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Article

The Rice Cation/H+ Exchanger Family Involved in Cd Tolerance and Transport

by
Wenli Zou
1,2,3,
Jingguang Chen
2,3,4,
Lijun Meng
2,3,
Dandan Chen
2,3,
Haohua He
1,* and
Guoyou Ye
2,3,5,*
1
Group of Crop Genetics and Breeding, Jiangxi Agricultural University, Nanchang 330045, China
2
CAAS-IRRI Joint Laboratory for Genomics-Assisted Germplasm Enhancement, Agricultural Genomics Institute at Shenzhen, Chinese Academy of Agricultural Sciences, Shenzhen 518120, China
3
Shenzhen Branch, Guangdong Laboratory of Lingnan Modern Agriculture, Genome Analysis Laboratory of the Ministry of Agriculture and Rural Affairs, Agricultural Genomics Institute at Shenzhen, Chinese Academy of Agricultural Sciences, Shenzhen 518120, China
4
School of Agriculture, Sun Yat-sen University, Guangzhou 510275, China
5
Rice Breeding Innovations Platform, International Rice Research Institute, Metro Manila 1301, Philippines
*
Authors to whom correspondence should be addressed.
Int. J. Mol. Sci. 2021, 22(15), 8186; https://doi.org/10.3390/ijms22158186
Submission received: 21 June 2021 / Revised: 25 July 2021 / Accepted: 27 July 2021 / Published: 30 July 2021
(This article belongs to the Special Issue Underground Mechanism to Enhance Nutrient Use Efficiency in Rice)
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Abstract

:
Cadmium (Cd), a heavy metal toxic to humans, easily accumulates in rice grains. Rice with unacceptable Cd content has become a serious food safety problem in many rice production regions due to contaminations by industrialization and inappropriate waste management. The development of rice varieties with low grain Cd content is seen as an economic and long-term solution of this problem. The cation/H+ exchanger (CAX) family has been shown to play important roles in Cd uptake, transport and accumulation in plants. Here, we report the characterization of the rice CAX family. The six rice CAX genes all have homologous genes in Arabidopsis thaliana. Phylogenetic analysis identified two subfamilies with three rice and three Arabidopsis thaliana genes in both of them. All rice CAX genes have trans-member structures. OsCAX1a and OsCAX1c were localized in the vacuolar while OsCAX4 were localized in the plasma membrane in rice cell. The consequences of qRT-PCR analysis showed that all the six genes strongly expressed in the leaves under the different Cd treatments. Their expression in roots increased in a Cd dose-dependent manner. GUS staining assay showed that all the six rice CAX genes strongly expressed in roots, whereas OsCAX1c and OsCAX4 also strongly expressed in rice leaves. The yeast (Saccharomyces cerevisiae) cells expressing OsCAX1a, OsCAX1c and OsCAX4 grew better than those expressing the vector control on SD-Gal medium containing CdCl2. OsCAX1a and OsCAX1c enhanced while OsCAX4 reduced Cd accumulation in yeast. No auto-inhibition was found for all the rice CAX genes. Therefore, OsCAX1a, OsCAX1c and OsCAX4 are likely to involve in Cd uptake and translocation in rice, which need to be further validated.

1. Introduction

Cadmium (Cd) is one of the most toxic heavy metal elements in the environment and has an inhibitory effect on the photosynthesis rate, enzyme activity and ion absorption of plant [1,2,3,4]. Cd stress causes the overproduction of reactive oxygen species (ROS), resulting in oxidative stress and negatively affects the defense system of plants [5,6,7], which, in turn, affects the growth and development, and ultimately reduces the yield, nutritional quality and taste of rice [8]. Moreover, Cd can be easily absorbed by rice and accumulated in grains, which are the staple food for more half of the world population [9,10]. Rice with unacceptable Cd content has become a serious food safety problem in many rice production regions due to contaminations caused by industrialization and inappropriate waste management [11,12]. The development of rice varieties with low grain Cd content is seen as an economic and long-term solution of this problem [13,14,15], since rice varieties show significant genetic variation in the ability to accumulate Cd [16,17]. Identification of varieties with high tolerance to Cd and low grain Cd content is feasible. To facilitate the use of molecular breeding methods, including marker-assisted selection, genetic engineering and genome editing, it is important to identify quantitative trait loci (QTLs) and key genes for the regulation of Cd absorption, transport, distribution and accumulation. QTLs identified by using linkage mapping and association analysis in rice have been summarized by Chen et al. (2019) [18].
Cd is absorbed from soil by roots and then translocated into shoots, and finally accumulated in the grains and other tissues [19]. Mechanisms are found to regulate absorption, transportation and accumulation of Cd in plants. Therefore, many genes are involved in the determination of Cd tolerance and acumination and have been reported to play some roles in Cd regulation in rice [18]. The following gene families appear to be particularly important: the mitogen-activated protein kinase (MAPK) family [20,21,22], the cation diffusion facilitator (CDT) family [23], ATP-binding cassette transporter (ABC) superfamily [24,25,26], the ZRT/IRT-like protein (ZIP) family [27,28,29,30], the heavy metal ATPase (HMA) family [31,32,33,34,35,36], the metal tolerance protein (MTP) family [37,38] and the natural resistance-associated macrophage protein (NRAMP) family [39,40,41,42,43,44].
In recent years, the tonoplast Ca2+/H+ exchanger (CAX) family, a member of the Ca2+/cation antiporter superfamily [45], has drawn great interest of researchers. Studies in Arabidopsis and other plant species have shown that CAX genes play important roles in the tolerance of multi-cation, metal transport, elemental distribution and abundance, ion homeostasis and the responses to other abiotic stresses [46,47]. Transgenic lines of CAX genes in multiple species have been shown to be involved in Cd regulation. The cax1 mutant in Arabidopsis thaliana caused higher Cd sensitivity at low concentrations of calcium (Ca), and a stronger accumulation of reactive oxygen species after Cd treatment [48,49]. AtCAX2 and AtCAX4 were reported to confer tolerance to high toxic levels of Cd, zinc (Zn) and manganese (Mn) in tobacco (Nicotiana tabacum L.) [50,51], while root-selective expression of AtCAX4 and AtCAX2 resulted in reduced leaf Cd in tobacco [52]. Overexpression of TuCAX1a and TuCAX1b from Triticum urartu could improve the tolerance and translocation to exogenous Ca and Zn, and inhibit Cd translocation in Arabidopsis [53]. The overexpression of SaCAX2h from Sedum alfredii enhanced the accumulation of Cd in transgenic tobacco [54]. In addition, all Arabidopsis CAX genes except the uncharacterized AtCAX6 involved in low Ca tolerance and Ca transport in yeast [55,56,57]. AtCAX5 was also involved in Mn transport and ion homeostasis in yeast [47,58]. AtCAX2 was found to participate in Ca transport and accumulation in both tomato (Lycopersicon esculentum L.) and potato (Solanum tuberosum L.) [59]. The Atcax1 mutant displayed tolerance to Mn and Mg (magnesium) toxicity and Ca deficiency [60] and increased CBF/DREB1 expression and cold-acclimation response in Arabidopsis [55]. The loss-of-function of both AtCAX3 and AtCAX4 exhibited salt sensitivity in Arabidopsis [61,62]. Heterologous expression in yeast indicates that all rice CAX genes, except OsCAX2, confer tolerance to low Ca [63], and OsCAX4 is also involved in the transport of Ca, Mn and copper (Cu) [64]. However, the roles of the rice CAX transporter family in Cd uptake and transport have not yet been explored. Therefore, this study aimed to characterize rice CAX genes, paying particular attention to the regulation of Cd. Bioinformatics approaches were used to conduct phylogenetic analysis and gene-structure analysis, including the number of exons and introns, and transmembrane structure. The expression pattern was studied by using qRT-PCR. Tissue-specificity of expression in the seedling stage was detected by GUS staining. Subcellular localization of the functional genes was investigated by transiently expressing GFP-gene fusion into rice protoplasts. Cd transport activity was tested by transforming yeast strains BY4741. In addition, the functions of the CAX family genes in ion transport in multiple species were summarized to assist in studying the roles of the rice CAX genes in other metals and ions. The results of this study have important theoretical significance and application value for rice genetics and breeding.

