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. 2014 Mar 5;5:74. doi: 10.3389/fpls.2014.00074

Plasmodesmata without callose and calreticulin in higher plants – open channels for fast symplastic transport?

Kirill N Demchenko 1, Olga V Voitsekhovskaja 1, Katharina Pawlowski 2,*
PMCID: PMC3943419  PMID: 24634671

Abstract

Plasmodesmata (PD) represent membrane-lined channels that link adjacent plant cells across the cell wall. PD of higher plants contain a central tube of endoplasmic reticulum (ER) called desmotubule. Membrane and lumen proteins seem to be able to move through the desmotubule, but most transport processes through PD occur through the cytoplasmic annulus (Brunkard etal., 2013). Calreticulin (CRT), a highly conserved Ca2+-binding protein found in all multicellular eukaryotes, predominantly located in the ER, was shown to localize to PD, though not all PD accumulate CRT. In nitrogen-fixing actinorhizal root nodules of the Australian tree Casuarina glauca, the primary walls of infected cells containing the microsymbiont become lignified upon infection. TEM analysis of these nodules showed that during the differentiation of infected cells, PD connecting infected cells, and connecting infected and adjacent uninfected cells, were reduced in number as well as diameter (Schubert etal., 2013). In contrast with PD connecting young infected cells, and most PD connecting mature infected and adjacent uninfected cells, PD connecting mature infected cells did not accumulate CRT. Furthermore, as shown here, these PD were not associated with callose, and based on their diameter, they probably had lost their desmotubules. We speculate that either this is a slow path to PD degradation, or that the loss of callose accumulation and presumably also desmotubules leads to the PD becoming open channels and improves metabolite exchange between cells.

Keywords: cell-to-cell communication; plasmodesmata; desmotubule, calreticulin; callose; callose synthase; pollen

PLASMODESMATA OF HIGHER PLANTS CONTAIN DESMOTUBULES AND ARE USUALLY ASSOCIATED WITH CALRETICULIN

Plasmodesmata (PD) represent membrane-lined channels that link adjacent plant cells across the cell wall and provide symplasmic connectivity, allowing the transfer of metabolites, RNAs, proteins, viruses, and even plastids (Thyssen et al., 2012). PD of higher plants contain a central tube of endoplasmic reticulum (ER) called the central rod or desmotubule. The surfaces of the desmotubule and of the plasma membrane are covered with globular particles interlinked with spokes, thereby stabilizing the internal structure of the PD and also limiting their lumen. Cell-to-cell movement of ER membrane dyes and even – proteins seems to be possible through the desmotubule (Martens et al., 2006; Guenoune-Gelbart et al., 2008), and in spite of its appressed form, molecules of up to 10.4 kDa can move through the ER lumen between neighboring cells in some cases (Barton et al., 2011). However, most transport processes through PD occur through the cytoplasmic annulus, the region between plasma membrane and desmotubule. Early studies suggested a size exclusion limit (SEL) of PD in the order of 1 kDa (Robards and Lucas, 1990), but this can be increased to up to 67 kDa in response to changes in the cytosolic Ca2+ concentration or interaction with specific proteins (Oparka et al., 1999; Stadler et al., 2005; Lucas, 2006). PD structure is highly dynamic; e.g., PD morphology can change from simple to branched during the sink source transition in leaves, concomitant with a decrease in SEL (Oparka et al., 1999; Roberts et al., 2001).

PD are assumed to have evolved in multicellular algae several times independently, including in Characeae, the ancestors of higher plants (Raven, 2005). Interestingly, not all multicellular algae have PD (Raven, 2005). The structure of algal PD differs from that of higher plants, most dramatically by the absence of a desmotubule in algal PD (Cook et al., 1997; Cook and Graham, 1999). However, there are reports on desmotubules in PD of Chlorophyceae and Characeae (Uronema, Stigeoclonium, Chara; Marchant, 1976; Brecknock et al., 2011).

