Open access peer-reviewed chapter

Phytochelatin Synthase in Heavy Metal Detoxification and Xenobiotic Metabolism

Written By

Ju-Chen Chia

Submitted: June 20th, 2021 Reviewed: June 25th, 2021 Published: September 14th, 2021

DOI: 10.5772/intechopen.99077

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Abstract

Phytochelatin synthase (PCS) is well-known for its role in heavy metal detoxification in plants, yeasts and non-vertebrate animals. It is a protease-like enzyme that catalyzes glutathione (GSH) to form phytochelatins (PCs), a group of Cys-rich and non-translational polypeptides with a high affinity to heavy metals. In addition, PCS also functions in xenobiotic metabolism by processing GS-conjugates in the cytosol. Because PCS is involved in GSH metabolism and the degradation of GS-conjugates, it is one of the important components in GSH homeostasis and GSH-mediated biodegradation. This chapter reviews the biochemical mechanism of PCS, how the enzyme activity is regulated, and its roles in heavy metal detoxification as well as GS-S-conjugate metabolism. This chapter also highlights the potential applications of PCS in the improvement of plant performance under combined stresses.

Keywords

  • Phytochelatin synthase
  • heavy metal stress
  • GS-conjugate metabolism
  • glutathione
  • combined pollution

1. Introduction

Phytochelatins (PCs, (γGlu-Cys)n-Gly, n = 2–11) are cysteine-rich polypeptides that are synthesized non-translationally from the tripeptide glutathione (GSH, γGlu-Cys-Gly); this process is catalyzed by phytochelatin synthase (PCS, EC 2.3.2.15) [1, 2, 3, 4]. PCs play essential roles in heavy metal detoxification because of their high affinities to a broad range of metal ions, e.g. cadmium (Cd), mercury (Hg), arsenic (As), zinc (Zn), lead (Pb), silver (Ag), nickel (Ni) and copper (Cu) [1, 2, 3]. Upon exposure to heavy metals, PCs are synthesized in the cytosol to chelate free metal ion and to prevent the generation of hydroxyl radicals [4, 5, 6] (Figure 1). These PC-metal complexes eventually are transferred into the vacuole through specific tonoplast ABCC-type transporters for sequestration [22, 23, 24, 25, 26] (Figure 1). In plants, PCS is constitutively expressed in the cytosol and can be activated by multiple types of metal ions [1, 3, 6]. For example, AtPCS1 isolated from Arabidopsis thalianacan be activated by the metal ions mentioned above [6]. In addition, some PCS homologs, such as the model legume Lotus japonicusLjPCS1 and LjPCS3, can be activated by iron (Fe) and aluminum (Al) [27].

Figure 1.

The involvement of phytochelatin synthase in glutathione metabolism, heavy metal detoxification, and glutathione-S-conjugate degradation.

An overview of the roles of phytochelatin synthase (PCS) in the metabolic pathways of glutathione (GSH, γ-Glu-Cys-Gly). The brief pathway of GSH biosynthesis and the major route of glutathione-S-conjugate (GS-conjugate) degradation are also shown in the figure [7,8,9]. The presence of xenobiotic compounds (X, marked as green circles) and free heavy metal ions (red circles) induces ROS generation and causes oxidative stress. The cytosolic xenobiotic compound is transferred to GSH by glutathione S-transferase (GST) to initiate the detoxification, and then the GS-conjugates enter vacuoles for further degradation [10,11,12,13]. In the vacuoles, GS-conjugates are first catalyzed to Cys-Gly-conjugates by γ-glutamyl transpeptidase (GGT) before the final deglycination catalyzed by carboxypeptidase (CP)[14,15,16]. In the presence of heavy metals, PCS uses GSH as substrates to synthesize phytochelatins (PCs), which chelate free metal ions in the cytosol [4]. Heavy metals also activate PCS to initiate the cleavage of GS-conjugates [17,18,19,20]. The cytosolic γ-Glu-Cys-conjugates then enter vacuoles and serve as the substrates of GGT for the second step of degradation [21]. The blue cylinders represent tonoplast ABCC transporters that facilitate the import of GS-metabolites and PC-metal complexes [12,13,22,23,24]. In the brief biosynthetic pathway of GSH, the rate-limiting enzymes are indicated in bold. Note that the cellular compartmentation of GSH synthesis or redox reactions is not included in this figure. SAT, serine acetyltransferase; γ-ECS, γ-glutamylcysteine synthetase; GSH-S, GSH synthetase. GP, GSH peroxidase; GR, GSH reductase. The figure was created withBioRender.com.

PCS can be found in plants, yeasts and non-vertebrate animals and plays a critical role in responding to heavy metal stress in these organisms [28, 29, 30, 31, 32]. It was first partially purified from the suspension cells of bladder campion (Silene cucubalus) for its ability to synthesize PCs from GSH in the presence of Cd2+ [4]. Soon after the isolation of the enzyme, the genes coding PCS were cloned from plant and yeast sources, including AtPCS1, TaPCS1 from wheat (Triticum aestivum), and SpPCS from Schizosaccharomyces pombeby three independent research groups [5, 33, 34]. Since then, PCS sequences from various model organisms have been largely characterized, such as Caenorhabditis elegans(CePCS1) [31], the Cd hyperaccumulator Thlaspi caerulescens(TcPCS1) [35], and Oryza sativa(OsPCS1, OsPCS2, OsPCS5, OsPCS15) [36, 37, 38]. Besides eukaryote PCS sequences, a gene encoding a PCS-like protein, NsPCS, was identified from the genome of cyanobacterium Nostocsp. [39, 40, 41, 42].

PCS is a key component for the heavy metal tolerance in plants. Its importance was first confirmed in the Arabidopsis mutants locking AtPCS1 activity, as these mutants show severe growth defects when challenged by heavy metals such as Cd2+, Hg2+, Zn2+, Pb2+, and As3+ [28, 43, 44, 45]. The synthesis of PCs is crucial to the local response to heavy metal stress and is also involved in the roots-to-shoots translocation of heavy metals [26, 37, 43, 46]. The first evidence of the long-distance transfer of PC-metal complexes is that the PCs synthesized in the roots can be translocated to the shoots via phloem loading and vice versa[26, 43, 46]. Additionally, plants defective in PC synthesis show altered patterns of heavy metal accumulation at the whole-plant level while being sensitive to heavy metal stress. For example, the Arabidopsis AtPCS1-deficient mutant, cad1–3, accumulated significantly less Cd in the shoots than the wild type or the transgenic line heterologously overexpressing TaPCS1 [43], and the rice OsPCS2RNAi plants failed to transfer As3+ from the roots to the shoots [37]. Overall, the phenotypes of these PCS-deficient mutants suggest heavy metal ions absorbed through the roots can be loaded into the shoots in the form of PC-chelates.

PCS is a well-known multitasker involved in different biological processes [21, 47]. Besides its significant role in synthesizing PCs from GSH, PCS can catalyze the deglycination of GSH-S-conjugates (GS-conjugates), and thus, it is involved in the GS-conjugate catabolism [17, 18, 19, 20, 21, 48]. In addition, PCS is also associated with indole glucosinolates metabolism and immune responses [49, 50, 51]. Intriguingly, the catalytic-site mutants of PCS are still functional in this pathway, which suggests that the role of PCS in the indole glucosinolate metabolism is independent of PC synthesis and GS-metabolism [51]. Among these PCS-involving biological processes, this chapter focuses on the catalytic mechanism of PCS and its functions in both heavy metal stress and GSH metabolism. The potential applications of PCS in combating multiple stresses are also discussed.