2. Results

2.1. Bioinformatics Analyses of CAX Family Genes in Oryza sativa and Arabidopsis thaliana

Both Arabidopsis and rice have six CAX genes. All identified CAX members were named based on their phylogenetic relationships (Figure 1). The two subfamilies (Type IA and Type IB) formed by the two main branches of the phylogenetic tree each have three genes from Arabidopsis and three genes from rice (Figure 1). Chromosome mapping showed that the six rice CAX genes are distributed on chromosomes 1, 2 (two genes), 3, 4 and 5 (Figure 1 and Table 1). The six CAX genes of Arabidopsis are distributed on chromosomes 1 (two genes), 2, 3 (two genes) and 5 (Figure 1 and Table 1). The CDS regions of the rice CAX genes range in length from 1089 to 1362 bp and encoded proteins with lengths of 363–454 amino acid residues, molecular weights of 39.07–49.11 KDa and pI values of 4.57–7.00 (Table 1). The length of CDS, encoded proteins with lengths, molecular weights and pI values of the Arabidopsis CAX genes range in length from 1326 to 1428 bp, 441–475 amino acid residues, 48.10–51.84 KDa and pI values of 4.45–6.51, respectively (Table 1). AtCAX1, with a relatively long length, appears to be distinct from the other five members of the Subfamily IA proteins (Table 1). OsCAX4, with a relatively short length, appears to be divergent from the other five members of the Subfamily IB proteins (Table 1). Gene structures were different in each of the two main subfamilies, as illustrated in Figure 1. Subfamily IA members have 8–11 exons and 7–10 introns. Subfamily IB members have 10–12 exons and 9–11 introns. The four members of the IB subfamily (AtCAX2, AtCAX5, AtCAX6 and OsCAX4) all have 12 exons and 11 introns. In particular, OsCAX4 was classified into Type IB phylogenetically and has no UTR (Figure 1). The rice CAX proteins have 8–11 putative transmembrane domains (TMDs) (Table 1 and Figure S1). Except for AtCAX3, which contains 11 TDMs, all other Arabidopsis CAX proteins have 10 putative TDMs (Table 1 and Figure S1).
In BLASTP analysis, the identity between the CAX genes is high with a minimum value of 54%, indicating that they are relatively conservative (Figure S2a). The Subfamily IB members have a higher degree of similarities, reaching 71% (Figure S2b), in comparison to the Subfamily IA members, which have their highest identity as 64% (Figure S2c). Sequence identity in aligned regions ranges from 31 to 88% outside of selfhits (Table 2), with the highest percentage of identity being between AtCAX5 and AtCAX6. The lowest identity is between OsCAX1c and OsCAX4 (Table 2). These results indicated that the CAX gene family has high homology in Oryza sativa and Arabidopsis thaliana.

2.2. Response of Rice CAX Family Genes to Cd Stress

The CAX genes of Arabidopsis and a few other species to Cd stress have been widely reported [58,65]. We analyzed the expression profiles of all the six rice CAX family genes, using qRT-PCR, under different CdCl2 treatments. The transcription levels of all the six genes were significantly upregulated in roots under the 30 and 100 μM CdCl2 treatments, and the expressions were increased with increasing Cd concentrations (Figure 2A). The highest expression was observed for OsCAX1a in roots treated with 100 μM CdCl2 (Figure 2A). Under 10 μM CdCl2 treatment, the expression of OsCAX1b, OsCAX1c and OsCAX4 in roots was similar to the untreated control (Figure 2A). The transcription levels in leaves were also significantly induced by all Cd treatments (Figure 2B). OsCAX1b and OsCAX2 showed relatively high expression in leaves under 100 μM CdCl2, with OsCAX1b being the highest among the six genes, while the other four CAX genes were highly expressed in leaves when treated at 30 μM CdCl2 (Figure 2B). These results suggested that the rice CAX genes could respond to Cd stress.