Calreticulin (CRT), a highly conserved Ca2+-binding protein found in all multicellular eukaryotes examined so far, is predominantly located in the ER (Michalak et al., 1999). CRT was also found in the Golgi (Borisjuk et al., 1998), and in animals also in the cytoplasm of certain cells (Dedhar, 1994), and at the cell surface (Johnson et al., 2001). CRT was shown to localize to PD in maize root apices (Baluška et al., 1999), as well as to PD in suspension cell cultures of tobacco and Arabidopsis (Laporte et al., 2003; Bayer et al., 2004), suggesting a role in cell-to-cell transport. This suggestion was supported by the finding that CRT interacts with a viral movement protein (Chen et al., 2005). However, root cap PD do not accumulate CRT (Baluška et al., 1999, 2000). Postmitotic cells of the root epidermis, which like root cap cells are symplasmically isolated, also do not accumulate CRT (Baluška et al., 1999, 2000, 2001), leading to the suggestion that CRT might represent a marker for sink strength. However, CRT is also formed in response to different stresses, and detailed observations led to hypothesis that it represents a universal mediator of fast plasmodesmal closure (Bilska and Sowiński, 2010). It is not quite clear whether CRT is localized in the ER – i.e., near the beginning of the desmotubule – or in the cell wall (Baluška et al., 1999; Bayer et al., 2004); yet, a comparison of the immunolocalization of CRT and callose favors a localization in the ER (Bayer et al., 2004).

CALLOSE PLAYS A ROLE IN REGULATING THE SEL OF PD

The transport through PD can be regulated by the deposition of callose, a β-1,3-glucan, between the plasma membrane and the wall in the neck region where the cytoplasmic annulus is constricted (Bucher et al., 2001; Simpson et al., 2009). Callose production is catalyzed by callose synthases in the cell wall and is induced by biotic as well as abiotic stresses (Scheible and Pauly, 2004; Benitez-Alfonso and Jackson, 2009). The identification of mutants affected in cell redox homeostasis as well as in intercellular transport, and the observation of changes in symplastic permeability of tissues in response to treatment with oxidants, have been interpreted to suggest that intercellular transport is regulated in response to the production of reactive oxygen species (ROS) via callose formation (Benitez-Alfonso and Jackson, 2009; Benitez-Alfonso et al., 2011).

INFECTED CELLS IN ROOT NODULES OF C. glauca REDUCE THEIR PD CONNECTIONS TO ADJACENT CELLS IN THE COURSE OF DEVELOPMENT, WHICH IS ASSOCIATED WITH THE LOSS OF CRT ASSOCIATION

Nitrogen-fixing root nodules, specifically their infected cells that harbor the nitrogen-fixing bacterial microsymbionts which rely on the plant for carbon supply, represent carbon sinks and nitrogen sources. Analysis of the mechanisms of phloem photosynthate partitioning in actinorhizal nodules of the Australian tree C. glauca revealed that here, plasmodesmal connections between infected cells, and to a lesser degree between infected and uninfected cells, were reduced during the differentiation of infected cells (Schubert et al., 2013). This concerned the number as well as the diameter of PD. The numbers of PD connecting infected cortical cells were reduced more strongly than the numbers connecting infected to adjacent uninfected cortical cells (by 84 vs. 60%, respectively) but the reduction in diameter was similar in both cases (by 55 vs. 49%, respectively). Furthermore, PD connecting mature infected cortical cells did not accumulate CRT (Schubert et al., 2013; Figures 1A,B). CRT labeling was only in rare cases observed for PD connecting infected and adjacent uninfected cells, but was common for PD connecting uninfected cells (Schubert et al., 2013; Figures 1C,D).

FIGURE 1.

FIGURE 1

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Immunolocalization of calreticulin (CRT) in longitudinal sections of C. glauca nodules embedded in Steedman’s wax (for the method, see Zdyb et al., 2011; for the antibody, see Baluška et al., 1999). Fluorescence micrographs (A,C) and differential interference contrast micrographs (B,D) are shown. The lignified walls of infected cells fluoresce in yellow under blue light. (A,B) No CRT labeling is found in walls (see arrow) between infected cells (ic). (C,D) CRT is labeled in walls connecting uninfected cells (uic) in a punctate pattern. Size bars denote 20 μm.