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2. The biochemical mechanism of phytochelatin synthase

2.1 The domain organization of phytochelatin synthase

The eukaryotic PCS has two domains with distinct functions: a conserved N-terminal domain that shows γ-glutamylcysteine dipeptidyl transpeptidase activity and a variable C-terminal domain involved in metal sensing [52, 53, 54]. Using AtPCS1 as a model, the molecular functions of the N- and C-domains as well as the catalytic mechanism of eukaryotic PCS were revealed [6, 53, 54, 55]. The N-terminal half AtPCS1 is sufficient for deglycination of GSH and elongating PC molecules, indicating that the N-terminal domain carries out the core catalysis [53, 56]. However, the truncated AtPCS1 without the C-terminal domain is less thermostable and has lower PC synthetic activity than the full-length enzyme [53, 55, 56]. Notably, the deletion of the C-terminal domain completely impairs the PC synthesis activity of the enzyme in the presence of Zn2+ and partially inactivates PC synthesis in the Cd- or Hg-containing reactions [53, 55]. These findings suggest that the C-terminal domain is essential for stabilizing the protein and functions as a metal sensor [53, 55]. More evidence has shown that the C-terminal end of AtPCS1 is required for the augmentation of PC synthetic activity. One example is that the residues from Asp373 to the C-terminal end of AtPCS1 contain multiple regions involved in Zn-dependent and As-dependent activation of PC synthesis [45, 57, 58]. (Also see Section 2.4: The activation of phytochelatin synthase through the chelation of heavy metal ions).

PCS-like sequences also exist in prokaryotes with moderate sequence homology to the N-domain of eukaryotic PCS [39, 40, 41]. However, prokaryotic PCS likely has unique functions apart from PC synthesis. For example, the PCS homolog found in cyanobacterium Nostocsp. PCC 7120 (NsPCS) shows distinct characters from its eukaryotic counterparts that efficiently catalyze PC synthesis. NsPCS is a “half-PCS molecule” that does not have a C-terminal domain [39, 40, 52] and catalyzes the hydrolysis of GSH at a high rate and the synthesis of PCs at a relatively low rate [39, 40, 42]. Besides, the enzyme activity of NsPCS seems insensitive to the absence or presence of Cd2+, which suggest that the prokaryotic PCS is involved in GSH metabolism in the cells rather than the responses to heavy metal stress [39, 42].

2.2 The core catalytic mechanism

Vatamaniuk et al. [6] first confirmed that the synthesis of PCs occurs through a ping-pong mechanism and involves two substrates: one GSH as the low-affinity substrate for the first step of PC synthesis and one metal-GSH conjugate as the high-affinity substrate for the second step [6]. In the standard PC synthesis reactions in vitro, which resemble the concentrations of the GSH and metal ions in the cytosol, GSH exists at a considerably higher level (millimolar) than heavy metal ions (micromolar) [6, 7, 59]. Presumably, more than 98% of total metal ions in this condition are associated with GSH as bis(glutathionato)metal ions (metal∙GS2), and the free Cd concentration can be as low as 10−6 μM [6]. Under these circumstances, GSH and Cd∙GS2 are two separate compounds for PC synthesis.

Right after GSH enters the catalytic site of PCS, a Gly residue is removed to form the γGlu-Cys acyl-enzyme intermediate, and then a metal-GS2 accepts the γGlu-Cys unit to generate a PC2 ((γGlu-Cys)2-Gly) [6, 21, 54, 55]. Following the synthesis of PC2, the elongation of PCs occurs using previously synthesized PCs as acceptors to receive γGlu-Cys [6, 21, 54, 55, 60]. The whole process can be described as two equations:

PCS+γGlu-Cys-GlyPCS-γGlu-Cys+GlyE1
PCS-γGlu-Cys+metalγGlu-Cys-Gly2PCS+metalγGlu-Cys2-Gly+γGlu-Cys-GlyE2

Overall, PCS catalyzes the peptide chain elongation from C-to-N terminus [4, 6, 21, 54]:

γGlu-Cys-Gly+γGlu-Cysn-GlyγGlu-CysγGlu-Cysn-Gly+GlyE3

PCS and Cys proteases share similar core catalytic mechanisms to hydrolyze a GSH molecule and form a γ-Glu-Cys-acyl–enzyme intermediate [41, 52]. The Cys protease-like catalytic triad of PCS was confirmed based on the mutagenic studies of AtPCS1 and the crystal structures of NsPCS [41, 54, 55]. Vatamaniuk et al. and Romanyuk et al. reported that Cys56, His162, and Asp180 of AtPCS1 are the three residues of the catalytic triad among divergent PCS sequences [54, 55]. The molecular interaction between these residues and GSH was further revealed by Vivares et al. with the crystal structures of native NsPCS and the γ-Glu-Cys-acyl–enzyme intermediate at a 2.0-Å resolution [41]. Although NsPCS only shares 36% identity at the amino acid level with AtPCS1, it contains the conserved catalytic triad and can catalyze the deglycination of GSH [39, 40, 41, 42]. These crystal structures provide details about the hydrolysis of the peptide bond that involves Cys56 and the 3D structure of the Cys-His-Asp catalytic triad [41]. It is worth mentioning that NsPCS formed homodimers in the crystallization experiments [26]. This is in agreement with the dimerization of the partially purified PCS from Silene cucubalus, which was confirmed by determining the native molecular weight of the protein [4].

2.3 Critical amino acids contributing to the enzyme activity

Based on the high-resolution crystal structure of NsPCS, multiple research groups have simulated putative 3D structures of eukaryotic PCS using various programs, and these structure models provide valuable information that uncovers the conserved molecular mechanism of PCS [56, 61, 62, 63, 64, 65]. For example, the molecular models of AtPCS1 reveal the key amino acids that contribute to the mechanism of the second substrate recognition and the enzyme activation through Thr phosphorylation [56, 61]. Chia et al. first reported how AtPCS1 might attract and stabilize the second substrate, metal-GS2, after the γ-Glu-Cys-acyl–enzyme intermediate is formed [61]. In this study, the modeled AtPCS1 structure revealed a pocket in proximity to the first substrate-binding site, consisting of three loops containing several conserved amino acids, including Arg152, Lys185, and Tyr55. Mutations on Arg152 or Lys185 (Arg-to-Lys or Lys-to-Arg substitutions) resulted in the complete abrogation of enzyme activity, indicating that the arrangement of these positive charges is crucial for the binding of the second substrate. Mutations at Tyr55 did not completely impair the enzyme activity, but the Tyr55 mutant AtPCS1 showed lower catalytic activities than the wild-type enzyme due to a reduced affinity to metal-GS2. In addition, the mutation at Tyr55 reduced Cd2+ binding ability of the AtPCS1 protein. It was therefore suggested that Tyr55 binds to the Cd ion of metal-GS2 through cation-π interaction and thus contributes to the recognition of the second substrate. Besides these three amino acids, other conserved residues on the loops constituting the second substrate-binding pocket, including Gln50, Glu52, Glen157, Phe184, and Tyr186, are also important for the PC synthesis activity [61, 62].

