacuole transport, GFPChi (Green Fluorescent Protein carrying the chitinase A CtVSD) and other markers based on chitinase signals will continue to help the investigation of vacuolar biogenesis in plants.
Over the past few decades, glycosyl hydrolases of families 18 and 19, commonly known as chitinases (EC 188.8.131.52), have been studied for their importance in the defense of crop plants from pathogen attacks and for their peculiar vacuolar sorting determinants. While family 18 chitinases are found in all organisms, family 19 chitinases are mostly found in plants, although they have been found in a few animals, fungi, protists and in many bacteria. Until January 2014, 3374 chitinase DNA sequences were present in the NCBI database while the Pfam database revealed for Viridiplantae 569 sequences from 111 species for family 18 and 1047 sequences from 204 species for family 19 chitinases. They catalyze the hydrolysis of internal β-1,4-bonds between monomers of N-acetylglucosamine of chitin, the major cell wall structural polysaccharide of many fungi. This activity can evidently contribute to the defenses against fungal pathogens.
Unfortunately, the chitinases in cultivated plants can also have negative effects on human health since they may trigger allergic responses. Chitinases are major allergens in several food plants like banana, avocado or apple, as well as in rubber. Like many allergens, they are resistant to proteolytic degradation in the acidic environment of the stomach. This resistance favors entry into the bloodstream triggering the allergic response. The use of heterologous chitinases to engineer pathogen-resistant crop plants requires that the proteins are suitably modified to be optimized for pathogen resistance as well as to be properly hydrolyzed in an acidic environment .
Full understanding of the post-translational modifications (PTMs) of the engineered transgenic product is necessary both for the development of plants over-expressing defense proteins, and for the increase of nutritional value. Glycosylation certainly possesses a considerable importance, being the most abundant PTM in plant cells  and the most frequent post-translational modification related to the allergenic potential. However chitinases are rarely glycosylated. The catalytic domain shows a lysozyme-like folding in which two glutamates, Glu67 (number in barley chitinase) located in the third helix and Glu89 located in a more variable loop-like structure, act as main reactive groups for the inverting acid-base catalysis . Additionally, Glu203 and Arg215 are both coordinated with Glu67. Not surprisingly, a similar triplet is shared with glycosyl hydrolases of families 46 (chitosanases) and 17 (β-1,3-glucanases) .
Family 19 chitinases have been subdivided in seven classes depending on the presence of a chitin-binding domain and on the presence of four loops within the catalytic domain. X-ray structures of several plant class I and II chitinases indicate a compact fold of the catalytic domain where the C-terminus is extended along the surface in such a way that additional residues would stick out over the catalytic cleft [5,6]. It is thus to be expected that the C-terminal propeptides found in many vacuolar class I chitinases are easily accessible to the sorting machinery as well as easily removed by endo- or exo-peptidases.
2. Chitinase Sorting, a Hidden Path
The vacuolar sorting determinant (VSD) residing in the C-terminal 7 amino acids long propeptide of tobacco chitinase A is both necessary and sufficient for the transport to the vacuole . Fusion of this C-terminal propeptide to enzymatic or fluorescent reporters (rat β-glucuronidase and Green Fluorescent Protein (GFP)) confirmed these early evidences [8,9]. Only few other C-terminal VSDs (CtVSD) have been demonstrated to be involved in vacuolar sorting: a barley lectin , a β-1,3-glucanase and an osmotin from tobacco [11,12,13], 2S albumin storage proteins from Brazil nut , pea  and bean phaseolin .
Contrary to ssVSDs (sequence-specific Vacuolar Sorting Determinants, as identified, e.g., in barley for aleurain or sweet potato for sporamin), no specific sequence motif is needed for vacuolar sorting and different amino-acid substitutions led to different efficiencies of delivery to the vacuole. The importance of the C-terminus for the sorting machinery is stressed by the fact that the C-terminal Met of chitinase A could be replaced by a Phe or a Lys or even deleted, but not replaced by a Gly . Similarly, addition of 1 or 2 Gly to the barley lectin propeptide or C-terminal addition of an N-glycosylation site caused a total secretion of the lectin .
