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Conceived and designed the experiments: AC KS LT DP MM PSL YS SW SP. Performed the experiments: AC KS LT WZ NT NF YS SP. Analyzed the data: AC KS LT WZ NT DP MM PSL YS MS SW SP. Wrote the paper: AC KS LT DP MM PSL YS MS SW SP.
Calreticulin (CRT) is a ubiquitous ER protein involved in multiple cellular processes in animals, such as protein folding and calcium homeostasis. Like in animals, plants have evolved divergent CRTs, but their physiological functions are less understood. Arabidopsis contains three CRT proteins, where the two CRTs AtCRT1a and CRT1b represent one subgroup, and AtCRT3 a divergent member.
Through expression of single Arabidopsis family members in CRT-deficient mouse fibroblasts we show that both subgroups have retained basic CRT functions, including ER Ca2+-holding potential and putative chaperone capabilities. However, other more general cellular defects due to the absence of CRT in the fibroblasts, such as cell adhesion deficiencies, were not fully restored. Furthermore, in planta expression, protein localization and mutant analyses revealed that the three Arabidopsis CRTs have acquired specialized functions. The AtCRT1a and CRT1b family members appear to be components of a general ER chaperone network. In contrast, and as recently shown, AtCRT3 is associated with immune responses, and is essential for responsiveness to the bacterial Pathogen-Associated Molecular Pattern (PAMP) elf18, derived from elongation factor (EF)-Tu. Whereas constitutively expressed AtCRT1a fully complemented Atcrt1b mutants, AtCRT3 did not.
We conclude that the physiological functions of the two CRT subgroups in Arabidopsis have diverged, resulting in a role for AtCRT3 in PAMP associated responses, and possibly more general chaperone functions for AtCRT1a and CRT1b.
The endoplasmic reticulum (ER) localized protein calreticulin (CRT) is an important component for protein folding and Ca2+ homeostasis in the ER of animal cells (for review see ). In addition, animal CRTs have been implicated in more than 40 other cellular functions, demonstrating the versatility of this protein .
More specifically, CRT-deficient mouse fibroblasts are impaired in ER Ca2+-storage, and in bradykinin (BK)-induced Ca2+-releases from the ER . These deficiencies are attributed to the two main functions of CRT, namely its Ca2+-buffering capacity in the ER, and its role in protein folding. The latter is presumably important for correct folding of the plasma membrane associated BK receptor . Consequently, mutations in CRT result in lower levels of the BK receptor, and therefore impairment in BK-induced Ca2+ releases from the ER. In addition, the crt−/− fibroblasts also exhibit defects in cell adhesiveness , which is linked to the decrease in ER Ca2+-storage in these cells. The ER Ca2+ is utilized to maintain cell adhesiveness by regulation of adhesion-specific proteins, such as fibronectin and vinculin, and by modulation of tyrosine phosphorylation cascades ; .
As compared to the functions of CRT in animal cells, the role of plant CRTs is less clear . Analogous to the animal protein, CRT may affect the ER Ca2+ homeostasis in tobacco cells in vitro , and in vivo . In addition, over-production of a maize CRT in tobacco cell suspensions improved growth of cells grown in high Ca2+-medium . Conversely, Arabidopsis plants over-expressing a maize CRT showed reduced leaf chlorosis when grown on Ca2+-depleted media compared to wild-type control plants . These data suggest that CRT has an important role in buffering and modulating ER Ca2+ also in higher plants. Recently a plant CRT, Arabidopsis thaliana (At)CRT1a, expressed in CRT-deficient mouse fibroblast was able to restore the Ca2+-holding capacity to levels comparable to control fibroblast . These results corroborate the results obtained in planta, and suggest a conservation of basic CRT functions between the two kingdoms.
CRT is also believed to harbor chaperone-like functions in plants (for review see . The best evidence for such a function is that CRT may form stress-induced, i.e. heat-shock-induced, protein complexes in tobacco leaves, suggesting that it may bind to unfolded proteins and therefore possibly function as a molecular chaperone . In addition,  showed that AtCRT1a restored putative folding deficiencies in CRT-deficient mouse fibroblasts.
The expression and localization of CRTs may vary depending on tissue and developmental stage. CRT appears to be present in most plant cells and tissues , but seems to be expressed abundantly in floral tissues , and in germinating seeds . In Arabidopsis flowers, CRT is mainly expressed in secreting nectaries, endosperm ovules early in development, and in the posterior of pollen sacs . CRT levels are also often elevated directly after fertilization and during early embryogenesis in a variety of plant species  to . CRT appears to mainly reside in the ER ; , and in the Golgi ; . Other studies have also localized CRT to the nuclear envelope in plant cells ; . Interestingly, CRT was preferentially localized to cell periphery-associated parts of ER, such as plasmodesmata, in maize roots . Similar localizations have also been reported in Nicotiana benthamiana .
Both plants and mammals appear to contain two subgroups of CRT proteins ; . For example, Arabidopsis holds three CRT family members that are classified into an AtCRT1a/1b, and an AtCRT3 group, on the basis of sequence homology . However, little is known about possible differences among the members of the plant CRT family regarding their functions, expression, and subcellular localization . One study demonstrated that AtCRT1a has retained basal CRT functions shared across different kingdoms as assessed by complementation of a CRT-deficient mouse fibroblast system . Atcrt1a mutant plants show lower tolerance to tunicamycin, an inhibitor of N-linked glycosylation that causes ER stress, referred to as the unfolded protein response (UPR; ). Another report suggests that mutations in different CRTs affect plant growth on Ca2+-deficient medium . In addition, several recent studies propose that AtCRT3 is necessary for the folding of the elf18 responsive EF-Tu receptor (EFR) associated with Pathogen-Associated Molecular Patterns (PAMPs) in plants ; . The same CRT (AtCRT3) was also recently shown to engage in the folding of a defective brassinosteroid receptor BRI-9 . The latter recognition was specific for AtCRT3, and not for the other two Arabidopsis CRT isoforms.
Through expression of AtCRT1a and CRT3 in CRT-deficient mouse fibroblasts we provide evidence that the two CRT sub-groups have retained certain, but not all, CRT functions. In planta analyses of the family members, including gene expression, protein localization and mutant analysis, revealed that the members of the two sub-groups have acquired specialized functions, and appear to act in different biological contexts.