Wang et al. identified that Thr49 is the phosphorylation site related to the activation of AtPCS1 [56]. The mutant AtPCS1 with Thr49-to-Ala49 substitution could not be phosphorylated, and its PC synthesis activity was significantly lower than that of the wild-type enzyme. According to the proposed 3D model of AtPCS1, Thr49 is within proximity to Arg183, which is also crucial for the catalytic activity of AtPCS1, and both residues are next to the catalytic site and substrate binding pockets. It was proposed that the phosphorylated Thr49 interacts with Arg183, and that this interaction serves as a “molecular clip” to give the active site a conformation appropriate for catalysis. Because Thr49 and Arg183 are both highly conserved among PCS sequences, the activity of eukaryotic PCS may as well be regulated by similar phosphorylation modifications [56, 66].

2.4 The activation of phytochelatin synthase through the chelation of heavy metal ions

As a key component of early response to heavy metal stress, PCS protein is constitutively expressed in the cytosol for rapid activation stimulated by heavy metals [2, 3, 6]. The heavy metal ions entering cytosol are essential for forming the second substrate [6, 60]. They can also bind to PCS, resulting in augmentative activation [6, 55, 67, 68]. Moreover, heavy metals could be a critical factor that triggers PCS phosphorylation [56, 69]. For example, AtPCS1 phosphorylation only occurred in the presence of Cd2+ in the in vitroexperiments [56].

PCS, confirmed to be a metalloenzyme in vitro, is also likely to be one in vivo[6, 17]. Equilibrium analyses show that one AtPCS1 molecule binds seven Cd2+ in solutions containing 10 μM CdCl2 [6, 61]. Apart from Tyr55, which is proposed to bind the Cd2+ on the metal-GS2, the Cd binding capability of PCS presumably comes from conserved Cys pairs and CysXXCys motifs also found in metallothionein [30, 61]. Peptide screening of SpPCS and TaPCS showed that the core sequences containing consensus Cys-rich motifs could bind Cd2+in vitro[67]. The subsequent site-direct mutagenesis analysis indicated that conserved Cys pairs at the N-terminal domain were critical for PCS activity, while the Cys-rich motifs at the C-terminal domain only slightly affected the PC synthesis rate [67]. It is not yet clear how these Cys-rich motifs enhance the PC synthesis rate. It is possible that they bind metal-GS2 complexes or free metal ions to stabilize the protein structure [6, 30, 55, 67]. More investigations are still needed to explain the molecular functions of these Cys-rich motifs and how they participate in the metal activation of PCS.

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3. Phytochelatin synthase-targeting genetic engineering approaches in phytoremediation of heavy metals

3.1 The effects of phytochelatin synthase overexpression on the accumulation of heavy metals in plants

PC synthesis plays a critical role in heavy metal tolerance and accumulation. It is therefore no surprise that the breeding and engineering approaches for phytoremediation requiring heavy metal hyperaccumulators have focused on strategies to enhance PC biosynthetic capacity [48, 70, 71, 72, 73, 74, 75, 76]. Studies have shown that the transgenic plants expressing functional PCS usually have a higher tolerance to heavy metal stress. For example, the overexpression of AtPCS1 in Arabidopsis, tobacco or Indian mustard (Brassica juncea) enhanced Cd, Zn, and As tolerance and accumulation [71, 77, 78, 79, 80]. Other PCS homologs e.g., CePCS, TaPCS1, NtPCS1, CdPCS from an aquatic As-accumulator plant (Ceratophyllum demersum), MaPCS1/MaPCS2 from mulberry (Morus alba), and VsPCS1 from legume Vicia sativawere also used to develop transgenic plants that accumulate higher concentrations of heavy metals than their natural variants [43, 46, 81, 82, 83, 84, 85, 86]. These reports on improving heavy metal accumulation and tolerance of the plants indicate the potential applications of PCS on phytoremediation approaches.

Although PCS can be a molecular tool for phytoremediation of heavy metal-contaminated soils and waters, the overexpression of PCS promotes the catabolism of GSH, which also plays essential roles in redox reactions and heavy metal stress [87, 88]. If the metabolic pathways supplying GSH cannot maintain specific levels in the presence of highly expressed PCS, the consumption of GSH usually leads to changes in the GSH/GSSG ratio that exacerbate oxidative stress [62, 72]. The increased GSH demand driven by PC synthesis may also affect other metabolic pathways requiring GSH [89]. In these regards, the use of functional PCS with diminished catalytic activity could reduce the depletion of GSH, maintain redox homeostasis and supporting PC synthesis during exposure to heavy metals at the same time [62]. Indeed, the Arabidopsis and Brassica junceatransgenic lines expressing a partially deactivated AtPCS1 mutant, AtPCS1-Y186C, showed enhanced Cd2+ tolerance and higher GSH/GSSG ratio than the transgenic lines expressing wild-type AtPCS1 [62]. These results suggest that PC synthesis and redox homeostasis are both important for successful heavy metal resistance.

Besides the imbalance of cellular redox state, PCS overexpression could result in an unknown disruption in cellular metal homeostasis under heavy metal stress because PCS itself is a metalloenzyme and can bind a wide range of metal ions [90, 91]. Expressing synthetic genes encoding peptide analogs of PCs with a general structure of Met(Glu-Cys)nGly (n = 16–20) could be an alternative way to enhance the accumulation of heavy metals in the plants without the overexpression of PCS [92]. The Arabidopsis transgenic plants transformed with the artificial genes encoding these PC-like polypeptides resulted in hyperaccumulation of Cd2+ and As3+/5+ in the plants [92]. However, the impact of accumulating synthetic PC-like polypeptides on the overall metal homeostasis is yet to be determined.

3.2 Phytochelatin synthase-involving pathway engineering for enhancing heavy metal accumulation

Pathway engineering involved in the co-expression of both GSH synthesis and PC synthesis pathways is another strategy to preserve the balance of GSH metabolism in the cells with constitutive PC synthesis [72, 74]. A kinetic model of GSH and phytochelatin synthesis in plants suggests that at least two enzymes, γ-glutamylcysteine synthetase (γ-ECS) and PCS, should be increased to enhance PC synthesis without depleting the GSH pool [89]. In fact, the effects of modified GSH/PC synthesis pathways have been tested in Escherichia coliand tobacco plants, respectively [93, 94]. In these experiments, the activities of SpPCS and two enzymes catalyzing the rate-limiting steps of GSH biosynthesis, including serine acetyltransferase (SAT) and γ-ECS, were enhanced (Figure 1) [7, 8, 93, 94]. The E. colicells co-overexpressing these enzymes accumulated significantly higher concentrations of PCs and Cd2+, while the single-gene expression in the PC synthesis pathway had limited effects [93]. These findings support the “gene stacking” approaches to enhancing heavy metal metabolism. Although the same strategy co-overexpressing these three genes in tobacco increased some classes of non-protein thiol, the Cd2+ accumulation in the transgenic plants did not change compared to the wild type [94]. These findings suggest that other mechanisms, in addition to the availability of precursors for PC synthesis, limit Cd accumulation in plants [94].