The tobacco chitinase VSD has been less widely used than another C-terminal targeting signal, the tetrapeptide AlaPheValTyr (AFVY) from bean phaseolin . There is no homology between these two CtVSDs but they now appear also to be sorted by different mechanisms . The research using the chitinase CtVSD has been very informative, leading to the observation of otherwise neglected phenomena, such as the possible formation of two ontogenically distinct vacuoles , the presence of separate vacuoles in differentiating cells  and the existence of a Golgi-independent route to vacuoles .
Vacuoles are multifunctional organelles showing a high plasticity according to physiological/environmental needs [20,21]. The coexistence of two functionally and morphologically distinct vacuoles in single plant cells was confirmed by several studies involving different species [22,23,24,25]. Distinct vacuoles with different contents can certainly answer to specific physiological needs [19,25]. There is still a debate whether they derive by fragmentation from a pre-existing unique vacuole or develop from different prevacuolar compartments [26,27,28,29]. In some cases, as in programmed cell death (PCD) during pathogen response, vacuoles can fragment and acquire new functions that require specific membrane characteristics . As for distinct biogenesis pathways, de Marchis and co-workers  recently reviewed several Golgi-independent pathways involved in the trafficking of different types of vacuolar proteins.
A recent electron microscopy study of Arabidopsis thaliana root tips using trafficking inhibitors  supports a model in which the lytic vacuole tonoplast forms from membranes derived from the endoplasmic reticulum, forming (empty) provacuoles. Similar models for the de novo biogenesis of a lytic vacuole had already been suggested long ago [33,34]. The provacuoles fuse with the pre-existing vacuolar network. Soluble contents then fill the vacuoles by the classical route via the Golgi. This corresponds well with the pattern observed with mini-protoplasts regenerating their central vacuole , when using the fluorescent vacuolar marker AleuGFP targeted with the sequence-specific VSD (ssVSD) of barley aleurain, a marker for lytic vacuoles, but not to what could be seen with the fluorescent vacuolar reporter GFPChi targeted with the CtVSD of tobacco chitinase-A . This study also revealed that the regenerating central vacuole responsible for cell turgor is generated mainly by the lytic vacuolar compartment, labeled by AleuGFP. In contrast, GFPChi labeled small peripheral vacuoles, which we called pre-vacuoles. These fused with the central vacuole in a second step, probably at the end of cell expansion. In transgenic Arabidopsis plants expressing either marker, it could be seen that in nascent and expanding root hairs the central vacuole was labeled by AleuGFP, while GFPChi was excluded, while in fully expanded root hairs the latter marker also made it to the central vacuole . This observation was not confirmed by other research groups using other vacuolar markers but can now be better understood considering the recent data  showing that GFPChi is a marker of a Sar1-independent traffic to the central vacuole. In our opinion, the central vacuole initially formed in mini-protoplasts  was filled by the standard Sar1-dependent pathway only, while the Sar1-independent pathway formed peripheral pre-vacuoles, supporting the idea of ontogenically distinct vacuoles.
In Arabidopsis plants accumulating anthocyanins, Brefeldin A (BFA) treatment did not alter the trafficking of either anthocyanins or GFPChi while it affected the trafficking of AleuGFP . Similarly, for the enzymatic marker rat β-glucuronidase fused to the chitinase CtVSD (RGUSChi) it was wortmannin and not BFA that completely impaired vacuolar targeting in protoplasts . The drug BFA is often used to demonstrate the involvement of Golgi in vacuolar trafficking (for a review see ) but it is also acting on endosomal compartments and on recycling to the plasmalemma, causing the formation of BFA bodies . Recent results in Nicotiana , indirectly confirmed in tomato , indeed suggest that GFPChi transits via an intermediate compartment independent from the trans-Golgi Network (TGN) but involved in the late events of BFA bodies formation.