Arabidopsis seedlings lacking AtCRT1a exhibit lessened seedling growth in response to tunicamycin treatment . One reason for this could be that other CRT family members are functionally redundant with AtCRT1a, i.e. in the absence of AtCRT1a the other CRTs may be sufficient to maintain CRT activity. In agreement with this, the two closely related CRT homologs AtCRT1a and CRT1b are co-expressed over approximately 2,000 publicly available microarray datasets (Figure S1A). Detailed semi-quantitative RT-PCR further revealed that AtCRT1a is expressed at moderate, or high levels in all major tissues investigated (Figure S1B). This is similar to what has previously been shown for AtCRT1b . The third CRT family member, AtCRT3, is also expressed in most of the investigated tissues, with an enhanced expression in senescing leaves (Figure S1B) To examine the expression in more detail we generated AtCRT1a, CRT1b and CRT3 promoter fusion constructs with the reporter gene β-glucuronidase (GUS), and introduced these into Arabidopsis plants. Three independent lines tested of both the AtCRT1a and CRT1b promoter constructs displayed almost identical expression patterns throughout different tissue- and cell types (Figure 1), consistent with the transcriptional coordination described above (Figure S1A). For example, these lines exhibited high GUS activity in the root tip, and expanding root cells, and were also active in rosette leaves, floral tissues including pollen, and in expanding cotyledons (Figure 1). The AtCRT3 expression was similarly confined to expanding cells, and rosette leaves, but was absent from the root tip, and from mature pollen (Figures 1C and F). Interestingly, two-day-old seedlings were stained heavily for AtCRT1a and CRT1b promoter activity, but GUS activity in the AtCRT3 reporter lines was virtually absent from such seedlings (Compare Figures 1G to I). In addition, whereas AtCRT3 showed GUS activity in senescing leaves, that of AtCRT1a and CRT1b (not shown) was much reduced (compare Figures 1P and Q).
To determine whether the different CRT promoters may be activated by external cues we grew three independent AtCRT1a, CRT1b, and CRT3 GUS lines on plates for three days in light. We then transferred the seedlings to microscope slides that were coated with MS medium, and grew them for two additional days. The slides were subsequently transferred to containers for exposure to different inductive treatments. We incubated the seedlings for three, 12 and 24 h in 150 mM glucose, 150 mM sucrose, 150 mM mannitol, 10 µg/ml tunicamycin, 10 mM DTT, or 250 µM salicylic acid. We chose these treatments based on publicly available microarray datasets, and on the chaperone related functions of CRTs . Both the AtCRT1a and CRT1b promoters showed strong signals at 12, and 24 h after tunicamycin treatment (Figure 2A). In contrast, the activity of the AtCRT3 promoter was not noticeably increased in response to the same treatment (Figure 2A). These data are in agreement with previous data obtained from northern blotting , or from microarray analyses . We did not observe any major changes in the activation or repression of the CRT promoters in response to any of the other stresses (data not shown). The strong activation of the AtCRT1a and CRT1b promoters in response to tunicamycin is indicative of an association to tunicamycin-induced ER stress, or the UPR ; . In animal cells, tunicamycin-mediated inhibition of N-linked glycosylation in the ER leads to the up-regulation of a battery of ER chaperones, including calnexins (CNXs), BiPs, and protein disulfide isomerases (PDIs; ). In agreement with this, AtCRT1a and CRT1b are closely co-expressed with other typical ER chaperone genes, including CNXs, PDIs and BiPs (Figure 2B; ), indicating that these CRTs may act as part of an ER chaperone network in Arabidopsis.
To assess the distribution of the CRT proteins at the tissue- and cellular level we generated specific antibodies for the different family members. We used as antigens peptides derived from their C-terminal regions, which are flexible in structure and variable in sequence between family members. We verified the specificity of the antibodies in western blot analyses (Figures 3A). An antibody raised against a full-length maize CRT recognizes three distinct bands in typical microsomal fractions from either cell suspensions (not shown), or Arabidopsis leaves (Figure 3A; ). The size differences might reflect differential N-glycosylation states between the different CRTs, i.e. the AtCRT1a is predicted to have three potential N-linked glycosylation sites whereas AtCRT1b and CRT3 only contains one predicted N-linked glycosylation site each (Figure 3B; ). Consistent with this, the AtCRT1a antibody recognized a band that is of similar apparent molecular weight to the upper CRT band recognized by the maize antibody, and which has previously been shown to be absent in Atcrt1a mutant plants . The AtCRT1b and CRT3 antibodies did, on the other hand, recognize bands with lower apparent molecular weights (Figure 3A). The different bands recognized by the peptide antibodies all correspond well with CRT bands recognized by the maize CRT antibody (Figure 3A).
After affinity purification we used the different CRT peptide antibodies to probe sections of Arabidopsis roots to reveal the distribution of the individual CRTs in different cell types. All the CRT family members appeared to be abundantly expressed in roots (Figure 1). The AtCRT1a antibody revealed an even distribution of this protein in most cells throughout the early elongation zone in young roots, and a high level accumulation in the root cap (Figure 3C). In equivalent sections incubated with the AtCRT1b antibody, fluorescence predominantly appeared in the outermost root cap (Figure 3D). In addition, AtCRT1b, but not CRT1a, labeling was evident in epidermal cells, both in trichoblasts and atrichoblasts, and in developing xylem cells, in sections corresponding to the late elongation zone (Figures 3G and H). These results are in agreement with GUS activity in promoter::reporter lines for the two genes, which showed strong GUS activity in the early elongation cells for AtCRT1a, and a slightly later onset for AtCRT1b, which was also active in the vascular tissues (Figures 3K and L). Furthermore, several of the trichoblasts and atrichoblasts showed immuno-fluorescence signals that appeared dotted (data not shown), possibly indicating ER-localization. We did not observe any immuno-fluorescence signal when probing with AtCRT3 antibodies, indicating that the protein accumulates at low levels, or that the epitope is masked in situ. No signals were obtained when probed with the respective pre-immune sera (Figures 3E, F, I and J), nor in Atcrt1a and crt1b mutants probed with AtCRT1a and CRT1b antibodies, respectively (data not shown).
The immuno-fluorescence data suggest that the two CRTs, AtCRT1a and CRT1b, accumulate in partially overlapping but distinct cell types. To determine whether there are also differences in the subcellular distribution we utilized immuno-cytochemical techniques together with transmission electron microscopy (TEM). The AtCRT1b antibody recognized epitopes that appeared associated with the ER, e.g. ribosome enriched segments, in Arabidopsis root sections from the early elongation zone (Figure 4A). No labeling was observed in an Atcrt1b mutant under the same conditions (data not shown). In addition, we also found AtCRT1b epitopes in structures resembling plasmodesmata (Figure 4B). To confirm the plasmodesmata localization we co-incubated the sections with the AtCRT1b antibody raised in rabbits, and a callose (β-1, 3–glucan) antibody raised in mice. Consistent with localization of AtCRT1b to the plasmodesmata the callose antibody labeled regions in close vicinity to the AtCRT1b labeling (Figure 4B). Similarly, we observed AtCRT1a associated with the plasmodesmata (Figure 4C), and also with intracellular compartments reminiscent of the ER (data not shown). However, labeling by the AtCRT1a antibodies appeared less dense than by the AtCRT1b antibody, possibly because the binding epitope was obscured, or perhaps due to lower levels of AtCRT1a in the analyzed cells.