Overall, the genetic engineering approaches involved in manipulating PC synthesis have shown promising prospects for improving the performance of plants in the phytoremediation of heavy metals. However, there are also setbacks pointing at the complexity of the stress response induced by heavy metals [75]. Thus, while enhanced PC synthesis can contribute to the heavy metal chelating, other factors, such as the subsequent vacuolar sequestration or the delicate balance of GSH metabolic pathways under heavy metal stress, should be considered in order to achieve heavy metal tolerance.

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4. The role of phytochelatin synthase in glutathione-S-conjugate metabolism

4.1 The involvement of phytochelatin synthase in the catabolism of glutathione derivates

PCS has a broad substrate selectivity and can use GS-derivates as substrates. For example, PCS isolated from plant species can accept S-alkylated GSH such as S-methyl-GS and S-hexyl-GS [6, 95] and large side residues like xenobiotic GS-conjugates (abbreviated as GS-conjugates) [17, 19, 20]. The bulky S-residues of GSH that can be converted to γ-Glu-Cys-conjugates by PCS include benzyl-, nitrophenyl-, phenylbenzyl-, uracil-, bimane-, and acetamido-fluorescein-groups [17, 19]. However, when PCS uses GS-derivates with these bulky S-linked side residues, it tends to transfer the γ-Glu-Cys-conjugate intermediate to a hydrogen group [17, 19, 20]. As a result, PCS processes the hydrolysis of GS-conjugates instead of their polymerization.

Besides its significant role in heavy metal detoxification, PCS also participates in the biodegradation of xenobiotic compounds because of its capability to process GS-conjugates [17, 18, 19, 20]. Glutathione conjugation is a major pathway to inactivate xenobiotic compounds in plant cells [7]. Glutathione transferase (GST) detoxifies xenobiotics in the cytosol by transferring these compounds to GSH [10, 11, 96, 97]. These GS-conjugates enter vacuoles rapidly for sequestration and further degradation [12, 13]. In Arabidopsis, the transport of GS-conjugates for vacuolar sequestration is facilitated by AtABCC1/AtMRP1 and AtABCC2/AtMRP2, which also transfer PC-metal complexes into vacuoles [12, 13, 22, 24]. Because of the high efficiency of this sequestration mechanism, the subsequent catabolism of GS-conjugates is presumably processed in the vacuoles [18]. First, vacuolar γ-glutamyl-transpeptidase (GGT) initializes the degradation of GS-conjugates by removing the γ-Glu-residue from the GS-conjugates to form Cys-Gly-conjugates [14, 15], and then, carboxypeptidase cleaves the Gly residue and results in the accumulation of the Cys-conjugates [16]. Alternatively, the GS-conjugate degradation can be initiated by PCS when vacuolar sequestration is not an available route [17, 18, 19, 20]. The pathways of GS-conjugate metabolism are summarized in Figure 1.

4.2 Phytochelatin synthase may participate in initiating the first step of glutathione-S-conjugates degradation in the cytosol

Monochlorobimane (MCB) is widely used as a model xenobiotic for Arabidopsis to study the catabolism of GS conjugates [14, 15, 17, 18, 19, 20, 98]. The bimane-labeled thiols can be analyzed by high performance liquid chromatography [99]. In addition, the fluorescent GS-bimane can be directly monitored in situ, which indicates the compartmentation and the turnover of GS-conjugates [15, 18, 20]. Data have shown that AtPCS1 initiates the first step of GS-bimane degradation in cytosol by removing the Gly residue and providing substrates for the vacuolar GGT [17, 19, 20, 21] (Figure 1). This detour could be a functionally alternative route to detoxify xenobiotics when the major pathway is blocked [17, 18, 19, 20].

The direct evidence showing the involvement of PCS in GS-conjugate metabolism is the defects in the turnover of GS-bimane shown in the Arabidopsis AtPCS1-deficient mutants [21, 47]. The AtPCS1-deficient mutant, ΔPCS1, and the AtPCS1/AtPCS2 double-deficient mutant, ΔPCS, are impaired in the degradation of GS-bimane to γ-Glu-Cys-bimane [19, 20]. Blum et al. (2007) report that in the absence of Cd2+, the abundance of the γ-Glu-Cys-bimane in both ΔPCS1and ΔPCSmutants was significantly reduced compared to the wild type after the plants were challenged by the xenobiotic bimane [19]. Moreover, the induction of γ-Glu-Cys-bimane was not observed in AtPCS1-deficient lines in the plants treated with Cd2+, which resulted in a > 10-fold lower γ-Glu-Cys-bimane accumulation compared with the wild type grown in the same conditions [19]. The GS-baimane concentration could be rescued by transfecting AtPCS1 cDNA into PCS-deficient protoplasts, suggesting that this process is indeed PCS-dependent [19]. The inhibited γ-Glu-Cys-bimane accumulation in the mutant lines indicates that AtPCS1 efficiently catalyzes GS-conjugates in the presence of Cd2+ [19, 20].

Although the GS-bimane conversion is altered in the AtPCS1-deficient mutants, the GS-bimane in these mutants still can be degraded through the major detoxification pathway in the vacuoles [18, 19, 20]. Besides, the overall turnover of GS-bimane in the mutants is only slightly affected without blocking the vacuolar transport pathway [18, 19, 20]. These findings underline that the vacuolar GGT-initiated GS-conjugates degradation is the major pathway among two compensatory routes responsible for the turnover of the xenobiotics [18].

In plant cells, both the cytosolic PCS and the vacuolar carboxypeptidase can catalyze the formation of γ-Glu-Cys-bimane [16, 17, 18, 19]. However, the vacuolar carboxypeptidase tends to catalyze the Cys-Gly-conjugates following the cleavage of γ-Glu-residue initiated by GGT [15]. In this regard, PCS is supposed to be the primary component responsible for the γ-Glu-Cys-bimane formation observed in the process of GS-conjugate conversion. Another example showing the importance of PCS in the initiation of the cytosolic xenobiotic compound is the metabolism of the herbicide safener fenclorim [100]. Fenclorim enhances GST activity in Arabidopsis and is subsequently degraded via the GS-conjugation pathway [97, 100]. In the Arabidopsis suspension cells, GS-fenclorim was sequentially processed to γ-Glu-Cys-fenclorim and Cys-fenclorim, suggesting that deglycination is the initial step to the catabolism of fenclorim [21, 100]. However, more evidence is needed to confirm the direct involvement of PCS in this process.

4.3 The glutathione-S-conjugate conversion via phytochelatin synthase is metal-dependent

The presence of metal ions is a critical requirement for PCS-dependent catalysis of GS-bimane [17, 18, 19, 20]. Intriguingly, the efficiency of GS-bimane hydrolysis activated by different metal ions is separate from that of metal-stimulated PC synthesis [17]. For example, the PC formation of AtPCS1 activated by Cd2+ is usually 2–5 times more efficient than the PC synthesis rate measured in the presence of Cu+/2+ [4, 6, 53]. On the other hand, AtPCS1 could catalyze the deglycination of GS-bimane 60% more efficiently in Cu+/2+ solutions than in the presence of Cd2+ [17]. It was suggested that in vivoAtPCS1 is a Cu-containing metalloenzyme in unstressed conditions, and consequently, the Cu-bound PCS favors the catalysis of GS-conjugate over PC synthesis in the normal growth conditions [17]. Evidence supporting this hypothesis is that in Arabidopsis, the deglycination of GS-bimane was PCS-dependent in the absence of heavy metals [19]. However, considering AtPCS1 binds Cu2+ only at a low affinity [6, 21], and the majority of cytosolic Cu is usually associated with Cu chaperons [101], it is possible that the concentration of free cytosolic Cu ions is not sufficient to fully activate PCS for the catalysis of GS-conjugates.