Other studies have however convincingly argued that GFPChi follows the canonical pathway through the Golgi–TGN–PVC (PreVacuolar Compartment). The functional studies of AtVPS45  and AtVTI12  showed that these proteins influence GFPChi sorting but mutants do not fully impair its transport to the central vacuole leaving open the possibility of a close interaction between the two pathways. Both AtVPS45 and AtVTI12 are positive regulators for vacuolar trafficking of cargoes carrying a CtVSD, being responsible for fusion processes at the tonoplast: AtVPS45 is a member of Sec1/Munc18 family and forms with AtVTI12 SNARE a multimeric complex also including SYP41/SYP61. In a vps45 null mutant, the vacuole forms small concentric multilayer compartments stressing the involvement of post-Golgi trafficking in provacuole release and/or provacuole fusion  and opening to future model re-interpretation. The authors did not exclude the interference of an unbalanced SNARE (soluble N-ethylmaleimide-sensitive factor associated protein receptor) complex, composed of VAMP727, SYP22, VTI11, and SYP51. In fact it is known that the absence of both SYP22 and VAMP727 lead to vacuole fragmentation . Over-expression of AtSYP51 also specifically interferes with GFPChi sorting to the vacuole [43,44]. SYP51 belongs to a new functional class of SNAREs with interfering activity, the i-SNAREs . The i-SNARE activity of SYP51 is not shared by other related SNAREs such as SYP61  and may be related to vacuole separation. SYP51 was localized on compartments of a different nature , which are distinct from Golgi and differently associated with free TGN , multivesicular bodies (MVB) (colocalizing with TGN and PVC markers) or tonoplast. For the investigation and characterization of the endoplasmic reticulum (ER)-to-vacuole pathways it is essential to identify valuable markers, such as chitinase. Even so many years after the discovery of the latter’s vacuolar targeting, the thorough study of the related-marker GFPChi leaves many unanswered questions.
A main issue is that putative vacuolar sorting receptor(s) for CtVSD proteins have been identified, but their sorting mechanism remains unclear. The CtVSD are not specifically recognized by the well-characterized Vacuolar Sorting Receptors (VSRs), which have a strong affinity for ssVSD [47,48]. These receptors have a similar structure to other vacuolar or lysosomal sorting receptors in animals or yeast, with a luminal cargo-binding domain, a single transmembrane domain and a short cytosolic tail with sorting signals controlling their incorporation into coated vesicles . In 2000 , a new class of putative receptors, the RMRs (Receptor-like Membrane RING-H2), was identified in Arabidopsis based on the homology of its PA (Protease Associated) domain, with the PA domain, which is a part of the cargo-binding luminal domain of VSRs. In vitro binding assays of the luminal domain of RMRs have demonstrated an affinity for CtVSDs and not for ssVSDs, supporting their role as vacuolar sorting receptors for CtVSDs involved in sorting to the storage vacuole [50,51,52]. Co-immunoprecipitation and in vitro binding assays of AtRMR1 with phaseolin also support an in vivo interaction between proteins with a CtVSD and some members of the RMR family  (For a review on RMRs, see ). GFPChi may be targeted to the vacuole in an aggregated form as already shown for phaseolin [54,55]. The localization of RMRs is not clear yet: they have been localized in a DIP-labeled organelle (Dark Intrinsic Protein ), in the vacuolar lumen , in a new type of prevacuolar compartment  or different isoforms in either ER or a prevacuolar compartment (Occhialini, Gouzerh and Neuhaus, manuscript in preparation). These different results may be due to the different experimental approaches or organisms used and the discrepancies remain to be resolved.