2.3. Functional Analysis of Rice CAX Genes in Yeast

Since the phenomena of auto-inhibition at the N-terminus have been reported for CAX genes in multiple species [58,66,67,68,69], the full-length rice CAX genes and their 15 N-terminal truncated versions were included in our functional test by using heterologous yeast assay. To create the truncated version without affecting the transmembrane structure, we removed several amino acids from the N-terminal (Figure S4). The truncated versions used were three ΔOsCAX1a (OsCAX1a-12AA, OsCAX1a-28AA and OsCAX1a-40AA), three ΔOsCAX1b (OsCAX1b-11AA, OsCAX1b-22AA and OsCAX1b-33AA), three ΔOsCAX1c (OsCAX1c-14AA, OsCAX1c-24AA and OsCAX1c-37AA), two ΔOsCAX2 (OsCAX2-16AA and OsCAX2-40AA), three ΔOsCAX3 (OsCAX3-10AA, OsCAX3-19AA and OsCAX3-40AA) and one ΔOsCAX4 (OsCAX4-29AA). Then they were expressed in wild-type yeast strain BY4741(MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0). On a SD-Gal medium without Cd, there were no differences in growth between the control carrying an empty vector (vector control) and the CAX-carrying yeast strains (Figure 3A). For the truncated versions of genes, the yeast cells expressing OsCAX1a, OsCAX1c, OsCAX4 had better growth than the vector control on SD-Gal medium containing 160 μmol/L CdCl2, while the other three genes showed no significant difference with the vector control on the SD-Gal medium containing 40 or 160 μmol/L CdCl2 (Figure 3A). Consequently, we did not find N-terminal auto-inhibition of the rice CAX genes.
Further experiments using liquid media with different Cd concentrations were conducted to confirm their Cd transport activity. Without Cd, all CAX genes expressing yeast cells showed similar growth to the control. However, the growth of BY4741 was significantly promoted by OsCAX1a (ΔOsCAX1a), OsCAX1c (ΔOsCAX1c) and OsCAX4 (ΔOsCAX4) when 10, 20 or 40 μmol/L CdCl2 was supplemented (Figure 3B–D and Figure S3). In addition, N-terminal auto-inhibition was still not observed in experiments using liquid medium either (Figure S3). Under the 24 h Cd exposure, OsCAX1a and OsCAX1c enhanced Cd accumulation, while OsCAX4 reduced Cd accumulation (Figure 3E). These results indicated that OsCAX1a, OsCAX1c and OsCAX4 had Cd transport activity in yeasts and might be involved in Cd uptake, transport and accumulation in rice.

2.4. Expression Pattern and Subcellular Localization of the Rice CAX Genes

To investigate the expression patterns of rice CAX genes, the expression in tissues of seedlings, booting, flowering and grain filling stages grown under normal field conditions were measured by qRT-PCR. We found that OsCAX1c was specifically expressed in leaves, with very limited expression elsewhere, while other genes were detected in all tissues of different growth stages (Figure 4A). It was obvious that OsCAX1c, OsCAX3 and OsCAX4 were strongly expressed in leaves (Figure 4A). Both OsCAX1a and OsCAX2 were expressed at a high level in flowering spikelet but weakly in leaves. The expression of OsCAX1b in roots and leaves was slightly higher than in other tissues (Figure 4A).
To further investigate their tissue-specific expression, we developed stable transgenic rice lines expressing the GUS reporter gene driven by the OsCAX1a, OsCAX1b, OsCAX1c, OsCAX2, OsCAX3 or OsCAX4 (−2000 bp from the start codon) promoter. Transgenic seedlings were cultured in deionized water for 14 days, and then various tissues were collected and stained for GUS detection (Figure 4B). All the six genes were observed in roots including the root tip (0.2 cm from the root tip), root hair (2 to 3 cm from the root tip) and root lateral branching zones. OsCAX3 and OsCAX4 expressed abundantly throughout the primary and lateral roots. OsCAX3 strongly expressed throughout the stele in primary roots, whereas other genes weakly expressed or hardly expressed at the base of the stele (Figure 4B). All genes, except OsCAX1b, expressed in the primary root tip. In the root–shoot junction, OsCAX1a, OsCAX1b and OsCAX3 strongly expressed, with OsCAX3 showing slightly higher expression than OsCAX1a and OsCAX1b. OsCAX1a and OsCAX2 hardly expressed in leaves; OsCAX1c, OsCAX3 and OsCAX4 were more strongly expressed in leaves than OsCAX1b (Figure 4B). These results were consistent with the (qRT–qPCR) results shown in Figure 4A.
To determine the subcellular localization of OsCAX1a, OsCAX1c and OsCAX4 proteins in plant cells, we constructed GFP fusion protein and transformed it into rice-sheath protoplasts. OsCAX1a, OsCAX1c and OsCAX4 fused with GFP was observed at the periphery protoplasts (Figure 5). Moreover, OsCAX1a and OsCAX1c were co-localized with the tonoplast membrane marker AtTPK, suggesting that both OsCAX1a and OsCAX1c were localized in the vacuolar membrane (Figure 5). The merge images of OsCAX4-GFP and FMTM4–64 indicated the plasma membrane subcellular localization of OsCAX4 (Figure 5). Vacuolar localization of OsCAX1a has been reported previously by Kamiya et al. (2005) [63]. The membrane localizations of OsCAX1a, OsCAX1c and OsCAX4 were consistent with their cation/H+ exchanger functions, which suggested that the rice CAX genes might play important roles in Cd regulation.