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5. Can phytochelatin synthase play a part in the phytoremediation of combined pollutions?

With global industrialization and the development of modern cropping systems, massive amounts of toxic substances such as pesticides, heavy metals and inorganic fertilizers have been released into the environment and caused massive pollutions [97, 102]. Inevitably, the combined contaminations have damaged the ecosystems and become global issues [103, 104].

In the case of soil pollution, the primary sources of heavy metals include pesticides, fertilizers, mining, industrial processing and wastewater [102, 105]. One example of combined pollutants is glyphosate-based herbicides, which are highly toxic to the environment yet are the most-used pesticides in the world [106]. Heavy metals such as As, Ni, and Pb, which activate the catalytic activity of PCS, can be found as contaminants in many commercial glyphosate-based herbicides [3, 6, 106]. Interestingly, the in vivochronic regulatory experiments showed that the toxicity of these herbicides might come from the heavy metals included in formulants instead of the active ingredients [106]. These findings suggest that heavy metal toxicity may occur in the biological materials used in the phytoremediation of xenobiotic compounds. Thus, heavy metal detoxification mechanisms in phytoremediation plants also need to be considered to improve their performance in co-contaminated soils and groundwaters.

GSH and its derivates are widely involved in plant development and stress response, and GSH itself serves as a hub for the mechanisms of heavy metal detoxification, xenobiotics biodegradation and oxidative stress response [7, 9]. Because PCS is a key enzyme in GSH metabolism, it is not surprising that PCS should be involved in both heavy metal stress and the turnover of xenobiotics. Other critical enzymes in the GSH metabolic pathway such as GST have been used in combating multiple stresses, including heavy metal and xenobiotics degradation, and biotic stress [107]. However, the role of PCS is primarily emphasized in heavy metal stress response despite its contribution to the degradation of GS-metabolites and innate immunity. Based on the knowledge about the diverse functions of PCS, it is worth exploring whether PCS can be a useful tool in enhancing the tolerance and performance of the plants challenged by combined stresses.

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6. Conclusion

Both heavy metals and pesticides significantly arrest plant growth and development. The co-contamination of soils by both heavy metals and pesticides has raised concerns regarding crop safety and productivity, and is therefore crucial to remediate. Phytoremediation presents the advantages of high efficiency, low cost, and sustainability. Thus, it has been one of the most common strategies for the remediation of polluted soils. This chapter summarizes the critical role of PCS in heavy metal detoxification and the involvement of PCS in GS-conjugate degradation. In the presence of heavy metals, PCS catalyzes the synthesis of PCs and the initiation of GS-conjugate metabolism. Despite a large body of literature illustrating the function of PCS in heavy metal resistance, there has been less emphasis on the participation of PCS in the detoxification of xenobiotic compounds and its potential application in biodegradation. Given that PCS has diverse functions in different types of stress, this chapter discusses the potential inclusion of PCS to achieve phytoremediation for combined pollutions.

The key question related to PCS overexpression in plant materials for phytoremediation is how GSH homeostasis can be balanced. Although pathway engineering enhancing GSH metabolism and PCS activity seems a promising approach, the consequences of manipulating these pathways may not directly lead to improving the performance of plants exposed to stress, due to the complexity of the cellular GSH network. Thus, the challenge for the future is not only to characterize the involvement of PCS in stress responses but also to broaden our knowledge in PCS as a factor that regulates GSH status and cellular redox homeostasis.

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Acknowledgments

I sincerely thank Dr. Rong-Huay Juang (National Taiwan University of Science and Technology) for stimulating discussion and critical reading of the manuscript.