The unclear results about sorting of markers with the chitinase A CtVSD suggests the existence of two different pathways for the chitinase: a classical pathway passing via the Golgi and the TGN and an alternative pathway in which soluble cargoes exit the ER by another Sar1-independent mechanism, delivering cargoes to the vacuoles without passing through the Golgi . This pathway seems particularly important in developing seeds and involves the formation of dense vesicles. Already in 1993 Hara-Nishimura and co-workers demonstrated the existence of such an alternative pathway for the accumulation of 2S albumin and 11S globulins in pumpkin seeds via dense precursor-accumulating compartment (PAC) vesicles . Over the years the number of proteins seen to bypass the Golgi has increased, including also the calcineurin B-like proteins , γ-gliadins , α-globulins , legumin-1 . In rice, the formation of two distinct types of protein storage vacuoles involves the formation of PAC-like vesicles and of a new prevacuolar compartment [52,60].
In vivo observation of tobacco (Figure 1) or Arabidopsis protoplasts expressing GFPChi fluorescent shows that this marker is distributed among ER, punctate structures, and in either small vacuoles or in the central vacuole. In developing seeds, GFPChi accumulates in dense vesicles, while such vesicles are not observed in germinating cotyledons and GFPChi accumulates in ER bodies (Giselbert Hinz, unpublished observations). In vegetative tissues these dense vesicles do not seem to exist. How CtVSD proteins are sorted in these tissues remains to be determined. Combined with the use of new pathway selective inhibitors , GFPChi will continue to help dissect the mechanisms of vacuolar biogenesis in plants.
G.-P. Di Sansebastiano activity was supported by the Italian national grant PON a3_00334. J.-M. Neuhaus was supported by the Swiss National Science Foundation grant FN 31003A-141257.
E. Stigliano wrote the first draft of this manuscript, which was then revised by the two other authors and finalized by J.-M. Neuhaus.
Conflicts of Interest
The authors declare no conflict of interest.
- Thomas, K.; Aalbers, M.; Bannon, G.A.; Bartels, M.; Dearman, R.J.; Esdaile, D.J.; Fu, T.J.; Glatt, C.M.; Hadfield, N.; Hatzos, C.; et al. A multi-laboratory evaluation of a common in vitro pepsin digestion assay protocol used in assessing the safety of novel proteins. Regul. Toxicol. Pharmacol. 2004, 39, 87–98. [Google Scholar]
- Helenius, A.; Aebi, M. Roles of N-linked glycans in the endoplasmic reticulum. Annu. Rev. Biochem. 2004, 73, 1019–1049. [Google Scholar] [CrossRef]
- Huet, J.; Rucktooa, P.; Clantin, B.; Azarkan, M.; Looze, Y.; Villeret, V.; Wintjens, R. X-ray structure of papaya chitinase reveals the substrate binding mode of glycosyl hydrolase family 19 chitinases. Biochemistry 2008, 47, 8283–8291. [Google Scholar] [CrossRef]
- Ohnishi, T.; Juffer, A.H.; Tamoi, M.; Skriver, K.; Fukamizo, T. 26 kDa endochitinase from barley seeds: An interaction of the ionizable side chains essential for catalysis. J. Biochem. 2005, 138, 553–562. [Google Scholar] [CrossRef]