3. Discussion

3.1. The CAX Family Genes in Rice Have High Identity to Their Homologues in Arabidopsis Thaliana

It is well-known that the homeostasis of intracellular Ca2+ plays an important role in signal transduction of stresses and is necessary for normal cell growth [44]. Hence, control of Ca2+ concentration is critical to cellular function. The Ca2+/cation antiporter (CaCA) superfamily members, including MHX (Mg2+/H+ exchanger), CCX (cation/Ca2+ exchanger) and CAX, are the most important Ca2+ transporters. The CaCA exchangers family structure is highly conserved in related plants [70]. Here, we explored the structural characteristics of CAX transporters through phylogenetic tree analysis, transmembrane structure and homology identification of CAX family proteins in rice and Arabidopsis. It was found that the two subfamilies formed by the two main branches of the phylogenetic tree each have three Arabidopsis genes and three rice genes (Figure 1), and the length of the CDS region and the encoded proteins, the molecular weight and the range of pI values were all relatively close in rice and Arabidopsis (Table 1). The gene structures of the two main subfamilies are slightly different. The members of Subfamily IA have 8–11 exons and 7–10 introns. The members of Subfamily IB have 10–12 exons and 9–11 introns, which were one more than those of the Subfamily IA members (Figure 1). CAX family proteins have 8–11 putative transmembrane domains (Figure S1). It is worth noting that the identity between CAX genes is high, the sequence identity in the aligned region ranges from 31 to 88% outside of selfhits (Table 2) and the homology among all CAX genes reached 54% (Mate Figure S2). Taken together, the CAX family genes in rice have high identity to their homologues in Arabidopsis thaliana, indicating that functional similarities are expectable, which is advantageous in leveraging the relatively more abundant information accumulated in Arabidopsis to speed up studies in rice.

3.2. N-Terminal Auto-Inhibition Was Not Found for the Rice CAX Genes Tested Using Cd Treatment

N-terminal auto-inhibition has been widely reported for CAX genes in different species [58,67,68,69], and it is most widely studied in Arabidopsis [66,71,72]. For instance, we found that deleting 36 amino acids at the N-terminus of AtCAX1 ORF improved Ca and Mn tolerance compared to the full-length AtCAX1 ORF by heterologous transformation of yeast [71,72]. The modified AtCAX2 (sCAX2A) with a domain of AtCAX2 and without the N-terminal autoinhibitory domain elevated Ca accumulation in the fruits of tomato. Mn transport in yeast was controlled by the N-terminus of tomato LeCAX2 [58]. The absence of N-terminal regulatory region (NRR) of the cotton (Gossypium hirsutum) GhCAX3 altered cold tolerance compared to full-length of GhCAX3 [68]. It has also been reported in rice that the N-terminus of CAX family genes (Type IA) regulates Ca tolerance and transport in yeast. OsCAX1a∆27 and OsCAX1c∆47 strongly enhanced the Ca tolerance of yeast, and OsCAX1b was more sensitive to 100 mM CaCl2 than OsCAX1b∆36 was [63]. We transformed the yeast strain BY4741 with all members of the rice CAX genes and their corresponding truncated versions with the removal of the 10–40 amino acids from the N-terminal. The Cd transport activity in yeast did not show any differences, indicating that the N-terminal auto-inhibition was not shown for Cd in rice. However, it is best not to interpret this as an indication that the N-terminal auto-inhibition is not present in the rice CAX genes, since we only tested for Cd. Kamiya et al. (2005) [63] reported that OsCAX2 and the N-terminal truncation mutants of OsCAX2 (OsCAX2∆26) expressed in yeast did not show Ca tolerance. The modified Arabidopsis CAX2 (sCAX2A) also showed almost no changes in Mn, Cu and Fe accumulation in the fruits, compared to the overexpression of AtCAX2 in tomato [73]. More detailed studies are needed to (dis)validate this observation.

3.3. Rice CAX Genes, Particularly OsCAX1a, OsCAX1c and OsCAX4, Might Be Important in Controlling Cd Uptake and Translocation in Rice