References

  1. 1. Grill E, Winnacker EL, Zenk MH. Phytochelatins: the principal heavy-metal complexing peptides of higher plants. Science. 1985;230(4726):674-6
  2. 2. Grill E, Winnacker EL, Zenk MH. Synthesis of seven different homologous phytochelatins in metal-exposedSchizosaccharomyces pombecells. FEBS Lett. 1986;197(1-2):115-20
  3. 3. Grill E, Winnacker EL, Zenk MH. Phytochelatins, a class of heavy-metal-binding peptides from plants, are functionally analogous to metallothioneins. Proc Natl Acad Sci USA. 1987;84(2):439-43
  4. 4. Grill E, Löffler S, Winnacker EL, Zenk MH. Phytochelatins, the heavy-metal-binding peptides of plants, are synthesized from glutathione by a specific γ-glutamylcysteine dipeptidyl transpeptidase (phytochelatin synthase). Proc Natl Acad Sci USA. 1989;86(18):6838-42
  5. 5. Clemens S, Kim EJ, Neumann D, Schroeder JI. Tolerance to toxic metals by a gene family of phytochelatin synthases from plants and yeast. EMBO J. 1999;18(12):3325-33
  6. 6. Vatamaniuk OK, Mari S, Lu YP, Rea PA. Mechanism of heavy metal ion activation of phytochelatin (PC) synthase. J Biol Chem. 2000;275:31451-9
  7. 7. Noctor G, Mhamdi A, Chaouch S, Han Y, Neukermans J, Marquez-Garcia B, et al. Glutathione in plants: an integrated overview. Plant Cell Environ. 2012;35(2):454-84
  8. 8. Mendoza-Cózatl D, Loza-Tavera H, Hernández-Navarro A, Moreno-Sánchez R. Sulfur assimilation and glutathione metabolism under cadmium stress in yeast, protists and plants. FEMS Microbiol Rev. 2005;29(4):653-71
  9. 9. Noctor G, Queval G, Mhamdi A, Chaouch S, Foyer CH. Glutathione. Arabidopsis Book. 2011;9:e0142
  10. 10. Hatton PJ, Dixon D, Cole DJ, Edwards R. Glutathione transferase activities and herbicide selectivity in maize and associated weed species. Pestic Sci. 1996;46(3):267-75
  11. 11. Andrews CJ, Skipsey M, Townson JK, Morris C, Jepson I, Edwards R. Glutathione transferase activities toward herbicides used selectively in soybean. Pestic Sci. 1997;51(2):213-22
  12. 12. Lu Y-P, Li Z-S, Rea PA.AtMRP1gene ofArabidopsisencodes a glutathioneS-conjugate pump: Isolation and functional definition of a plant ATP-binding cassette transporter gene. Proc Natl Acad Sci USA. 1997;94(15):8243-8
  13. 13. Lu Y-P, Li Z-S, Drozdowicz YM, Hörtensteiner S, Martinoia E, Rea PA. AtMRP2, an Arabidopsis ATP binding cassette transporter able to transport glutathioneS-conjugates and chlorophyll catabolites: Functional comparisons with AtMRP1. Plant Cell. 1998;10(2):267-82
  14. 14. Ohkama-Ohtsu N, Zhao P, Xiang C, Oliver DJ. Glutathione conjugates in the vacuole are degraded by γ-glutamyl transpeptidase GGT3 in Arabidopsis. Plant J. 2007;49(5):878-88
  15. 15. Grzam A, Martin MN, Hell R, Meyer AJ. γ-Glutamyl transpeptidase GGT4 initiates vacuolar degradation of glutathione S-conjugates in Arabidopsis. 2007;581(17):3131-8
  16. 16. Wolf AE, Dietz KJ, Schröder P. Degradation of glutathioneS-conjugates by a carboxypeptidase in the plant vacuole. FEBS Lett. 1996;384(1):31-4
  17. 17. Beck A, Lendzian K, Oven M, Christmann A, Grill E. Phytochelatin synthase catalyzes key step in turnover of glutathione conjugates. Phytochemistry. 2003;62(3):423-31
  18. 18. Grzam A, Tennstedt P, Clemens S, Hell R, Meyer AJ. Vacuolar sequestration of glutathioneS-conjugates outcompetes a possible degradation of the glutathione moiety by phytochelatin synthase. FEBS Lett. 2006;580(27):6384-90
  19. 19. Blum R, Beck A, Korte A, Stengel A, Letzel T, Lendzian K, et al. Function of phytochelatin synthase in catabolism of glutathione-conjugates. Plant J. 2007;49(4):740-9
  20. 20. Blum R, Meyer KC, Wünschmann J, Lendzian KJ, Grill E. Cytosolic action of phytochelatin synthase. Plant Physiol. 2010;153(1):159-69
  21. 21. Rea PA. Phytochelatin Synthase. eLS2020. p. 1-15
  22. 22. Song WY, Park J, Mendoza-Cózatl DG, Suter-Grotemeyer M, Shim D, Hörtensteiner S, et al. Arsenic tolerance inArabidopsisis mediated by two ABCC-type phytochelatin transporters. Proc Natl Acad Sci USA. 2010;107:6
  23. 23. Mendoza-Cózatl DG, Zhai Z, Jobe TO, Akmakjian GZ, Song W-Y, Limbo O, et al. Tonoplast-localized Abc2 transporter mediates phytochelatin accumulation in vacuoles and confers cadmium tolerance. J Biol Chem. 2010;285(52):40416-26
  24. 24. Park J, Song W-Y, Ko D, Eom Y, Hansen TH, Schiller M, et al. The phytochelatin transporters AtABCC1 and AtABCC2 mediate tolerance to cadmium and mercury. Plant J. 2012;69(2):278-88
  25. 25. Vögeli-Lange R, Wagner GJ. Subcellular localization of cadmium and cadmium-binding peptides in tobacco leaves: implication of a transport function for cadmium-binding peptides. Plant Physiol. 1990;92(4):1086-93
  26. 26. Mendoza-Cózatl DG, Jobe TO, Hauser F, Schroeder JI. Long-distance transport, vacuolar sequestration, tolerance, and transcriptional responses induced by cadmium and arsenic. Curr Opin Plant Biol. 2011;14(5):554-62
  27. 27. Ramos J, Naya L, Gay M, Abián J, Becana M. Functional characterization of an unusual phytochelatin synthase, LjPCS3, ofLotus japonicus. Plant Physiol. 2008;148(1):536-45
  28. 28. Howden R, Goldsbrough PB, Andersen CR, Cobbett CS. Cadmium-sensitive,cad1mutants ofArabidopsis thalianaare phytochelatin deficient. Plant Physiol. 1995;107(4):1059-66
  29. 29. Cobbett CS. Phytochelatins and their roles in heavy metal detoxification. Plant Physiol. 2000;123(3):825-32
  30. 30. Cobbett C, Goldsbrough P. Phytochelatins and metallothioneins: Roles in heavy metal detoxification and homeostasis. Ann Rev Plant Biol. 2002;53(1):159-82
  31. 31. Vatamaniuk OK, Bucher EA, Ward JT, Rea PA. A new pathway for heavy metal detoxification in animals. J Biol Chem. 2001;276(24):20817-20
  32. 32. Bundy JG, Kille P, Liebeke M, Spurgeon DJ. Metallothioneins may not be enough—The role of phytochelatins in invertebrate metal detoxification. Environ Sci Technol. 2014;48(2):885-6
  33. 33. Vatamaniuk OK, Mari S, Lu YP, Rea PA. AtPCS1, a phytochelatin synthase fromArabidopsis: Isolation andin vitroreconstitution. Proc Natl Acad Sci USA. 1999;96(12):7110-5
  34. 34. Ha SB, Smith AP, Howden R, Dietrich WM, Bugg S, O’Connell MJ, et al. Phytochelatin synthase genes from Arabidopsis and the yeastSchizosaccharomyces pombe. Plant Cell. 1999;11(6):1153-64
  35. 35. Küpper H, Parameswaran A, Leitenmaier B, Trtílek M, Šetlík I. Cadmium-induced inhibition of photosynthesis and long-term acclimation to cadmium stress in the hyperaccumulatorThlaspi caerulescens. New Phytol. 2007;175(4):655-74
  36. 36. Das N, Bhattacharya S, Bhattacharyya S, Maiti MK. Identification of alternatively spliced transcripts of rice phytochelatin synthase 2 geneOsPCS2involved in mitigation of cadmium and arsenic stresses. Plant Mol Biol. 2017;94(1):167-83