- Kezuka, Y.; Kojima, M.; Mizuno, R.; Suzuki, K.; Watanabe, T.; Nonaka, T. Structure of full-length class I chitinase from rice revealed by X-ray crystallography and small-angle X-ray scattering. Proteins 2010, 78, 2295–2305. [Google Scholar] [CrossRef]
- Neuhaus, J.-M. Plant chitinases (PR-3, PR-4, PR-8, PR-11). In Pathogenesis-Related Proteins in Plants; Datta, S.K., Muthukrishnan, S., Eds.; The CRC Press: Boca Raton, FL, USA, 1999; pp. 77–105. [Google Scholar]
- Neuhaus, J.-M.; Pietrzak, M.; Boller, T. Mutation analysis of the C-terminal vacuolar targeting peptide of tobacco chitinase: Low specificity of the sorting system, and gradual transition between intracellular retention and secretion into the extracellular space. Plant J. 1994, 5, 45–54. [Google Scholar]
- Di Sansebastiano, G.P.; Paris, N.; Marc-Martin, S.; Neuhaus, J.-M. Specific accumulation of GFP in a non-acidic vacuolar compartment via a C-terminal propeptide-mediated sorting pathway. Plant J. 1998, 15, 449–457. [Google Scholar] [CrossRef]
- Di Sansebastiano, G.; Rehman Reiaz, U.L.; Neuhaus, J.-M. Rat β-glucuronidase as a reporter protein for the analysis of the plant secretory pathway. Plant Biosyst. 2007, 141, 329–336. [Google Scholar] [CrossRef]
- Dombrowski, J.E.; Schroeder, M.R.; Bednarek, S.Y.; Raikhel, N.V. Determination of the functional elements within the vacuolar targeting signal of barley lectin. Plant Cell 1993, 5, 587–596. [Google Scholar] [CrossRef]
- Melchers, L.S.; Sela-Buurlage, M.B.; Vloemans, S.A.; Woloshuk, C.P.; van Roekel, J.S.C.; Pen, J.; van den Elzen, P.J.M.; Cornelissen, B.J.C. Extracellular targeting of the vacuolar tobacco proteins-AP24, chitinase and β-1,3-glucanase in transgenic plants. Plant Mol. Biol. 1993, 21, 583–593. [Google Scholar]
- Neuhaus, J.M.; Sticher, L.; Meins, F.; Boller, T. A short C-terminal sequence is necessary and sufficient for the targeting of chitinases to the plant vacuole. Proc. Natl. Acad. Sci. USA 1991, 88, 10362–10366. [Google Scholar] [CrossRef]
- Sticher, L.; Hinz, U.; Meyer, A.D.; Meins, F. Intracellular transport and processing of a tobacco vacuolar β-1,3-glucanase. Planta 1992, 188, 559–565. [Google Scholar]
- Saalbach, G.; Jung, R.; Kunze, G.; Saalbach, I.; Adler, K.; Müntz, K. Different legumin protein domains act as vacuolar targeting signals. Plant Cell 1991, 3, 695–708. [Google Scholar] [CrossRef]
- Higgins, T.J.V.; Chandler, P.M.; Randall, P.J.; Spencer, D.; Beach, L.R.; Blagrove, R.J.; Kortt, A.A.; Inglis, A.S. Gene structure, protein structure, and regulation of the synthesis of a sulfur-rich protein in pea seeds. J. Biol. Chem. 1986, 261, 11124–11130. [Google Scholar]
- Frigerio, L.; de Virgilio, M.; Prada, A.; Faoro, F.; Vitale, A. Sorting of phaseolin to the vacuole is saturable and requires a short C-terminal peptide. Plant Cell 1998, 10, 1031–1042. [Google Scholar] [CrossRef]
- Stigliano, E.; Faraco, M.; Neuhaus, J.-M.; Montefusco, A.; Dalessandro, G.; Piro, G.; di Sansebastiano, G.P. Two glycosylated vacuolar GFPs are new markers for ER-to-vacuole sorting. Plant Physiol. Biochem. 2013, 73, 337–343. [Google Scholar] [CrossRef]