Many attempts were made to visualize the AtCRT3 by immuno-gold labeling but, analogous to the immuno-labeling attempts, we were unable to obtain any signals above the pre-immune serum control. Since contrasting localization data has been presented for AtCRT3, i.e. ER (27) and cytoplasm or nucleus (25), we argued that it would be important to consolidate the subcellular location of the protein. We therefore generated an AtCRT3 fusion with the fluorescent marker CFP (cyano fluorescent protein) under the control of a 35S promoter. We inserted the CFP seven amino acids upstream of the C terminus to minimize a possible influence on the activity of its putative ER-retention signal (HDEL). We subsequently transiently transformed the construct into tobacco leaves, and visualized the CFP signal under a confocal microscope (Figure 4D). The CFP signal displayed a reticular network, reminiscent of the ER. In addition, the signal also clearly outlined the nucleus, possibly representing the nuclear envelope (Figure 4D). These data are consistent with the predicted sub-cellular localization of CRTs, i.e. in the ER , and with the fact that AtCRT3 holds an ER retention signal in its far C terminus.
We have previously shown that AtCRT1a restores CRT deficiencies in mouse fibroblasts . To test whether also AtCRT3 can complement the CRT-deficient mouse cells we expressed the AtCRT3 fused to a HA-tag in these cells. Five stable transgenic cell lines were established, and expression was confirmed using immuno-blotting with a HA-tag antibody (Figure 5A). A single band at 60 kDa was detected in all AtCRT3 lines, while no bands were present in the CRT-deficient control lines. To confirm that the recombinant AtCRT3 was located to the ER, immuno-labeling using the HA-tag antibody was performed (Figure 5B, red color). All AtCRT3 transgenic cell lines showed ER-localization, which was confirmed by co-localization with an antibody against the ER marker PDI (Figures. 5C and E). These data support the ER localization of the CFP-tagged CRT3 in tobacco leaves (Figure 4D).
Most animal CRTs do not hold N-linked glycans (Frickel and Ellgaard, 2003). To test whether plant CRTs, i.e. the AtCRT3 and CRT1a , undergo N-linked glycosylation when expressed in the mouse cells we treated lysates derived from mouse cells, expressing either AtCRT1a or CRT3, with the glycosidase PNGase F that removes N-linked glycans (Figure S2A). The glycosidase treatment of cell lysates decreased the apparent molecular weights of the plant CRTs on immunoblots (Figure S2A), suggesting that the AtCRT1a and CRT3 may acquire N-linked glycans when expressed in the mouse cells.
AtCRT3 contains a smaller number of negatively charged amino acids in its C terminus compared to AtCRT1a and CRT1b, and most animal CRTs, indicating a lower Ca2+-holding ability of the protein . Notably, most amino acids that are important for chaperone functions in animal CRTs are conserved in AtCRT1a and CRT1b, but not in AtCRT3 (Figure 5F; ). For example, the amino acids corresponding to Asp258 and Glu260 in animal CRT (numbers referred to human CRT1) that are necessary for chaperone activities and ERp57 interactions  have been changed to Asn268 and Leu270 in AtCRT3 (Figure 5F). Similar changes are also seen in CRT3 orthologs in maize and rice (data not shown). To assess whether these changes may distinguish AtCRT3 functions from that of typical CRTs, we measured the ER Ca2+-holding potential and the responsiveness to BK of the AtCRT3 complemented crt−/− mouse fibroblasts. These fibroblasts were cultured in the presence of 45Ca2+ for 50 h, as described in . Addition of the ER Ca2+-ATPase blocker thapsigargin caused a significant increase (approximately 1.5-fold) in Ca2+-release in AtCRT3 expressing cells compared with the CRT-deficient control cells (Figure 5G).
We further measured the BK-induced Ca2+-release in the AtCRT3-transfected fibroblasts, via the fluorescent Ca2+ indicator Fura2 . The basal Ca2+ level in the cytosol before addition of BK was estimated to be ~100 nM for all cell lines (Figure 5H). Addition of BK to the cells resulted in a rapid release of Ca2+ in all lines tested (Figure 5H). However, the release from the mouse control, and AtCRT3 expressing cells were approximately 1.5- to 2-fold higher as compared to that from the CRT-deficient control cells (Figure 5H). In addition, the amounts of Ca2+ release in the mouse wild-type, and AtCRT3 expressing lines were similar, indicating that AtCRT3 restored the CRT deficiencies in the crt−/− fibroblasts (Figure 5I). These data are similar to data obtained from AtCRT1a expressing crt−/− fibroblasts , and show that AtCRT3 holds basic CRT functions.
In spite of the alteration of the amino acids Asp258 and Glu260 conserved in animal CRTs to Asn268 and Leu270 in AtCRT3, AtCRT3 restored the ER Ca2+-holding, and BK-induced release of Ca2+ in the CRT-deficient mouse cells. To assure that this is the case we introduced these amino acids, essential for ERp57 interaction (Asp and Glu), to the positions of Asn268 and Leu270 in AtCRT3, respectively, and then generated five transgenic mouse cells expressing this AtCRT3 variant, referred to as AtCRT3m. We verified that the expression and localization of AtCRT3m was similar to that of AtCRT3 (Figures S2B to F). The thapsigargin-sensitive ER Ca2+ content in the crt−/− mouse fibroblasts expressing AtCRT3m was very similar to the thapsigargin sensitive ER Ca2+ storage capacity of the AtCRT3 expressing cells (Figure 5G). Similarly, no significant differences between the AtCRT3 and CRT3m were detected when we assessed the BK-induced Ca2+ releases (Figures 5H, I, and S3). These data suggest that the introduction of the Asp258 and Glu260 conserved in most CRTs, at corresponding sites to Asn268 and Leu270 in AtCRT3 do not affect localization of the protein, the ability to retain Ca2+ in the ER, nor the capability to sustain BK-induced Ca2+-release from the ER in the mouse fibroblast system.
In addition to compromised ER Ca2+ levels and BK-induced Ca2+ releases, the crt−/− fibroblasts also exhibit a lower degree of cell-substratum adhesion . To test whether expression of AtCRT1a or CRT3 in the crt−/− mouse fibroblasts have regained their adhesive potency we determined the cell shape, which is conventionally examined to assess cell spreading, and therefore the level of cell adhesion . Figures 6A and B clearly show that wild-type cells, which contain CRT, readily adhered to the surface. In contrast, the CRT-deficient cells did not (Figures 6A and C). Interestingly, the AtCRT1a and CRT3 expressing cell lines that restored the ER Ca2+ content, and the BK-induced Ca2+ release from the ER only partially restored the cell adhesiveness (Figures 6A, D and E). Approximately, 50% of the AtCRT1a and CRT3 expressing cells showed cell spreading, whereas wild-type cells typically had above 75% cell spreading (Figure 6A). Thus the level of cell adhesion is not fully restored by the plant CRTs. This suggests that restoration of the ER Ca2+ content alone is not sufficient to fully restore cell adhesion activity.
We previously described wild-type like growth in Atcrt1a mutant plants under normal growth conditions . However, Atcrt1a mutants exhibited an increased sensitivity to the UPR-inducing agent tunicamycin. This relatively weak phenotype, i.e. lessened seedling growth, in response to tunicamycin may be due to functional compensation by AtCRT1b that is present in the mutant. To test this, we isolated two independent Atcrt1b mutant lines that appear to be null mutants for the encoded protein as assessed by western blotting (Figures 7A and B). The western analysis also revealed that the AtCRT1b band migrated to an apparent lower molecular weight (Figure 7B), consistent with the notion that AtCRT1b may hold lower levels of glycans compared to AtCRT1a.