Under the assumption that CRT is localized in the ER at the opening of the PD, its absence might imply the absence of desmotubules. Desmotubule membranes are the closest juxtaposed lipid bilayers known in nature, 10–15 nm in diameter at their most constricted (Burch-Smith and Zambryski, 2012). Thus, in PD with a diameter of 22 or 26 nm, respectively, the absence of desmotubules should not be surprising, particularly in view of the fact that proteinaceous spokes should protrude from the desmotubule, and globular particles from the plasma membrane in the cytoplasmic sleeve (Burch-Smith and Zambryski, 2012). Loss of desmotubules has also been observed in nematode-parasitized root cortical cells from clover (Trifolium incarnatum) and tomato (Solanum esculentum), but here this phenomenon was associated with an increase in PD diameter (Hussey et al., 1992).

PD OF MATURE INFECTED CELLS OF C. glauca NODULES DO NOT SHOW CALLOSE ACCUMULATION

In order to obtain more information on the special features of the PD between infected cells, we analyzed the distribution of callose and of callose synthase. The gradual decrease of PD diameter during the differentiation of infected cortical cells of C. glauca nodules was associated with the loss of callose accumulation at PD connecting infected cells, or infected and adjacent uninfected cells, as detected by Aniline blue staining (Figure 2A). Aniline blue staining of callose was common for PD connecting uninfected cortical cells (Figure 2B). In an attempt to confirm the absence of callose at PD connecting infected cells, an antibody raised against callose synthase from Nicotiana alata pollen tubes (Cai et al., 2011) was used. The antibody labeled small granules in the plasma membranes of the youngest cells of the nodule lobe, close to the meristem (Figure 2C). Punctate labeling adjacent to the cell walls between uninfected cortical cells in the area of mature infected cells was also found (Figure 2D); however, no labeling was observed in walls of infected cells (Figure 2E). Since callose synthases are encoded by a gene family (Verma and Hong, 2001), no firm conclusions can be drawn regarding the potential presence of callose at PD connecting infected cells of C. glauca nodules; yet, the localization of callose and the immunolocalizations of callose synthase are consistent.

FIGURE 2.

FIGURE 2

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Anilin Blue staining of callose (A,B) in longitudinal vibratome sections of living C. glauca nodules embedded in agarose (Brundrett et al., 1988), and immunolocalization of callose synthase (C–E) in cross sections of fixed nodules embedded in Steedman’s wax (for the method, see Zdyb et al., 2011; for the antibody, see Cai et al., 2011). Micrographs were taken under fluorescent light. The lignified walls of infected cells show in white under UV light (A,B) and in yellow under blue light (C–E) . (A,B) Punctate Anilin Blue-staining of callose (white fluorescence) is found in the walls connecting uninfected cells (uic; white arrow), but no labeling is found in infected cells [recognizable by their fluorescent cell walls; labeling should be visible because the fluorescence of Anilin Blue, as obvious in (B) which shows a younger area of the cortex before the onset of infection, is more yellowish then the fluorescence of the walls of infected cells]. (C) Callose synthase is detected in the plasma membranes of uninfected cortical cells in the youngest part of the cortex, close to the apical meristem. In the older part of the cortex – (D) shows the outer cortex in the zone of nitrogen fixation – the labeling is less dense. (E) No labeling was seen in the plasma membranes of infected cells (ic; arrow). Size bars denote 20 μm in (A–D) and 25 μm in (E) .

MATURE INFECTED CELLS OF C. glauca ARE APOPLASTICALLY ISOLATED

Interestingly, C. glauca infected cells should depend on symplasmic supply with photosynthates since apoplastic transport pathways a blocked by the impregnation of the walls of infected cells with a very hydrophobic type of lignin (Berg and McDowell, 1988; Schubert et al., 2013). It has been suggested that the properties of the cell wall surrounding PD may restrict the degree to which the microchannels can dilate (Kragler et al., 1998). Therefore, this lignification, which commences upon infection by the microsymbiont, is the most likely explanation for the observed reduction of PD diameter in C. glauca infected cells. While many cases are known where lignification or suberization of cell walls does not affect the PD traversing these cell walls, in such cases the PD are organized in primary pit fields, i.e., areas with reduced thickness of the primary wall and without secondary cell wall deposition (Robinson-Beers and Evert, 1991) and with, it seems, a distinctive cell wall composition (Orfila and Knox, 2000), while in infected cells of C. glauca nodules, the primary walls are lignified, i.e., the PD traverse the lignified parts of the wall.

WHAT ARE THE EFFECTS OF THE CHANGES IN PD OF INFECTED CELLS IN C. glauca NODULES ON SYMPLASTIC TRANSPORT?