- Di Sansebastiano, G.P.; Paris, N.; Marc-Martin, S.; Neuhaus, J.-M. Regeneration of a lytic central vacuole and of neutral peripheral vacuoles can be visualized by green fluorescent proteins targeted to either type of vacuoles. Plant Physiol. 2001, 126, 78–86. [Google Scholar] [CrossRef]
- Flückiger, R.; de Caroli, M.; Piro, G.; Dalessandro, G.; Neuhaus, J.-M.; di Sansebastiano, G.P. Vacuolar system distribution in Arabidopsis tissues, visualized using GFP fusion proteins. J. Exp. Bot. 2003, 54, 1577–1584. [Google Scholar] [CrossRef]
- Xiang, L.; Etxeberria, E.; van den Ende, W. Vacuolar protein sorting mechanisms in plants. FEBS J. 2013, 280, 979–993. [Google Scholar] [CrossRef]
- Marty, F. Plant vacuoles. Plant Cell 1999, 11, 587–600. [Google Scholar] [CrossRef]
- Di Sansebastiano, G.; Renna, L.; Gigante, M.; de Caroli, M.; Piro, G.; Dalessandro, G. Green fluorescent protein reveals variability in vacuoles of tree plant species. Biol. Plant. 2007, 51, 49–55. [Google Scholar] [CrossRef]
- Faraco, M.; di Sansebastiano, G.P.; Spelt, K.; Koes, R.E.; Quattrocchio, F.M. One protoplast is not the other! Plant Physiol 2011, 156, 474–478. [Google Scholar]
- Irani, N.G.; Grotewold, E. Light-induced morphological alteration in anthocyanin-accumulating vacuoles of maize cells. BMC Plant Biol. 2005, 5, 7. [Google Scholar] [CrossRef]
- Epimashko, S.; Meckel, T.; Fischer-Schliebs, E.; Lüttge, U.; Thiel, G. Two functionally different vacuoles for static and dynamic purposes in one plant mesophyll leaf cell. Plant J. 2004, 37, 294–300. [Google Scholar] [CrossRef]
- Pedrazzini, E.; Komarova, N.Y.; Rentsch, D.; Vitale, A. Traffic routes and signals for the tonoplast. Traffic 2013, 14, 622–628. [Google Scholar] [CrossRef]
- Robinson, D.G. Response to Rogers letter. Plant Physiol. 2008, 146, 1026. [Google Scholar] [CrossRef]
- Jolliffe, N.A.; Craddock, C.P.; Frigerio, L. Pathways for protein transport to seed storage vacuoles. Biochem. Soc. Trans. 2005, 33, 1016–1018. [Google Scholar] [CrossRef]
- Zouhar, J.; Rojo, E. Plant vacuoles: Where did they come from and where are they heading? Curr. Opin. Plant Biol. 2009, 12, 677–684. [Google Scholar] [CrossRef]
- Hatsugai, N.; Hara-Nishimura, I. Two vacuole-mediated defense strategies in plants. Plant Signal. Behav. 2010, 5, 1568–1570. [Google Scholar] [CrossRef]
- De Marchis, F.; Bellucci, M.; Pompa, A. Unconventional pathways of secretory plant proteins from the endoplasmic reticulum to the vacuole bypassing the Golgi complex. Plant Signal. Behav. 2013, 8, e25129. [Google Scholar] [CrossRef]
- Viotti, C.; Krüger, F.; Krebs, M.; Neubert, C.; Fink, F.; Lupanga, U.; Scheuring, D.; Boutté, Y.; Frescatada-Rosa, M.; Wolfenstetter, S.; et al. The endoplasmic reticulum is the main membrane source for biogenesis of the lytic vacuole in Arabidopsis. Plant Cell 2013, 25, 3434–3449. [Google Scholar] [CrossRef]
- Matile, P.; Moor, H. Vacuolation: Origin and development of the lysosomal apparatus in root-tip cells. Planta 1968, 80, 159–175. [Google Scholar] [CrossRef]
- Mesquita, J.F. Electron microscope study of the origin and development of the vacuoles in root-tip cells of Lupinusalbus L. J. Ultrastruct. Res. 1969, 26, 242–250. [Google Scholar] [CrossRef]