  37. 37. Yamazaki S, Ueda Y, Mukai A, Ochiai K, Matoh T. Rice phytochelatin synthases OsPCS1 and OsPCS2 make different contributions to cadmium and arsenic tolerance. 2018;2(1):e00034
  38. 38. Park HC, Hwang JE, Jiang Y, Kim YJ, Kim SH, Nguyen XC, et al. Functional characterisation of two phytochelatin synthases in rice (Oryza sativacv. Milyang 117) that respond to cadmium stress. Plant Biol (Stuttg). 2019;21(5):854-61
  39. 39. Harada E, von Roepenack-Lahaye E, Clemens S. A cyanobacterial protein with similarity to phytochelatin synthases catalyzes the conversion of glutathione to γ-glutamylcysteine and lacks phytochelatin synthase activity. Phytochemistry. 2004;65(24):3179-85
  40. 40. Tsuji N, Nishikori S, Iwabe O, Shiraki K, Miyasaka H, Takagi M, et al. Characterization of phytochelatin synthase-like protein encoded by alr0975 from a prokaryote,Nostocsp. PCC 7120. Biochem Biophys Res Commun. 2004;315(3):751-5
  41. 41. Vivares D, Arnoux P, Pignol D. A papain-like enzyme at work: Native and acyl–enzyme intermediate structures in phytochelatin synthesis. Proc Natl Acad Sci USA. 2005;102(52):18848-53
  42. 42. Tsuji N, Nishikori S, Iwabe O, Matsumoto S, Shiraki K, Miyasaka H, et al. Comparative analysis of the two-step reaction catalyzed by prokaryotic and eukaryotic phytochelatin synthase by an ion-pair liquid chromatography assay. Planta. 2005;222(1):181-91
  43. 43. Gong JM, Lee DA, Schroeder JI. Long-distance root-to-shoot transport of phytochelatins and cadmium inArabidopsis. Proc Natl Acad Sci USA. 2003;100(17):10118-23
  44. 44. Estrella-Gómez N, Mendoza-Cózatl D, Moreno-Sánchez R, González-Mendoza D, Zapata-Pérez O, Martínez-Hernández A, et al. The Pb-hyperaccumulator aquatic fernSalvinia minimaBaker, responds to Pb2+ by increasing phytochelatins via changes inSmPCSexpression and in phytochelatin synthase activity. Aquat Toxicol. 2009;91(4):320-8
  45. 45. Tennstedt P, Peisker D, Böttcher C, Trampczynska A, Clemens S. Phytochelatin synthesis is essential for the detoxification of excess zinc and contributes significantly to the accumulation of zinc. Plant Physiol. 2009;149(2):938-48
  46. 46. Chen A, Komives EA, Schroeder JI. An Improved grafting technique for mature Arabidopsis plants demonstrates long-distance shoot-to-root transport of phytochelatins in Arabidopsis. Plant Physiol. 2006;141(1):108-20
  47. 47. Clemens S, Peršoh D. Multi-tasking phytochelatin synthases. Plant Sci. 2009;177(4):266-71
  48. 48. Stephan C. Evolution and function of phytochelatin synthases. J Plant Physiol. 2006;163(3):319-32
  49. 49. Clay NK, Adio AM, Denoux C, Jander G, Ausubel FM. Glucosinolate metabolites required for anArabidopsisinnate immune response. Science. 2009;323(5910):95-101
  50. 50. De Benedictis M, Brunetti C, Brauer EK, Andreucci A, Popescu SC, Commisso M, et al. TheArabidopsis thalianaknockout mutant forPhytochelatin Synthase1(cad1-3) is defective in callose deposition, bacterial pathogen defense and auxin content, but shows an increased stem lignification. Front Plant Sci. 2018;9(19)
  51. 51. Hématy K, Lim M, Cherk C, Piślewska-Bednarek M, Sanchez-Rodriguez C, Stein M, et al. Moonlighting function of Phytochelatin Synthase1 in extracellular defense against fungal pathogens. Plant Physiol. 2020;182(4):1920
  52. 52. Rea PA, Vatamaniuk OK, Rigden DJ. Weeds, worms, and more. Papain’s long-lost cousin, phytochelatin synthase. Plant Physiol. 2004;136(1):2463-74
  53. 53. Ruotolo R, Peracchi A, Bolchi A, Infusini G, Amoresano A, Ottonello S. Domain organization of phytochelatin synthase. J Biol Chem. 2004;279(15):14686-93
  54. 54. Vatamaniuk OK, Mari S, Lang A, Chalasani S, Demkiv LO, Rea PA. Phytochelatin synthase, a dipeptidyltransferase that undergoes multisite acylation with γ-glutamylcysteine during catalysis. J Biol Chem. 2004;279(21):22449-60
  55. 55. Romanyuk ND, Rigden DJ, Vatamaniuk OK, Lang A, Cahoon RE, Jez JM, et al. Mutagenic definition of a papain-like catalytic triad, sufficiency of the N-terminal domain for single-site core catalytic enzyme acylation, and C-terminal domain for augmentative metal activation of a eukaryotic phytochelatin synthase. Plant Physiol. 2006;141(3):858-69
  56. 56. Wang HC, Wu JS, Chia JC, Yang CC, Wu YJ, Juang RH. Phytochelatin synthase is regulated by protein phosphorylation at a threonine residue near its catalytic site. J Agric Food Chem. 2009;57(16):7348-55
  57. 57. Kühnlenz T, Hofmann C, Uraguchi S, Schmidt H, Schempp S, Weber M, et al. Phytochelatin synthesis promotes leaf Zn cccumulation ofArabidopsis thalianaplants grown in soil with adequate Zn supply and is essential for survival on Zn-contaminated soil. Plant Cell Physiol. 2016;57(11):2342-52
  58. 58. Uraguchi S, Sone Y, Ohta Y, Ohkama-Ohtsu N, Hofmann C, Hess N, et al. Identification of C-terminal regions inArabidopsis thalianaPhytochelatin Synthase 1 specifically involved in activation by arsenite. Plant and Cell Physiol. 2018;59(3):500-9
  59. 59. Pettersson O. Heavy-metal ion uptake by plants from nutrient solutions with metal ion, plant species and growth period variations. Plant and Soil. 1976;45(2):445-59
  60. 60. Ogawa S, Yoshidomi T, Yoshimura E. Cadmium(II)-stimulated enzyme activation ofArabidopsis thalianaphytochelatin synthase 1. J Inorg Biochem. 2011;105(1):111-7
  61. 61. Chia JC, Yang CC, Sui YT, Lin SY, Juang RH. Tentative identification of the second substrate binding site in Arabidopsis phytochelatin synthase. PLoS One. 2013;8(12):e82675
  62. 62. Cahoon RE, Lutke WK, Cameron JC, Chen S, Lee SG, Rivard RS, et al. Adaptive engineering of phytochelatin-based heavy metal tolerance. J Biol Chem. 2015;290(28):17321-30
  63. 63. Zayneb C, Imen RH, Walid K, Grubb CD, Bassem K, Franck V, et al. The phytochelatin synthase gene in date palm (Phoenix dactyliferaL.): Phylogeny, evolution and expression. Ecotoxicol Environ Saf. 2017;140:7-17
  64. 64. Kolahi M, Yazdi M, Goldson-Barnaby A, Tabandeh MR.In silicoprediction, phylogenetic and bioinformatic analysis ofSoPCSgene, survey of its protein characterization and gene expression in response to cadmium inSaccharum officinarum. Ecotoxicol Environ Saf. 2018;163:7-18
  65. 65. Filiz E, Saracoglu IA, Ozyigit II, Yalcin B. Comparative analyses of phytochelatin synthase (PCS) genes in higher plants. Biotechnol Biotechnol Equip. 2019;33(1):178-94
  66. 66. Moudouma C, Gloaguen V, Riou C, Forestier L, Saladin G. High concentration of cadmium inducesAtPCS2gene expression inArabidopsis thaliana(L.) Heynh ecotype Wassilewskija seedlings. Acta Physiol Plant. 2012;34(3):1083-91
  67. 67. Maier T, Yu C, Küllertz G, Clemens S. Localization and functional characterization of metal-binding sites in phytochelatin synthases. Planta. 2003;218(2):300-8
  68. 68. Vestergaard M, Matsumoto S, Nishikori S, Shiraki K, Hirata K, Takagi M. Chelation of cadmium ions by phytochelatin synthase: role of the Cystein-rich C-terminal. Anal Sci. 2008;24(2):277-81