Existing studies have shown that the CAX genes in plants are involved in ion tolerance, transport and homeostasis, as shown in Figure 6 and Table S3. However, the response of rice CAX genes to Cd has not been studied. Our results showed that the expression of all the six rice CAX genes were upregulated by high-concentration CdCl2 treatments. This was particularly true in roots, for which gene expression increased with increasing Cd concentration (Figure 2). By transforming the BY4741 yeast strain, we found that OsCAX1a, OsCAX1c and OsCAX4 had better Cd tolerance than the control on a SD-Gal medium containing 160 μmol/L CdCl2 and more active in liquid media containing Cd (Figure 3A–D). OsCAX1a and OsCAX1c increased, while OsCAX4 decreased, the accumulation of Cd in yeast (Figure 3E). Thus, OsCAX1a, OsCAX1c and OsCAX4 involve in Cd tolerance and transport in yeast, implying that they might involve in Cd tolerance and accumulation in rice as well. As discussed above, the rice CAX family genes have high identity to their homologous genes in Arabidopsis, indicating that their functions may be conserved. Three Arabidopsis CAX genes, namely AtCAX1 [48,49], AtCAX2 and AtCAX4 [50,51,52], were verified by transgenic methods to participate in Cd tolerance, transport and accumulation (Figure 6 and Table S3). OsCAX1a has very high homology with AtCAX1 and AtCAX4, reaching 64% and 56%, respectively (Figure 1 and Table 2). OsCAX1c has high homology with AtCAX1 (57%) and AtCAX4 (49%) (Figure 1 and Table 2). OsCAX1a strongly expressed in spikelet and nodes, while OsCAX1c very strongly expressed in leaves (Figure 4A). Both of OsCAX1a and OsCAX1c are most likely to locate on the vacuolar membrane. OsCAX4 on plasma membrane has the highest identity (54%) to AtCAX2 (Figure 1 and Table 2) and is strongly expressed in roots and grains. Taken together, we speculate that OsCAX1a, OsCAX1c and OsCAX4 may play different roles in the key processes, including the absorption by the roots, the xylem loading, the distribution and transportation via the nodes, and the redistribution in the leaf via phloem. These processes collectively determine the plant tolerance and accumulation of Cd.
Although OsCAX1b, OsCAX2 and OsCAX3 did not show Cd transport activity in our yeast assay (Figure 3), their roles in Cd regulation could not be completely ruled out. Firstly, their expression levels in roots and leaves were all induced by Cd treatments (Figure 2). Secondly, OsCAX1b and OsCAX3 were previously reported to involve in tolerance to Ca, and OsCAX3 also confers Mn tolerance in yeast [63]. Thirdly, CAX proteins function as Ca2+/H+ and/or heavy metal/H+ exchangers [56,73]. The importance of Ca2+ acts as a secondary messenger in the signal transduction of various biotic and abiotic stimuli in plants has been well documented [74,75,76]. Changes in apoplastic pH or Ca2+ concentrations can be expected to strongly affect Cd binding capacity, since Cd2+ and Ca2+ have similar ionic radii [77]. Fourthly, CAX genes interact with other genes to form regulatory network controlling tolerance to metals. Yeast two-hybrid analysis showed that AtCAX1 directly interacts with AtSOS2, which is a serine/threonine kinase whose function is essential for salt tolerance in Arabidopsis [78]. Co-expression of AtSOS2 specifically activated AtCAX1 and integrated Ca transport in yeast and salt tolerance in Arabidopsis [79]. Therefore, it is likely that CAX genes interact with key genes for Cd absorption and accumulation, or are regulated by transcription factors or phosphorylated by receptor kinases to affect Cd transport. Fifthly, since CAX genes have high degree of genetic identity, it is likely that some of the genes may have functional redundancy (Table 2). Thus, any test/assay using a single gene, as we performed, may fail to identify the function of a gene. Indeed, it has been reported that the AtCAX1 and AtCAX3 function as dimers, and co-expressing both AtCAX1 and AtCAX3 mediated Ca, lithium (Li) and salt tolerance in yeast [61,80], and affected element distribution and abundant Arabidopsis seeds [81].
In conclusion, we investigated all rice CAX genes and demonstrated that OsCAX1a, OsCAX1c and OsCAX4 were associated with Cd tolerance and Cd transport in yeast. They are also highly likely to involve in Cd tolerance, absorption and accumulation in rice; however, further validation through transgenic methods in rice is needed.

4. Materials and Method

4.1. Identification and Bioinformatics Analyses of the Cation/H+ Antiporters from Oryza sativa and Arabidopsis thaliana Species

To identify CAX homologs in rice, the nucleic acid and amino acid sequences of all reported CAX genes in Arabidopsis and rice were downloaded from the rice (accessed on 16 December 2019; http://www.ricedata.cn/gene/) and Arabidopsis (accessed on 16 December 2019; https://www.arabidopsis.org/) databases. CAX genes were named according to the phylogenetic relationship between proteins. The protein molecular weight and theoretical isoelectric point (pI) value were calculated by ProtParam (accessed on 16 December 2019; http://web.expasy.org/protparam/). The DNAMAN software (accessed on 1 March 2019; https://www.lynnon.com/dnaman.html) was used to determine the sequence identity between rice and Arabidopsis CAX proteins, and the homology between subfamilies. The transmembrane structures in the proteins were predicted through TMHMM Server v2.0 (accessed on 3 June 2021; http://www.cbs.dtu.dk/services/TMHMM/). The subcellular localization of unreported CAX proteins were predicted by using CELLO v2.5 (http://cello.life.nctu.edu.tw/ (accessed on 21 May 2021; http://cello.life.nctu.edu.tw/). Multi-sequence alignment was performed with Clustal W (accessed on 1 January 2021; Clustal Omega, ClustalW and ClustalX Multiple Sequence Alignment) and drawn in Genedoc. Phylogenetic trees based on full-length protein-sequence alignments were constructed by the neighbor-joining method with 1000 bootstrap replicates, using MEGA 7.0 software (accessed on 1 January 2021; http://www.megasoftware.net/download_form). The downloaded coding DNA sequences (CDS) and genome sequences of CAX genes were used to construct gene structure by the Gene Structure Display Server 2.0 (accessed on 16 December 2019; http://gsds.cbi.pku.edu.cn/index.php).

4.2. Plant Materials and Growth Conditions

Rice (Oryza sativa L. cv. Nipponbare) seeds were surface-sterilized with 10% (v/v) hydrogen peroxide solution for 30 min, thoroughly rinsed, washed six times with deionized water and germinated for 48 h under dark conditions and a temperature of 30 °C [82]. The dew-white and uniformly growing seeds were sown in a 96-well polymerase chain reaction (PCR) plate (8 × 12) with perforated wells at the bottom to facilitate the roots to fully contact with the nutrient solution [83]. The nutrient solution was prepared according to the composition of IRRI solution: 1.0 mM MgSO4·7H2O, 1.25 mM NH4NO3, 0.3 mM KH2PO4, 1.0 mM CaCl2, 0.35 mM K2SO4, 0.5 mM Na2SiO3, 20.0 μM Fe-EDTA, 20.0 μM H3BO3, 9.0 μM MnCl2, 0.77 μM ZnSO4, 0.32 μM CuSO4 and 0.39 μM (NH4)6Mo7O24, at pH 5.5. The nutrient solution was replaced every three days. Rice seedlings were grown for 10 days.
The seedlings that grew consistently were moved to a rectangle 3.5 L box containing 2 L of normal nutrient solution, with a 3 × 8 foam board being used as bed, and grown for a week. Then the seedlings were grown under treatment conditions of 0, 10, 30 or 100 μM CdCl2. The nutrient solution was changed every two days and the night before sampling. Culture was conducted in a greenhouse, under natural light, at day/night temperatures of 30 °C/22 °C and 60% relative humidity. After a 2-week treatment, root and leave samples were rapidly taken, frozen in liquid nitrogen and stored in a refrigerator, at −80 °C, for RNA extraction and real-time quantitative reverse-transcription PCR (qRT-PCR) analysis.