Under normal growth conditions mature Atcrt1b mutant plants did not display any significant phenotypes compared to wild-type control plants. However, both light-grown and etiolated seedlings were significantly smaller compared to wild-type seedlings (Figures 7C to G). Interestingly, Atcrt1b seedlings exhibited a relatively lower sensitivity to tunicamycin compared to wild-type control seedlings (Figures 7C and E). These data may suggest that loss of AtCRT1b constitutively triggers a stress similar to UPR in the seedlings, or that the perception of this type of stress is altered in the mutant seedlings.
To assess whether the relatively mild phenotypes for Atcrt1a and crt1b are due to functional redundancy between the two homologs we generated Atcrt1a crt1b double mutants. The absence of both proteins was confirmed in western blot analyses (Figure 7B). Although we did not observe any obvious phenotypes in mature plants, the double mutant seedlings were significantly smaller compared to the wild-type line (Figures 7C and D), and to the Atcrt1a mutant parent line (Figure 7C). However, there was no major size difference between the Atcrt1b mutant and the Atcrt1a crt1b double mutant seedlings grown in light (Figure 7C). These data suggest a predominant role of AtCRT1b over AtCRT1a in light-grown seedlings. However, when grown in the dark the Atcrt1a crt1b double mutant did exhibit an additive phenotype compared to the Atcrt1a and crt1b single mutant parent lines (Figures 7F and G), suggesting that both AtCRT1a and CRT1b contribute to etiolated seedling growth. The Atcrt1a crt1b seedlings displayed lower sensitivity to tunicamycin-dependent growth retardation as compared to wild-type seedlings (Figures 7C to E) indicating that they either are under constitutive ER stress, or that the perception of such stress is different in the mutants. Consistent with this hypothesis both the Atcrt1b and the Atcrt1a crt1b mutants were two- to four-fold less sensitive to tunicamycin compared to wild-type control seedlings (data not shown), corroborating that the mutants may be primed for ER stress prior to the tunicamycin treatment.
One explanation for the lower tunicamycin sensitivity in the mutant seedlings could be that they constitutively produce higher levels of different ER chaperones in the absence of AtCRT1b. However, in the case of the Atcrt1b single mutants, it is likely that an increased production of, for example, the tunicamycin-sensitive AtCRT1a would mask any growth phenotype. Indeed, this scenario is corroborated by the fact that AtCRT1a complemented the Atcrt1b growth phenotypes when over-expressed (Figure 8; see below). To assess whether the expression of ER chaperones is constitutively active in the mutants we performed real-time PCR analysis on a range of such genes, which have been shown to be induced by tunicamycin . Figure S4 shows no significant differences in the basal expression levels of these chaperone-related genes in the mutants as compared to wild-type control seedlings. Although it cannot be ruled out that these putative chaperones are altered at the protein level, it is plausible that the perception of, or response to, tunicamycin is altered in Atcrt1b and Atcrt1a crt1b.
To test whether the different Arabidopsis CRTs could restore the growth defects in the Atcrt1b single, and Atcrt1a crt1b double mutants we introduced two constructs with either an AtCRT1a cDNA or an AtCRT3 cDNA driven by a constitutive 35S promoter into the two mutant lines. To confirm the expression of AtCRT1a and CRT3 we performed semi-quantitative RT-PCR, and western blotting, respectively (Figures 8A, B, E, F and S3B). Several independent AtCRT1a-transformed Atcrt1b mutant lines displayed an increase in AtCRT1a mRNA production and AtCRT1a protein accumulation (Figures 8E and F). Similarly, mutant lines transformed with AtCRT3 displayed increased levels of AtCRT3 protein (Figures 8B and S3B). These data show that the transformed mutant lines produce higher levels of AtCRT1a and CRT3 compared to the untransformed mutant lines, respectively. AtCRT1a restored the growth to wild-type levels of the Atcrt1b mutant (Figures 8C and G), indicating that the AtCRT1a and CRT1b proteins are functionally redundant at least during seedling growth. In contrast, AtCRT3 did not complement the Atcrt1b, nor the Atcrt1a crt1b double mutant phenotypes (Figures 8C and D). These differences were significant (t-tests t9=5.74, P=1.3×10−5 for Atcrt1b compared to Atcrt1b AtCRT3), suggesting a divergent role of AtCRT3 from AtCRT1a and CRT1b.
To assess whether mutations in the AtCRT3 gene affect any aspects of plant growth we screened T-DNA lines for homozygous inserts in the gene (SALK_051336). AtCRT3 protein was undetectable in homozygous mutant plants, confirming that the T-DNA insertion disrupted the expression of the gene (Figures 9A and B). No obvious growth phenotypes were evident in the mutant compared to wild-type under normal growth conditions, nor upon tunicamycin treatment. These data suggest a minor role of AtCRT3 under UPR conditions, which is consistent with undetectable AtCRT3 activation upon tunicamycin application (Figure 2A). In addition, AtCRT3 is not part of the closely co-expressed ER chaperone network that contains AtCRT1a and CRT1b. However, we noticed that AtCRT3 is instead transcriptionally coordinated with several genes that are responsive to biotic and abiotic stresses (Figure 10). For example, two of the MAP kinase kinases (MAPKK), MKK1 and MKK2, are closely co-expressed with AtCRT3 (Figure 10). Both MKK1 and MKK2 appear to be part of a phosphorylation cascade that is triggered by PAMPs, such as elf18, and flg22 (For review see ). Consistent with this ;  recently showed AtCRT3 is necessary for elf18 perception and responses. To test whether AtCRT1a and CRT1b also participate in the responsiveness to PAMPs, we tested possible alterations in PAMP responses in the absence of these CRTs. First we grew the single-, and double mutant lines on medium containing 100 mM sucrose in the absence, or presence of elf18 or flg22 (Figure 9C). These peptides suppress anthocyanin accumulation in wild-type seedlings that are exposed to high levels of sucrose (Figure 9C). However, while no elf18-induced anthocyanin suppression was observed in Atcrt3 seedlings (Figure 9C; ; ), both the Atcrt1a and crt1b single, and the Atcrt1a crt1b double mutants showed wild-type-like suppression of anthocyanin accumulation in the presence of elf18 (Figure 9C). These results are in agreement with the recent report from Li et al. . The de-repression of anthocyanin accumulation in the Atcrt3 mutants in the presence of elf18 has been attributed to the defects in the biogenesis, and stable accumulation, of the receptor-like kinase EFR that acts as the elf18 receptor (Figure 9D; ; ). Consistent with these data, we detected no significant alteration in the steady-state levels of EFR in the Atcrt1a crt1b double mutants compared to wild-type (Figure 9F, upper panel; Figure S3C).
The perception of PAMPs induces a transient generation of reactive oxygen species (ROS) at the outer-surface of the plasma membrane . While this response is readily triggered in the Atcrt3 mutant by flg22, elf18 failed to induce ROS in this mutant (Figures 9D and E; ; ). Interestingly, the ROS generation was also partially impaired in the Atcrt1a crt1b double mutants, albeit not to the same extent as in the Atcrt3 mutants, similar to what has recently been reported in  (Figure 9D). These data either indicate that EF receptor outputs are not fully retained in the Atcrt1a crt1b double mutant, or that the production of ROS is impaired in this mutant.