The diameters of PD connecting infected cells with adjacent infected or uninfected cells are significantly reduced compared to those connecting uninfected cells (Schubert et al., 2013). The lack of callose and callose synthase would mean the absence of negative regulation of the SEL of these PD by callose deposition. Similarly, no callose deposition was observed along cell walls between giant cells in nematode feeding sites of tobacco, but callose deposition was found frequently along cell walls toward neighboring cells (Hofmann et al., 2010).

The complete lack of CRT labeling at PD connecting infected cells, and the rarity of CRT labeling at PD connecting infected and adjacent uninfected cells, cannot be linked to the hypothesis that CRT represents a marker for sink strength (Baluška et al., 2001) since these cells, which express sucrose synthase at high levels, are strong sinks (Schubert et al., 2013). Furthermore, the infected cells are microaerobic (Berg and McDowell, 1987; Schubert et al., 2013) and usually, ATP depletion leads to the opening of PD (Cleland et al., 1994). However, the loss of CRT labeling is consistent with the hypothesis that CRT is a mediator of fast plasmodesmal closure. First, the PD closure mechanism involving CRT might not be able to function in PD traversing lignified primary cell walls. Second, since the infected cells are apoplastically isolated, additional symplastic isolation would mean cell death, and therefore should not be too easy to install.

It seems likely the changes in PD traversing the walls of infected cells are linked to the lignin deposition in the primary walls of infected cells. This can be interpreted in two ways. Either, the effect of lignification might be the gradual loss of function of PD, adding symplastic isolation to the apoplastic isolation of infected cells of C. glauca nodules. In that case, infection would eventually lead to cell death. Alternatively, the shrinking of the PD diameter could be compensated for by the loss of the desmotubules that might be implied by the loss of CRT labeling. Thanks to the central desmotubule, globular particles on the plasma membrane that lines the channel, and spoke-like connections between the desmotubule and the plasma membrane, the operational diameter of PD is no larger than 2 (Van Bel, 1993) or 3 nm (Kragler, 2013). Thus, the disappearance of the desmotubule could be expected to correlate with the disappearance of the spokes, increasing the operational diameter to one that is higher than of normal PD. Hence, the lack of desmotubules and callose would transform the PD to wide open channels for symplasmic transport. That would be consistent with the only known example for loss of PD desmotubules in plant cells, namely in nematode-parasitized root cortical cells from clover (T. incarnatum) and tomato (S. esculentum; Hussey et al., 1992).

PD OF INFECTED CELLS OF C. glauca NODULES – ON THE WAY TO COMPLETE CLOSURE, OR OPEN CHANNELS FOR OPTIMIZED SYMPLASTIC TRANSPORT?

In order to test which of these hypotheses is correct, a construct expressing green fluorescent protein (GFP) under control of a promoter specific to uninfected nodule cortical cells could be used. So far, no promoter driving expression specific to uninfected root cortical cells of C. glauca nodules has been characterized; however, Perrine-Walker et al. (2011) described an auxin efflux carrier (CgPIN1) that was present specifically in uninfected, not in infected nodule cortical cells. Hence, the promoter of CgPIN1 could be used to drive the expression of GFP in uninfected nodule cortical cells. With a molecular mass of 27 kDa and a Stokes radius of 1.8 nm, GFP can travel through the PD connecting root cortical cells (Stadler et al., 2005) and should also be able to pass through the PD connecting infected with adjacent uninfected cortical cells of C. glauca. A β-glucuronidase (GUS) fusion construct with the same promoter could serve as negative control, since with a molecular mass of 68 kDa and a Stokes radius of 3.3 nm (Fisher and Cash-Clark, 2000), GUS cannot travel through most PD (Fukuda et al., 2005). If cytological analysis shows the presence of GFP in infected cells of transgenic nodules, larger GFP constructs could be tested for a precise assessment of the SEL of the PD of infected cells.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

This work was supported by a grant from the Swedish research council VR to Katharina Pawlowski and grants from the Russian Foundation for Basic Research (11-04-02022-a, 12-04-32002, 13-04-40344, 13-04-02000), and the Focus Program of Presidium of the Russian Academy of Sciences, to Kirill N. Demchenko and Olga V. Voitsekhovskaja.

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