4.3. RNA Extraction and Real-Time PCR

Total RNA was extracted by using the TRIzol reagent (Vazyme Biotech Co. Ltd., Nanjing, China). DNaseI-treated total RNAs were subjected to reverse transcription (RT) with the HiScript II Q Select RT SuperMix for qPCR (+gDNA wiper) kit (Vazyme Biotech Co. Ltd., Nanjing, China). Transcript levels of selected genes were measured by qRT-PCR, using the CFX96® Real-Time PCR System using the 2 × T5 Fast qPCR Mix (SYBRGreenI) kit (Vazyme Biotech Co. Ltd., Nanjing, China). Rice actin gene (Rac1) was used for normalization. The ΔΔCt method was used to calculate the relative transcript abundance [78]. The primers for qRT-PCR are given in Table S1.

4.4. Functional Analysis of Rice CAX Genes in Yeast

The heterologous yeast assay was utilized to identify the Cd transport ability of rice CAX proteins by transforming the BY4741 yeast strain (MATa his3Δ1 leu2Δ0 met15Δ0 ura3Δ0). All CAX genes were amplified from full-length cDNA clones, using the PCR primers lying downstream from the start codon and just upstream of the stop codon (Table S2). The protocol for removing some amino acids from the N-terminus of the CAX transporters was described in detail by Shigaki et al. (2010) [72]. Using BamH I and EcoR I, we ligated each rice CAX gene into the pYES2 vector (Invitrogen), with correct direction, using a ClonExpress® Ultra One Step Cloning Kit (Vazyme Biotech Co. Ltd., Nanjing, China), resulting in the pYES2-OsCAXs construct. The vectors truncated were verified by Sanger sequencing. Empty vector pYES2 and the CAX gene vectors were then transformed into BY4741 yeast cells, respectively, according to the manufacturer’s protocol (Yeast Transformation Kit; Beijing Coolaber Technology Co. Ltd., Beijing, China). Transformants were selected on synthetic dextrose medium without uracil (SD-Ura) and verified by PCR with yeast plasmid extraction (Yeast Plasmid Extraction Kit; Beijing Solarbio Technology Co. Ltd., Beijing, China). Positive clones were cultured on an SD-Ura liquid medium until the early logarithmic phase. For plate growth tests, yeast transformants were diluted to an OD600 of 1.0, 0.1, 0.01 and 0.001, step by step, with sterile water; 6 μL of the cell suspension was spotted on SD-Ura plates containing 0, 40 or 160 μmol/L CdCl2, respectively. The plates were incubated at 30 °C for 2 days before the growth phenotypes were evaluated.
To quantify the growth of BY4741 yeast strain transformed with various plasmids in liquid SD-Ura media containing CdCl2 overnight yeast cells were prepared and the optical density (OD) at 600 nm was adjusted to 0.8 with sterile distilled water. Then 20 μL of cell suspensions was added to 20 mL liquid SD-Ura media containing 0, 10, 20 or 40 μmol/L CdCl2. The OD values at 600 nm were determined at the indicated time.
For the Cd concentration determination, the yeast transformants were cultured overnight with a liquid SD-Ura medium with 2% galactose, at 30 °C and 200 rpm, until the OD600 reached 0.8. Then the yeast transformants were treated with 5 μM CdCl2 for 24 h. The yeast strain carrying empty vector was used as control. The cultures of each set were harvested in pre-weighed microfuge tubes by centrifugation and washed with sterile water for three times. After aspirating the supernatant, pelleted cells were dried in the oven, overnight, at 60 °C. The samples were wet-digested by using 5 mL concentrated HNO3+HClO4 (4 + 1), at 120 °C, in a heating block for 30 min. After cooling, the digested solution was diluted to 15 mL with deionized water. The Cd concentrations were determined by inductively coupled plasma–mass spectrometry (ICP–MS). All the assays were performed at least three times.

4.5. Tissue Expression Assay

For histochemical analysis of GUS activity, the upstream 2.0 kb genomic fragment of each gene was cloned into pCAMBIA1300 to generate OsCAXs promoter: GUS vector. The vectors were then transformed into Nipponbare to produce transgenetic plants. The GUS staining Solution (1 mg/mL) from (Beijing Coolaber Technology Co., Ltd., Beijing, China) was used to determine the activity of GUS. The samples were incubated at 37 °C for 24 h, and the solution containing (X-gluc dry powder + X-gluc solution): GUS staining buffer = 1:50. After staining, green tissue materials (such as leaves) were treated 2 or 3 times by 75% ethanol to remove chlorophyll and decolorize until the negative control material was white. GUS activity was detected by a stereoscopic fluorescence microscopy (TL5000; Leica Microsystems).

4.6. Subcellular-Localization Assay

Subcellular localization was investigated by transiently expressing GFP-OsCAXs fusion into rice protoplasts. The ORF of OsCAX1a, OsCAX1c and OsCAX4 were amplified by PCR from rice (‘Nipponbare’) root cDNA, using primers (Table S2). Protoplasts generated from the young stems of 3-week-old rice seedlings grown under light were transformed with transient expression plasmids, according to Bart et al. (2006) [84]. GFP fluorescence signals were detected with a TCS SP5 confocal laser scanning microscope (Leica Microsystems) at 500–535 nm, after excitation at 488 nm, while FMTM4–64 (plasma membrane specific localization dye) was excited at 543 nm and scanned at 600–630 nm. Double staining using AtTPK (red signal) as the tonoplast membrane marker was used for further confirmation of the subcellular localization. For co-localization experiments, sequential scanning was done for both of the channels and then merged together to show overlapping signals. All the images were further processed by using Leica LAS AF Lite software.

Supplementary Materials

The following are available online at https://www.mdpi.com/article/10.3390/ijms22158186/s1.