The multi-functional protein CRT has been widely studied in animals where the protein is associated with more than 40 cellular functions . Studies on CRTs in plants are less advanced, in particular in that specific roles of the individual CRT family members present in plants have, until recently, been largely unaddressed. We show that while the three different CRT family members in Arabidopsis have retained basic CRT functions, they have attained diverged functions in planta.
Both AtCRT1a and CRT3 restored the ER Ca2+ levels, and putative chaperone deficiencies in the crt−/− mouse fibroblasts. Such complementation was somewhat unexpected for AtCRT3 given significant divergence in its protein sequence that may be predicted to hamper characteristic CRT activities. For example, the protein only holds negatively charged amino acid residues in 28 of the 110 residues of the C-domain. In comparison, AtCRT1a holds 44 negatively charged amino acids in the equivalent region. These negatively charged amino acids are believed to constitute the main Ca2+-binding mechanism of the CRTs . AtCRT1a does, similar to AtCRT3, also complement the CRT deficiencies in the mouse fibroblast system. More detailed analyses are necessary to distinguish any differences that are attributable to the different numbers of negatively charged amino acids between the two CRT isoforms. Interestingly,  recently showed that the C-terminal part of AtCRT3 is crucial for the protein to retain the defective BRI1-9 in the ER. These data further support an important role for the C-domain of the CRTs for the divergent functions.
Surprisingly, while the ER Ca2+ homeostasis and the putative chaperone functions were restored in the CRT-deficient mouse fibroblasts by expression of either AtCRT1a or CRT3, other phenotypes were only partially complemented. For example, the reduced cell adhesiveness associated with the CRT-deficient fibroblasts could not be fully rescued by either AtCRT1a or CRT3 (Figure 6). However, it is important to point out that the relative expression level of the AtCRT1a and CRT3 also may influence the adhesive ability in the mouse fibroblast. While this may be the case, it is clear that the Ca2+ levels were restored to control levels in the AtCRT1a and CRT3 expressing lines, and it is therefore unlikely that the defects in adhesion of these cells are due to a decrease in the ER Ca2+ content in the transfected crt−/− fibroblasts. Rather, our results suggest other CRT characteristics that are not conserved in the plant CRTs. The adhesion between the cells and substrate depends on several proteins connecting the cell surface to the cytoskeleton, such as fibronectin and vinculin, and also on tyrosine phosphorylation cascades ; . It is possible that AtCRT1a and CRT3 are unable to properly fold some of these components, and thus fail to restore cell adhesion activity. It is also plausible that AtCRT1a and CRT3 are unable to efficiently fold different Ca2+-releasing components in the ER, or that AtCRT1a and CRT3 fail to interact with these components that may require a direct interaction with CRT to facilitate Ca2+-signaling. Such impairments could of course also impair Ca2+-releases and therefore cell adhesion . In any case, the inability of the AtCRT1a and CRT3 to fully restore the cell adhesion phenotype in the CRT-deficient cells suggets that while some functions are conserved between the CRTs in the two kingdoms there may also be diverged characteristics that are specific to plant and animal CRTs.
Analyses of publicly available expression data, and our promoter:GUS experiments, suggest that expression of AtCRT1a and CRT1b is active in the same tissue- and cell types (Figure 1). However, immuno-fluorescence data using peptide specific antibodies clearly show that the similarity in expression only partly is mirrored on the protein level (compare Figures 1 and and3).3). These results suggest that while the two CRTs may be active in different cell types, certain cells may need additional CRT activity perhaps for increased protein production, or for an increased need for ER Ca2+ holding potential. The potential functional overlap between these CRTs was corroborated by the complementation of AtCRT1b mutants by AtCRT1a. AtCRT1a and CRT1b are also co-expressed with several other ER chaperones, including CNXs, BiPs and PDIs, and are induced by tunicamycin, a trigger of UPR in the ER . Several reports show that genes that are transcriptionally coordinated tend to be functionally related (for example ; ). It is therefore tempting to speculate that the AtCRT1a and CRT1b are part of a larger network of ER chaperones, which could provide a basal folding apparatus of newly synthesized proteins in the ER.
Although our data suggest a role for AtCRT1a and CRT1b in the UPR (; Figure 7), we did not see any indications for a similar function for AtCRT3. Instead, the Atcrt3 mutant plants displayed defects in elf18 responses, which were not observed to the same extent in the Atcrt1a crt1b double mutant plants (Figure 9, ; ). These results are in agreement with two recent reports ; , which showed failure of Atcrt3 mutants to repress anthocyanin accumulation in response to elf18. Interestingly, genes encoding MKK1 and MKK2 that mediate PAMP responses  are closely co-expressed with AtCRT3 (Figure 10). In addition, several other immune response-related genes are also co-expressed with AtCRT3. These include two genes encoding CC-NBS-LRR homologs. Several family members of this class of proteins act as resistance (R) proteins and confer isolate-specific immunity . Another co-expressed gene is RIN4, a gene required for immune-responses to phytopathogenic Pseudomonas syringae conditioned by the R proteins RPS2 and RPM1 (Figure 10; ). These data are suggestive of a role for AtCRT3 in immune responses.
Both EFR and Flagellin-sensing 2 (FLS2) contain multiple putative N-glycosylation sites in their LRR domains . This domain is predicted to be exposed to the ER lumen during protein folding, and maturation. It is therefore tempting to speculate that AtCRT3 recognizes the N-linked glycans attached to the unfolded EFR, thereby becoming engaged in the folding of the receptor. A similar recognition does not seem to occur for the FLS2 (Figure 9), or if it does, the ER holds other agents that are sufficient to facilitate correct folding of the FLS2 in the absence of ACRT3. Since AtCRT1a and CRT1b do not seem to be predominantly involved in the folding of the EFR (Figures 9; ), it is apparent that the different subgroups of CRTs have developed substrate specificity. This notion was further corroborated by the inability of AtCRT3 to complement the Atcrt1b, and the Atcrt1a crt1b plants even when over-expressed (Figure 8). In contrast, over-expression of AtCRT1a complemented Atcrt1b plants. Given that both the AtCRT1a and CRT3 restored the ER Ca2+ levels in the CRT-deficient mouse fibroblasts (Figure 5; ), we assume that the Ca2+ storage activity is similar between these two types of plant CRTs. We therefore propose that AtCRT1a and CRT3 mainly differ in their chaperone functions. While the main chaperone-related functions typically are associated with the N-, and P-domain of CRTs , a recent study showed that the C-terminal part of AtCRT3 is essential for retention of the defective BRI1-9 . This raises the interesting point that chaperone, or at least chaperone-related retention, mechanisms may also be present in the C-domain of the CRTs.