- Poustka, F.; Irani, N.G.; Feller, A.; Lu, Y.; Pourcel, L.; Frame, K.; Grotewold, E. A trafficking pathway for anthocyanins overlaps with the endoplasmic reticulum-to-vacuole protein-sorting route in Arabidopsis and contributes to the formation of vacuolar inclusions. Plant Physiol. 2007, 145, 1323–1335. [Google Scholar] [CrossRef]
- Robinson, D.G.; Jiang, L.; Schumacher, K. The endosomal system of plants: Charting new and familiar territories. Plant Physiol. 2008, 147, 1482–1492. [Google Scholar] [CrossRef]
- Geldner, N.; Anders, N.; Wolters, H.; Keicher, J.; Kornberger, W.; Muller, P.; Delbarre, A.; Ueda, T.; Nakano, A.; Jürgens, G. The Arabidopsis GNOM ARF–GEF mediates endosomal recycling, auxin transport, and auxin-dependent plant growth. Cell 2003, 112, 219–230. [Google Scholar] [CrossRef]
- Di Sansebastiano, G.P.; Fornaciari, S.; Barozzi, F.; Piro, G.; Arru, L. New insights on plant cell elongation: A role for acetylcholine. Int. J. Mol. Sci. 2014, 15, 4565–4582. [Google Scholar] [CrossRef]
- Zouhar, J.; Rojo, E.; Bassham, D.C. AtVPS45 is a positive regulator of the SYP41/SYP61/VTI12 SNARE complex involved in trafficking of vacuolar cargo. Plant Physiol. 2009, 149, 1668–1678. [Google Scholar] [CrossRef]
- Sanmartin, M.; Ordonez, A.; Sohn, E.J.; Robert, S.; Sanchez-Serrano, J.J.; Surpin, M.A.; Raikhel, N.V.; Rojo, E. Divergent functions of VTI12 and VTI11 in trafficking to storage and lytic vacuoles in Arabidopsis. Proc. Natl. Acad. Sci. USA 2007, 104, 3645–3650. [Google Scholar] [CrossRef]
- Viotti, C. ER and vacuoles: Never been closer. Front. Plant Sci. 2014, 5, 20. [Google Scholar] [CrossRef]
- Ebine, K.; Okatani, Y.; Uemura, T.; Goh, T.; Shoda, K.; Niihama, M.; Morita, M.T.; Spitzer, C.; Otegui, M.S.; Nakano, A.; et al. A SNARE complex unique to seed plants is required for protein storage vacuole biogenesis and seed development of Arabidopsis thaliana. Plant Cell 2008, 20, 3006–3021. [Google Scholar] [CrossRef]
- De Benedictis, M.; Bleve, G.; Faraco, M.; Stigliano, E.; Grieco, F.; Piro, G.; Dalessandro, G.; di Sansebastiano, G.P. AtSYP51/52 functions diverge in the post-Golgi traffic and differently affect vacuolar sorting. Mol. Plant 2013, 6, 916–930. [Google Scholar] [CrossRef]
- Faraco, M.; Latino, A.; de Benedictis, M.; Piro, G.; di Sansebastiano, G.P. Atsyp51 and Atsyp52 differently affect sorting of GFPChi and AleuGFP vacuolar markers. J. Plant Biochem. Physiol. 2013, 1, 2. [Google Scholar]
- Di Sansebastiano, G.P. Defining new SNARE functions: The i-SNARE. Front. Plant Sci. 2013, 4, 99. [Google Scholar] [CrossRef]
- Kang, B.H.; Nielsen, E.; Preuss, M.L.; Mastronarde, D.; Staehelin, L.A. Electron tomography of RabA4b-and PI-4Kβ1-labeled trans Golgi network compartments in Arabidopsis. Traffic 2011, 12, 313–329. [Google Scholar] [CrossRef]
- Cao, X.; Rogers, S.W.; Butler, J.; Beevers, L.; Rogers, J.C. Structural requirements for ligand binding by a probable plant vacuolar sorting receptor. Plant Cell 2000, 12, 493–506. [Google Scholar] [CrossRef]
- Ahmed, S.U.; Bar-Peled, M.; Raikhel, N.V. Cloning and subcellular location of an Arabidopsis receptor-like protein that shares common features with protein-sorting receptors of eukaryotic cells. Plant Physiol. 1997, 114, 325–336. [Google Scholar]