Author Contributions

Conceptualization and methodology, G.Y., H.H. and J.C.; validation, W.Z., J.C., L.M. and D.C.; formal analysis and data curation, W.Z. and D.C.; writing—original draft preparation, W.Z., G.Y.; writing-review and editing G.Y.; supervision, G.Y. and J.C.; project administration, G.Y. and L.M.; funding acquisition, G.Y. and L.M. All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by Shenzhen Science and Technology, Program, JCYJ20190813104211014; the National Natural Science Foundation of China, 31961143016; the open funds of the State Key Laboratory of Crop Genetics and Germplasm Enhancement, Nanjing Agricultural University, ZW202011 and the Agricultural Science and Technology Innovation Program, CAAS-ZDRW202001.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

All data generated or analyzed during this study are included in this published article.

Acknowledgments

We thank Jiaolong Li and Wenna Yang for excellent technical assistance.

Conflicts of Interest

The authors declare no conflict of interest.

Abbreviations

ABCATP-binding cassette
CAXCation/H+ exchanger
CaCACa2+/cation antiporter
CCXCation/Ca2+ exchanger
CDTCation diffusion facilitator
HMAHeavy metal ATPase
ICP-MSInductively coupled plasma mass spectrometry
MAPKMitogen-activated protein kinase
MHXMg2+/H+ exchanger
MTPMetal tolerance protein
NRRN-terminal regulatory region
TFTranscription factors
TMDsTransmembrane domains