Thus, in agreement with several recent reports  to  our data suggest a significantly diverged role of AtCRT3 from that of AtCRT1a and CRT1b, as demonstrated by the observed strict requirement of the former for the biogenesis of EFR. However, our data also suggest a minor role of AtCRT1a and CRT1b for the establishment of full EFR functions (Figure 9; ), implying functional interactions between these two types of CRTs in plants. Further experimentation is needed to elucidate the mechanistic basis for diversified yet mutually supporting functions of CRTs in plants.
Arabidopsis seeds with T-DNA insertion in AtCRT1a, CRT1b and CRT3 were obtained from the Arabidopsis Biological Resource Center (ABRC; http://arabidopsis.org; ). The lines used were SALK_055452 (Atcrt1a) , SALK_062083 (Atcrt1b-1), SAIL_ 662_DO5 (Atcrt1b-2), SALK_051336 (Atcrt3). PCR was performed, with primer sequences generated against the genomic regions flanking the insert and a standard primer for the 3′ end of the insertion sequence, to obtain homozygous insertion lines (Table S1). Reciprocal crosses were undertaken to generate the Atcrt1a crt1b double mutant (SALK_055452 with SALK_062083). RT-PCR and western blotting, as described below, was used to ensure that the transcript in the insertion lines was not present (Table S1).
Hypocotyl length was first crudely measured using a 0.5 mm marks, and subsequently confirmed using the software Leica Application Suite (Version 2.8.1, Leica Microsystems CMS, GmBH, Switzerland) with seedlings photographed using a Leica stereomicroscope (Leica MZ 12.5) equipped with a Leica DFC420 digital camera.
Amino acid sequences of AtCRT1a, CRT1b and CRT3 and human CRT1 and CRT2 (GenBank accession no. AAC49695, AAK74014, AAC49697, AAA51916, NP_659483, respectively) were obtained from National Center for Biotechnology Information (NCBI; www.ncbi.nlm.nih.gov). Alignment was done using ClustalW, MacVector 8.0 software (Oxford Molecular group plc, UK).
Microarray datasets were obtained from NASCarrays (http://affymetrix.arabidopsis.info/narrays/experimentbrowse.pl), and were downloaded and plotted in excel. Signals with values below 100 were excluded from the analysis.
RNA was isolated from Arabidopsis tissues with Qiagen RNeasy Plant Mini Kit (Qiagen Inc., Valencia, CA, USA). One µg RNA was DNase digested (Promega, Madision, WI, USA) followed by cDNA synthesis with iScript cDNA Synthesis Kit (BIO-RAD, Hercules, Ca, USA). RT-PCR primers (Table S1) were designed over exon-exon junctions and set on a Tm ranging from 58–62°C with a GC-content to 45–55%. Actin was used as a control to assure intact RNA.
The tissue-level expression pattern of the AtCRT1a, CRT1b and CRT3 genes were studied using the β -glucuronidase (GUS) reporter gene. A genomic DNA fragment approximately extending 1.5-kb upstream from the ATG starting codon for the genes were amplified and inserted, using BamHI and NcoI, in front of the GUS gene in the pCAMBIA1305 GUS-Plus vector (Table S1). The constructs were transformed into wild-type plants by Agrobacterium-mediated transformation . Transgenic plants were selected on hygromycin, and used for GUS reporter analyses. Tissues were incubated in GUS staining solution (100 mM sodium phosphate, pH 7.0, 10 mM EDTA, 1 mM ferricyanide, 1 mM ferrocyanide, and 1 mM 5-bromo-4-chloro-3-indolyl β-D-glucuronic acid) at 37°C. After clearing in 70% ethanol, the tissues were observed for GUS staining under a dissecting microscope.
Arabidopsis seeds were germinated and grown for three days on ½ Murashige and Skoog (MS) medium with 0.8% (w/v) agar and 1% (w/v) sucrose. Seedlings were subsequently transferred to slides coated with ½ Murashige and Skoog (MS) medium with 0.8% (w/v) agar and 1% (w/v) sucrose, and grown for two additional days. The slides were immersed vertically in liquid covering the lower parts of the roots for 12 and 24 h. The liquids contained either 150 mM glucose, 150 mM sucrose, 150 mM mannitol, 10 µg/ml tunicamycin, 10 mM DTT, or 250 mM salicylic acid, respectively. The seedlings were then immersed in GUS staining solution and treated as described above.
Peptide anti-rabbit antibodies were raised against the AtCRT1a (GDDSDNESKSEETKEAE), the CRT1b (SEETSEKDATAHD), and for the CRT3 as described in . An N-terminal cysteine was added to allow affinity purification on SulfoLink Coupling Gel (Pierce Biotechnology) according to manufacturer's protocol. The buffer was exchanged to PBS (137 mM NaCl, 2.7 mM KCl, 10vmM Na2HPO4, 2 mM KH2PO4, pH 7.4) using a PD10 column (Pharmacia Amersham). The pre-immune sera for the respective antibodies were handled the same way. The specificity of the peptide antibodies were confirmed using mutants for the respective CRTs. The CRT maize antibody were used in dilution 110 000 .
Two-week-old roots from seedling grown in a liquid culture were fixed for 3 h in 4% (w/v) paraformaldehyd, 0.05% (w/v) glutaraldehyd in 0.1 M potassium phosphate buffer, pH 5.7. The sections was washed several times in 0.1 M potassium phosphate buffer, and then put in a 25% (w/v) sucrose in potassium phosphate buffer in 4°C over night. The roots were cryo-sectioned to 14 µm sections and washed in PBS with 0.25% (w/v) Triton X-100, 2×15 min. They were incubated with the respective antibody and pre-immune serum, diluted 1500 in PBS with 0.25% (w/v) Triton X-100 and 1% (w/v) BSA, over night in a moist chamber. The sections were washed in PBS, 2×15 min and than incubated with Alexa Fluor 488 antibody (Molecular Probes), 1200 in PBS with 1% BSA for 1 h in darkness in a moist chamber. The sections were washed as before in PBS and then mounted with glycerol and PBS at a ratio of 91. Microscopy was performed in a wide field fluorescent microscopy with GFP filter.
Roots for TEM were fixed for 24 h at 4°C in 4% (w/v) paraformaldehyde, 0.25% (w/v) glutaraldehyde in 0.1 M potassium phosphate buffer, at pH 5.7. The roots were washed several times in 0.1 M potassium phosphate buffer and embedded in lowicryl according to . Fifty µm thick sections on nickel grids were blocked for 1 h in PBS with 1% BSA and 0.1% Tween 20. The grids were then added to primary antibodies, (in PBS with 0.1% BSA and 0.01% Tween 20, diluted 150 AtCRT1b and 1200 callose [1-3-β-glucan (Biosupplies, Australia)] at 4°C 16 h. The grids were washed three times in PBS and incubated with a secondary gold antibody (Aunoprobe EM GAR15, or AunoProbe EM GAM G10) ratio 130 diluted in the same buffer as the primary antibody for 3 h in room temperature and then washed with PBS, fixed with 1% (w/v) glutaraldehyde for 5 minutes and washed with dH2O three times for one h. The grids were stained with 2% uranyl acetate for 30 min, and with lead citrate according to  for 3 minutes. TEM was performed in a JEOL 1230 transmission electron microscopy.