- Jiang, L.; Phillips, T.E.; Rogers, S.W.; Rogers, J.C. Biogenesis of the protein storage vacuole crystalloid. J. Cell Biol. 2000, 150, 755–770. [Google Scholar] [CrossRef]
- Park, M.; Kim, S.J.; Vitale, A.; Hwang, I. Identification of the protein storage vacuole and protein targeting to the vacuole in leaf cells of three plant species. Plant Physiol. 2004, 134, 625–639. [Google Scholar] [CrossRef]
- Park, M.; Lee, D.; Lee, G.J.; Hwang, I. AtRMR1 functions as a cargo receptor for protein trafficking to the protein storage vacuole. J. Cell Biol. 2005, 170, 757–767. [Google Scholar] [CrossRef]
- Shen, Y.; Wang, J.; Ding, Y.; Lo, S.W.; Gouzerh, G.; Neuhaus, J.-M.; Jiang, L. The rice RMR1 associates with a distinct prevacuolar compartment for the protein storage vacuole pathway. Mol. Plant 2011, 4, 854–868. [Google Scholar] [CrossRef]
- Wang, H.; Rogers, J.C.; Jian, L. Plant RMR proteins: Unique vacuolar sorting receptors that couple ligand sorting with membrane internalization. FEBS J. 2011, 278, 59–68. [Google Scholar] [CrossRef]
- Castelli, S.; Vitale, A. The phaseolin vacuolar sorting signal promotes transient, strong membrane association and aggregation of the bean storage protein in transgenic tobacco. J. Exp. Bot. 2005, 56, 1379–1387. [Google Scholar] [CrossRef]
- Stigliano, E.; University of Neuchâtel, Neuchâtel, Switzerland. Unpublished work, 2014.
- Scabone, C.M.; Frigerio, L.; Petruccelli, S. A fluorescent reporter protein containing AtRMR1 domains is targeted to the storage and central vacuoles in Arabidopsis thaliana and tobacco leaf cells. Plant Cell Rep. 2011, 30, 1823–1833. [Google Scholar]
- Hara-Hishimura, I.; Takeuchi, Y.; Inoue, K.; Nishimura, M. Vesicle transport and processing of the precursor to 2S albumin in pumpkin. Plant J. 1993, 4, 793–800. [Google Scholar]
- Batistic, O.; Kudla, J. Plant calcineurin B-like proteins and their interacting protein kinases. Biochim. Biophys. Acta 2009, 1793, 985–992. [Google Scholar] [CrossRef]
- Levanony, H.; Rubln, R.; Altschuler, Y.; Gallli, G. Evidente for a novel route of wheat storage proteins to vacuoles. J. Cell Biol. 1992, 119, 1117–1128. [Google Scholar] [CrossRef]
- Takahashi, H.; Saito, Y.; Kitagawa, T.; Morita, S.; Masumura, T.; Tanaka, K. A novel vesicle derived directly from endoplasmic reticulum is involved in the transport of vacuolar storage proteins in rice endosperm. Plant Cell Physiol. 2005, 46, 245–249. [Google Scholar] [CrossRef]
- Reyes, F.C.; Chung, T.; Holding, D.; Jung, R.; Vierstra, R.; Otegui, M.S. Delivery of prolamins to the protein storage vacuole in maize aleurone cells. Plant Cell 2011, 23, 769–784. [Google Scholar] [CrossRef]
- Rivera-Serrano, E.E.; Rodriguez-Welsh, M.F.; Hicks, G.R.; Rojas-Pierce, M. A small molecule inhibitor partitions two distinct pathways for trafficking of tonoplast intrinsic proteins in Arabidopsis. PLoS One 2012, 7, e44735. [Google Scholar]
© 2014 by the authors; licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution license (http://creativecommons.org/licenses/by/3.0/).