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Figure 1. Phylogenetic relationship of CAX family genes of Oryza sativa and Arabidopsis thaliana. The phylogenetic tree was constructed based on sequence alignment of CAX homologs from Arabidopsis (At) and rice (Os), using the neighbor-joining method with bootstrapping analysis implemented in MEGA 7.0. The CAX proteins are clustered into two groups (Type IA and Type IB). Gene structures were drawn, using Gene Structure Display Server 2.0 with genomic sequences and CDS sequences. Introns and exons are represented by black lines and yellow boxes, respectively. Blue boxes represent UTRs.
Figure 1. Phylogenetic relationship of CAX family genes of Oryza sativa and Arabidopsis thaliana. The phylogenetic tree was constructed based on sequence alignment of CAX homologs from Arabidopsis (At) and rice (Os), using the neighbor-joining method with bootstrapping analysis implemented in MEGA 7.0. The CAX proteins are clustered into two groups (Type IA and Type IB). Gene structures were drawn, using Gene Structure Display Server 2.0 with genomic sequences and CDS sequences. Introns and exons are represented by black lines and yellow boxes, respectively. Blue boxes represent UTRs.
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Figure 2. Expression of rice CAX genes under CdCl2 treatments. The relative transcript levels were quantified by qRT–PCR in (A) roots and (B) leaves (mixed collection of shoots and leaves) of rice variety Nipponbare grown in hydroponic culture under 0, 10, 30 or 100 μM CdCl2 treatment with the IRRI solution for 7 days. The rice actin gene (Rac1) was used as an internal reference to normalize gene-expression data. Statistical comparison was performed by one-side t-test (* p < 0.05 and ** p < 0.01). Values are mean ± SE (n = 3, three replicates with tissues being collected from three plants per replicate, three plants per pool).
Figure 2. Expression of rice CAX genes under CdCl2 treatments. The relative transcript levels were quantified by qRT–PCR in (A) roots and (B) leaves (mixed collection of shoots and leaves) of rice variety Nipponbare grown in hydroponic culture under 0, 10, 30 or 100 μM CdCl2 treatment with the IRRI solution for 7 days. The rice actin gene (Rac1) was used as an internal reference to normalize gene-expression data. Statistical comparison was performed by one-side t-test (* p < 0.05 and ** p < 0.01). Values are mean ± SE (n = 3, three replicates with tissues being collected from three plants per replicate, three plants per pool).
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Figure 3. Functional assay of rice CAX genes by heterologous expression in yeast. (A) Yeast mutant strain expressing the empty vector pYES2 or vectors for CAX genes grown in SD-Ura medium containing galactose without Cd or with different Cd concentrations. Pictures were taken after 2 days of growth at 30 °C. The growth curve of empty vector, OsCAX1a, OsCAX1c and OsCAX4 transformed yeast BY4741 strain in liquid medium with (B) 0, (C) 20 or (D) 40 μM CdCl2. The absorbance at 600 nm (OD600) of cell cultures was measured every 5 h. (E) Cd accumulation in the wild-type BY4741 (gray) and BY4741 expressing OsCAX1a (green), OsCAX1C (red) and OsCAX4 (orange) treated with 5 μM CdCl2 for 24 h. Statistical comparison was performed by one-side t-test (* p < 0.05 and ** p < 0.01). Error bar indicates standard deviation, and the data are presented as means ± SD (n = 3).
Figure 3. Functional assay of rice CAX genes by heterologous expression in yeast. (A) Yeast mutant strain expressing the empty vector pYES2 or vectors for CAX genes grown in SD-Ura medium containing galactose without Cd or with different Cd concentrations. Pictures were taken after 2 days of growth at 30 °C. The growth curve of empty vector, OsCAX1a, OsCAX1c and OsCAX4 transformed yeast BY4741 strain in liquid medium with (B) 0, (C) 20 or (D) 40 μM CdCl2. The absorbance at 600 nm (OD600) of cell cultures was measured every 5 h. (E) Cd accumulation in the wild-type BY4741 (gray) and BY4741 expressing OsCAX1a (green), OsCAX1C (red) and OsCAX4 (orange) treated with 5 μM CdCl2 for 24 h. Statistical comparison was performed by one-side t-test (* p < 0.05 and ** p < 0.01). Error bar indicates standard deviation, and the data are presented as means ± SD (n = 3).
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Figure 4. Tissue expression pattern. (A) Relative expression of rice CAX members in various tissues at different growth stages. Various tissues samples were taken from cv. Nipponbare grown in a paddy field. (B) Localization of pOsCAXs-GUS expression in transgenic rice plants. GUS staining pattern in tissues of 14-day-old seedlings cultured with de-ionized water: (a) root tip, (b) 2 to 3 cm from the root tip, (c) root lateral branching zones, (d) hand-cut cross-section of the root–shoot junction and (e) leaves. (a–c) Scale bar = 0.5 mm. (d,e) Scale bar = 2 mm.
Figure 4. Tissue expression pattern. (A) Relative expression of rice CAX members in various tissues at different growth stages. Various tissues samples were taken from cv. Nipponbare grown in a paddy field. (B) Localization of pOsCAXs-GUS expression in transgenic rice plants. GUS staining pattern in tissues of 14-day-old seedlings cultured with de-ionized water: (a) root tip, (b) 2 to 3 cm from the root tip, (c) root lateral branching zones, (d) hand-cut cross-section of the root–shoot junction and (e) leaves. (a–c) Scale bar = 0.5 mm. (d,e) Scale bar = 2 mm.
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Figure 5. Subcellular location of OsCAX1a, OsCAX1c and OsCAX4 in rice protoplasts. (a) The fluorescence of OsCAX1a-GFP, AtTPK (left), and overlay of FM4–64 and OsCAX1a-GFP, bright field (right) are shown, respectively. (b) The fluorescence of OsCAX1c-GFP, AtTPK (left), and overlay of AtTPK and OsCAX1c-GFP, bright field (right) are shown, respectively. (c) The fluorescence of OsCAX4-GFP, FMTM4–64 (left), and overlay of FMTM4–64 and OsCAX4-GFP, bright field (right) are shown, respectively. Bars = 10 μm.
Figure 5. Subcellular location of OsCAX1a, OsCAX1c and OsCAX4 in rice protoplasts. (a) The fluorescence of OsCAX1a-GFP, AtTPK (left), and overlay of FM4–64 and OsCAX1a-GFP, bright field (right) are shown, respectively. (b) The fluorescence of OsCAX1c-GFP, AtTPK (left), and overlay of AtTPK and OsCAX1c-GFP, bright field (right) are shown, respectively. (c) The fluorescence of OsCAX4-GFP, FMTM4–64 (left), and overlay of FMTM4–64 and OsCAX4-GFP, bright field (right) are shown, respectively. Bars = 10 μm.
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Figure 6. Model of the involvement of CAX family members in ion transport in plants. Ions are transported with the help of CAX genes. The solid black border indicates the subcellular location of the known genes, and the dotted line indicates the subcellular location predicted by CELLO v2.5 (accessed on 21 May 2021; http://cello.life.nctu.edu.tw/).
Figure 6. Model of the involvement of CAX family members in ion transport in plants. Ions are transported with the help of CAX genes. The solid black border indicates the subcellular location of the known genes, and the dotted line indicates the subcellular location predicted by CELLO v2.5 (accessed on 21 May 2021; http://cello.life.nctu.edu.tw/).
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Table
Table 1. Basic characteristics of CAX family genes in Oryza sativa and Arabidopsis thaliana.
Table 1. Basic characteristics of CAX family genes in Oryza sativa and Arabidopsis thaliana.
GeneLocusLength of CDS (bp)No. of Amino
Acids (aa)		ChromosomeMW (KDa)pITypeNo. of Transmembrane Domains
OsCAX2LOC_Os03g279601317439347.484.57IB10
OsCAX3LOC_Os04g559401254418445.454.76IB11
OsCAX4LOC_Os02g046301089363239.077.00IB8
OsCAX1aLOC_Os01g376901356452147.716.78IA10
OsCAX1bLOC_Os05g516101362454549.116.34IA10
OsCAX1cLOC_Os02g210091353451248.165.62IA8
AtCAX1AT2G381701428475251.646.25IA10
AtCAX2AT3G133201326441348.214.45IB10
AtCAX3AT3G518601380459349.855.39IA11
AtCAX4AT5G014901365454549.616.51IA10
AtCAX5AT1G557301326441148.104.61IB10
AtCAX6AT1G557201404467151.845.40IB10
Table
Table 2. Percentage of protein sequence identity among the CAX family proteins of Oryza sativa and Arabidopsis thaliana.
Table 2. Percentage of protein sequence identity among the CAX family proteins of Oryza sativa and Arabidopsis thaliana.
% IdentityOsCAX1aOsCAX1bOsCAX1cOsCAX2OsCAX3OsCAX4AtCAX1AtCAX2AtCAX3AtCAX4AtCAX5AtCAX6
%%%%%%%%%%%%
OsCAX1a100
OsCAX1b69100
OsCAX1c5958100
OsCAX2505243100
OsCAX349514074100
OsCAX43638315555100
AtCAX1646257484938100
AtCAX246494472725446100
AtCAX36766565048397948100
AtCAX4565949464734574759100
AtCAX548494472735248874947100
AtCAX64745386665534682474588
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Zou, W.; Chen, J.; Meng, L.; Chen, D.; He, H.; Ye, G. The Rice Cation/H+ Exchanger Family Involved in Cd Tolerance and Transport. Int. J. Mol. Sci. 2021, 22, 8186. https://doi.org/10.3390/ijms22158186

AMA Style

Zou W, Chen J, Meng L, Chen D, He H, Ye G. The Rice Cation/H+ Exchanger Family Involved in Cd Tolerance and Transport. International Journal of Molecular Sciences. 2021; 22(15):8186. https://doi.org/10.3390/ijms22158186

Chicago/Turabian Style

Zou, Wenli, Jingguang Chen, Lijun Meng, Dandan Chen, Haohua He, and Guoyou Ye. 2021. "The Rice Cation/H+ Exchanger Family Involved in Cd Tolerance and Transport" International Journal of Molecular Sciences 22, no. 15: 8186. https://doi.org/10.3390/ijms22158186

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