An AtCRT3 cDNA was introduced into a TOPO cloning vector (Invitrogen, CA, USA) using primers according to Table S1. An endogenous restriction site close to the C-terminal end (AgeI) was used to clone in the CFP (Table S1), resulting in the plasmid pTOPO:AtCRT3-CFP. The AtCRT3 tagged CFP was cut out using BstEII and SpeI and was introduced into a pCAMBIA1302 after the 35S promoter. The resulting plasmid was introduced into tobacco leaves via agrobacterium leaf infiltration (culture OD600=19) essentially according to . Confocal microscopy was carried out on a Leica SP5 TCS confocal fitted to a Leica BM6000B upright microscope equipped with a 63X water objective. CFP was visualized using a 405 nm Lazer controlled by Leica Application Suite Advanced Fluorescence imaging software. For the CRT3-CFP images, one µm Z-stack sections were recorded (36 sections in total), which were merged to a single Z-stack image using the Leica Application Suite Advanced Fluorescence imaging software.
A full-length AtCRT3 cDNA (GenBank Accession U66345) or mutated AtCRT3 were cloned into a pcDNA3.1/Zeo vector containing a hemagglutinin epitope (HA) tag in the C terminus, upstream of the ER retention signal (HDEL) of AtCRT3 to generate pcDNA-AtCRT3-HA. Site-specific mutagenesis was carried out for the mutated AtCRT3 using a QuickChange II Site-directed mutagenesis kit (Stratagene, La Jolla, Ca, USA). Two amino acids were mutated from Asn268 to Asp268 and Leu270 to Glu270. The mutated amino acids were placed at N268 and L270 respectively. Throughout this work, the mutated AtCRT3 will be referred to AtCRT3m. Wild-type and crt−/− mouse embryonic fibroblasts were grown at 37°C in a 5% CO2 environment in Dulbecco's modified Eagle's medium containing 10% (w/v) fetal bovine serum and 1% (w/v) penicillin streptomycin-glutamine . crt−/− cells were transfected with pcDNA AtCRT3-HA or pcDNA CRT3m-HA using Effectene Transfection Reagent (Qiagen Inc., Valencia, CA, USA), and stable transfected cell lines were selected in the presence of 400 µg ml−1 zeocin. Five of these cell lines were analyzed more in detail with respect to AtCRT3 or AtCRT3m protein expression, subcellular localization, and effects on Ca2+ homeostasis and putative protein folding.
SDS-PAGE was carried out essentially according to  with a Bio-Rad Mini-Protean II electrophoresis system. For mouse embryonic fibroblasts, the cells were lysed with RIPA buffer (50 mM Tris-HCl, pH 7.5, 150 mM NaCl, 1 mM EGTA, 1 mM EDTA, 1% (w/v) Triton-X100, 0.5% (w/v) deoxycholic acid, 0.1% (w/v) SDS, 1 mM benzamidine, 1 mM PMSF, 0.025 mg ml−1 aprotinin, 0.01 mg ml−1 pepstatin, 0.05 mg ml−1 E-64, 0.025 mg ml−1 leupeptin and 0.1 mg ml−1 tosyl phenylalanyl chloromethyl ketone (TPCK)) and proteins were solubilized by addition of sample buffer (125 mM Tris HCl, pH 6.8, 4% (w/v) SDS, 20% (v/v) glycerol, 5% β-mercaptoethanol and 0.02% bromphenol blue), and separated using a 12% SDS-polyacrylamide gel. For immunoblotting analysis, proteins were electrophoretically transferred to a PVDF membrane (Millipore) for 1 h at 100 V. After transfer, the membrane was blocked with 5% blocking solution (5% (w/v) skimmed milk powder in 10 mM Tris-HCl, pH 8.0, 150 mM NaCl), washed in 10 mM Tris-HCl, pH 8.0, 150 mM NaCl and 0.05% (w/v) Tween-20. For mouse embryonic fibroblasts the blotting membranes were probed with antibodies against the HA-tag (11000). The HA-tag antibodies were detected with anti-rat IgG, horseradish peroxidase secondary antibodies (15000). For plants ten or twenty (indicated in figure legends) µg protein from microsomal fractions of cell suspension or homogenate from leaves was used and incubated with the respective antibody [maize CRT (110,000), or peptide antibodies for the respective CRT (11,000)], and a secondary antibody [110,000 (antirabbit IgG from Amersham Biosciences)] linked with horseradish peroxidase. Detection was obtained using the Enhanced Chemiluminescence protocol (BioRad Laboratories) and developed on hyperfilm ECL (Amersham Biosciences). The anti-EFR, and anti-FLS2 sera used was described in .
To localize AtCRT3 and CRT3m intracellularly in mouse embryonic fibroblasts, cells were cultured on coverslips, washed with PBS (5 mM potassium phosphate buffer, pH 7.5, 150 mM NaCl), fixed with 4% (w/v) formaldehyde, extracted with 0.1% (w/v) saponin, 2% (w/v) milk powder in PBS, and incubated with HA-tag monoclonal antibodies (150) and PDI polyclonal antibodies (1500). The HA-tag antibodies were detected with fluorescence Alexa Fluor anti-rat secondary antibodies at 546 nm and the PDI antibodies with fluorescence Alexa Fluor anti-rabbit secondary antibodies at 488 nm. The nucleus was stained with DAPI (4,6-diamidino-2-phenylindole), and visualized at 350 nm. All imaging was done on a Zeiss confocal microscope.
Mouse embryonic fibroblasts were lysed with RIPA buffer and used for glycosidase analysis, SDS-PAGE and immunoblotting. Recombinant PNGase F was used for the N-linked glycosidase treatment (New England Biolabs, Beverly, MA). De-glycosylation was carried out essentially according to the manufacturer's protocol under native conditions
Mouse embryonic fibroblasts were cultured for 50 h in the presence of 55 µCi 45Ca2+ . Cells were then washed twice with 5 mM EDTA in PBS, and then once with 5 mM EDTA in culture medium (without fetal bovine serum), detached from Petri dishes by trypsinization (0.25% (w/v) trypsin and 0.02% (w/v) EDTA in Ca2+/Mg2+-free PBS), and finally resuspended in Ca2+-free buffer (143 mM NaCl, 6 mM KCl, 1 mM MgSO4, 20 mM Hepes-NaOH, pH 7.4, 0.1% (w/v) glucose and 0.1 mg mL−1 sulfinpyrazone). For 45Ca2+ release experiments, aliquots of 5×106 cells mL−1 were preincubated for 3 min at 37°C followed by treatment with thapsigargin or ionomycin for 4 min at 37°C. Cells were then pelleted by centrifugation (9,600g for 3 min) and the radioactivity in the supernatant was measured in a Beckman LS 7800 scintillation counter. Background values, i.e. radioactivity recovered in the supernatant in control incubations without additions of thapsigargin or ionomycin, were subtracted prior to presentations in Figures.
Cells were incubated with 2 µmol L−1 Fura 2-AM (Sigma-Aldrich) in Ca2+ buffer (143 mM NaCl, 6 mM KCl, 1 mM MgSO4, 20 mM Hepes-NaOH, pH 7.4, 0.1% (w/v) glucose, 1 mM CaCl2 and 0.1 mg ml−1 sulfinpyrazone) essentially as described in , washed with PBS, trypsinized (0.25% (w/v) trypsin and 0.02% (w/v) EDTA in Ca2+/Mg2+-free PBS), centrifuged, washed in Ca2+-free buffer (143 mM NaCl, 6 mM KCl, 1 mM MgSO4, 20 mM Hepes, pH 7.4, 0.1% (w/v) glucose and 0.1 mg ml−1 sulfinpyrazone), centrifuged, and resuspended in Ca2+-free buffer at 1×106 cells ml−1. The cells were transferred to a cuvette and 2 mM EGTA was added. Fluorescence was measured at λex=340 nm or 380 nm and λem=510 nm. When the resting free cytoplasmic Ca2+ level of the cells (basal Ca2+ level) was reached the cells were stimulated with 600 nM bradykinin (Figure 5H). Thapsigargin (300 nM), a SERCA (ER Ca2+-ATPase) inhibitor, was later added to the cells to measure the Ca2+ store in the ER and to control that no Ca2+-release of BK-induced cells were due to incomplete Ca2+ storage functions in the ER (Figure 5H). To measure the store-operated Ca2+ influx, 2 mM CaCl2 was added to the cells. Ionomycin (7.5 µM) together with CaCl2 (4 mM) was added to the cells to obtain the max value and to obtain the minimum value 32 mM EGTA, 24 mM Tris-HCl, pH 7.4 and 0.4% (w/v) Triton X-100 were added to the cells.
Mouse fibroblasts of wild-type, crt−/− and CRT-deficient mouse fibroblasts expressing AtCRT3 or CRT3m were plated, with a density of 300 000 cells per line, in 2.5 mm diameter tissue culture dishes and grown at 37°C in a 5% CO2 environment in Dulbecco's modified Eagle's medium containing 10% (w/v) fetal bovine serum and 1% (w/v) penicillin streptomycin-glutamine for 16 h before phase contrast image and cell counting.
Arabidopsis seeds were germinated and grown on ½ Murashige and Skoog (MS) medium with 0.8% (w/v) agar at 23°C with 16 h of light (100 µE m−2 s−1) and were transferred after one week to ½ MS medium with 0.8% agar containing 0.1 µg mL−1 tunicamycin. After 8 days of tunicamycin treatment the plants were photographed and fresh weight was measured. Dark grown hypocotyls were grown for 6 days on H2O with 0.8% agar in 23°C in dark.
Real-time PCR analysis (Table S1) was performed on six-day-old light grown seedlings grown on 1MS supplemented with 1% sucrose. The real-time PCR was executed using a Step-One plus system (Applied Biosystems, CA, USA), following the outline presented in . The relative numbers for CT were normalized to the house keeping gene ubiquitin10 (UBQ10) that was used as control. For visualization purposes we calculated the 40 cycles minus ΔCT, i.e. the value obtained from the normalized CT value, and therefore obtained positive values for the ΔCT.
A full-length AtCRT1a cDNA (GenBank Accession U66343) or AtCRT3 cDNA (GenBank Accession U66345) was cloned into a p35SBARN binary vector (; Table S1). The construct was transformed into electro-competent Agrobacterium tumefaciens GV3101, and transformed into Atcrt1b mutant by floral dip . Transformed plants were grown on ½ MS medium with 0.8% agar containing 50 µg ml−1 kanamycin (resistance conferred by Atcrt1a and crt1b T-DNA insertion mutation) and 25 µg ml−1 BASTA (resistance conferred from AtCRT1a or CRT3 transgene) for selection to homozygous seed lines. Expression of the transgene was monitored by RT-PCR analyses or western blot.
Anthocyanin content, and ROS accumulation were analyzed as described in , using six-day-old seedlings (anthocyanin assays) or leaf discs (5 mm in diameter) for ROS accumulation).
Statistical significance of differences between treatments or measurements of different cell lines was assessed by Student's t-test (Microsoft Office Excel, Microsoft Corporation, Redmond, WA). The number of replicates and the level of significance is given in text or table.
Expression analyses of AtCRT1a, CRT1b, and CRT3. A. Microarray signal values for AtCRT1a plotted against values for AtCRT1b over 2332 microarray datasets obtained from the Nottingham Arabidopsis Science Center (NASC; http://arabidopsis.info/). B. Expression analysis of AtCRT1a and CRT3 in different Arabidopsis tissues using a semi-quantitative RT-PCR. Upper panel AtCRT1a, middle panel AtCRT3, and lower panel ACTIN that was used as control.
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Expression, glycosylation status and localization of a mutated AtCRT3 in crt−/− mouse fibroblasts. A. Analysis of glycosylation status of AtCRT3 and CRT1a transfected into crt−/− mouse fibroblasts, before and after treatment with N-glycosidase F (PNGase F) for 1 h under native conditions, and probed with HA-tag antibodies. -, without PNGase F and +, with PNGase F. B. Western blot analysis of AtCRT3m produced in crt−/− mouse fibroblasts. The PVDF membranes were probed with anti-HA-tag antibodies. crt−/−, CRT-deficient mouse fibroblasts; Empty vector, mock transfected crt−/− mouse fibroblasts; other cell lines represent AtCRT3m transfected into crt−/− mouse fibroblasts. C to F. Immunolabeling of AtCRT3m-24 produced in CRT-deficient mouse cells with anti-HA-tag; (C) anti-HA for AtCRT3m, (D) anti-PDI (ER-marker), and (E) DAPI (nucleus-marker). F. Overlay, the yellow color indicates identical localization of ER-marker and AtCRT3.
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Cellular Ca2+ content in AtCRT3 expressing fibroblast lines. A. The Ca2+ content was determined by incubation with 45Ca2+ followed by addition of ionomycin to determine total cellular Ca2+ levels. The background values (counts min-1 in supernatant before addition of thapsigargin or ionomycin) were subtracted. Results represent the average ± SE of three independently performed experiments. B and C. Protein loading controls for Fig. 8B (B), and Fig. 9F (C).
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Real-time PCR analysis of different genes for putative ER chaperones in the Atcrt mutants. The relative expression values of the different genes are displayed as 40 minus the normalized deltaCT value. * denote the N/A assay for AtCRT1a in the Atcrt1a and Atcrt1a crt1b mutants.
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We would like to thank Eugenia Maximova (MPI), and Rita Wallén (LU) for technical help with electron microscopy. We would also like to thank Prof. Jeff Harper for the homozygous Atcrt1b-2 line.
Competing Interests: The authors have declared that no competing interests exist.
Funding: NF and SP were funded through the Max-Planck Gesellschaft. MM is supported by the Canadian Institute of Health Research (MOP-15291), and DP was supported by an Alberta Heritage for Medical Research Summer Student Award. MS was supported by the Swedish Research Council, Swedish Foundation for Strategic Research, and The Swedish Research Council Formas. SW was supported by the Carl Tryggers Foundation. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.