  69. 69. Kulik A, Anielska-Mazur A, Bucholc M, Koen E, Szymańska K, Żmieńko A, et al. SNF1-related protein kinases type 2 are involved in plant responses to cadmium stress. Plant Physiol. 2012;160(2):868-83
  70. 70. Peterson AG, Oliver DJ. Leaf-targeted phytochelatin synthase inArabidopsis thaliana. Plant Physiol Biochem. 2006;44(11-12):885-92
  71. 71. Gasic K, Korban S. Transgenic Indian mustard (Brassica juncea) plants expressing anArabidopsisphytochelatin synthase (AtPCS1) exhibit enhanced As and Cd tolerance. Plant Mol Biol. 2007;64(4):361-9
  72. 72. Guo J, Dai X, Xu W, Ma M. OverexpressingGSH1andAsPCS1simultaneously increases the tolerance and accumulation of cadmium and arsenic inArabidopsis thaliana. Chemosphere. 2008;72(7):1020-6
  73. 73. Koźmińska A, Wiszniewska A, Hanus-Fajerska E, Muszyńska E. Recent strategies of increasing metal tolerance and phytoremediation potential using genetic transformation of plants. Plant Biotechnology Reports. 2018;12(1):1-14
  74. 74. Suman J, Uhlik O, Viktorova J, Macek T. Phytoextraction of heavy metals: A promising tool for clean-up of polluted environment? Front Plant Sci. 2018;9(1476)
  75. 75. Yan A, Wang Y, Tan SN, Mohd Yusof ML, Ghosh S, Chen Z. Phytoremediation: A promising approach for revegetation of heavy metal-polluted land. Front Plant Sci. 2020;11(359)
  76. 76. Török A, Gulyás Z, Szalai G, Kocsy G, Majdik C. Phytoremediation capacity of aquatic plants is associated with the degree of phytochelatin polymerization. J Hazard Mater. 2015;299:371-8
  77. 77. Pomponi M, Censi V, Girolamo V, Paolis A, Toppi L, Aromolo R, et al. Overexpression of Arabidopsis phytochelatin synthase in tobacco plants enhances Cd2+ tolerance and accumulation but not translocation to the shoot. Planta. 2006;223(2):180-90
  78. 78. Gasic K, Korban S. Expression of Arabidopsis phytochelatin synthase in Indian mustard (Brassica juncea) plants enhances tolerance for Cd and Zn. Planta. 2007;225(5):1277-85
  79. 79. Brunetti P, Zanella L, Proia A, De Paolis A, Falasca G, Altamura MM, et al. Cadmium tolerance and phytochelatin content ofArabidopsisseedlings over-expressing the phytochelatin synthase geneAtPCS1. J Exp Bot. 2011;62(15):5509-19
  80. 80. Zanella L, Fattorini L, Brunetti P, Roccotiello E, Cornara L, D’Angeli S, et al. Overexpression ofAtPCS1in tobacco increases arsenic and arsenic plus cadmium accumulation and detoxification. Planta. 2016;243(3):605-22
  81. 81. Wojas S, Clemens S, Hennig J, Skłodowska A, Kopera E, Schat H, et al. Overexpression of phytochelatin synthase in tobacco: distinctive effects ofAtPCS1andCePCSgenes on plant response to cadmium. J Exp Bot. 2008;59(8):2205-19
  82. 82. Wojas S, Clemens S, Skłodowska A, Antosiewicz DM. Arsenic response ofAtPCS1- andCePCS-expressing plants – effects of external As(V) concentration on As-accumulation pattern and NPT metabolism. J Plant Physiol. 2010;167(3):169-75
  83. 83. Lee BD, Hwang S. Tobacco phytochelatin synthase (NtPCS1) plays important roles in cadmium and arsenic tolerance and in early plant development in tobacco. Plant Biotechnol Rep. 2015;9(3):107-14
  84. 84. Zhang X, Rui H, Zhang F, Hu Z, Xia Y, Shen Z. Overexpression of a functionalVicia sativaPCS1 homolog increases cadmium tolerance and phytochelatins synthesis in Arabidopsis. Front Plant Sci. 2018;9(107)
  85. 85. Fan W, Guo Q, Liu C, Liu X, Zhang M, Long D, et al. Two mulberry phytochelatin synthase genes confer zinc/cadmium tolerance and accumulation in transgenicArabidopsisand tobacco. Gene. 2018;645:95-104
  86. 86. Shri M, Dave R, Diwedi S, Shukla D, Kesari R, Tripathi RD, et al. Heterologous expression ofCeratophyllum demersumphytochelatin synthase,CdPCS1, in rice leads to lower arsenic accumulation in grain. Sci Rep. 2014;4(1):5784
  87. 87. Schützendübel A, Polle A. Plant responses to abiotic stresses: heavy metal-induced oxidative stress and protection by mycorrhization. J Exp Bot. 2002;53(372):1351-65
  88. 88. Singh S, Parihar P, Singh R, Singh VP, Prasad SM. Heavy metal tolerance in plants: Role of transcriptomics, proteomics, metabolomics, and ionomics. Front Plant Sci. 2016;6(1143)
  89. 89. Mendoza-Cózatl DG, Moreno-Sánchez R. Control of glutathione and phytochelatin synthesis under cadmium stress. Pathway modeling for plants. J Theor Biol. 2006;238(4):919-36
  90. 90. Lee S, Moon JS, Ko TS, Petros D, Goldsbrough PB, Korban SS. Overexpression of Arabidopsis phytochelatin synthase paradoxically leads to hypersensitivity to cadmium stress. Plant Physiol. 2003;131(2):656-63
  91. 91. Kim JH, Lee S. Overexpression ofArabidopsisphytochelatin synthase (AtPCS1) does not change the maximum capacity for non-protein thiol production induced by Cadmium. J Plant Biol. 2007;50(2):4
  92. 92. Shukla D, Tiwari M, Tripathi RD, Nath P, Trivedi PK. Synthetic phytochelatins complement a phytochelatin-deficientArabidopsismutant and enhance the accumulation of heavy metal(loid)s. Biochem Biophys Res Commun. 2013;434(3):664-9
  93. 93. Wawrzyńska A, Wawrzyński A, Gaganidze D, Kopera E, Piatek K, Bal W, et al. Overexpression of genes involved in phytochelatin biosynthesis inEscherichia coli: effects on growth, cadmium accumulation and thiol level. Acta biochimica Polonica. 2005;52(1):109-16
  94. 94. Wawrzyński A, Kopera E, Wawrzyńska A, Kamińska J, Bal W, Sirko A. Effects of simultaneous expression of heterologous genes involved in phytochelatin biosynthesis on thiol content and cadmium accumulation in tobacco plants. J Exp Bot. 2006;57(10):2173-82
  95. 95. Oven M, Page JE, Zenk MH, Kutchan TM. Molecular characterization of the homo-phytochelatin synthase of soybeanGlycine max. J Biol Chem. 2002;277(7):4747-54
  96. 96. Dixon DP, Cummins I, Cole DJ, Edwards R. Glutathione-mediated detoxification systems in plants. Curr Opin Plant Biol. 1998;1(3):258-66
  97. 97. Del Buono D, Terzano R, Panfili I, Bartucca ML. Phytoremediation and detoxification of xenobiotics in plants: herbicide-safeners as a tool to improve plant efficiency in the remediation of polluted environments. A mini-review. Int J Phytoremediation. 2020;22(8):789-803
  98. 98. Fricker MD, May M, Meyer AJ, Sheard N, White NS. Measurement of glutathione levels in intact roots of Arabidopsis. J Microsc. 2000;198(3):162-73
  99. 99. Newton GL, Fahey RC. Determination of biothiols by bromobimane labeling and high-performance liquid chromatography. Method Enzymol. 1995;251:148-66
  100. 100. Brazier-Hicks M, Evans KM, Cunningham OD, Hodgson DRW, Steel PG, Edwards R. Catabolism of glutathione conjugates inArabidopsis thaliana: Role in metabolic reactivation of the herbicide safener fenclorim. J Biol Chem. 2008;283(30):21102-12
  101. 101. Printz B, Lutts S, Hausman J-F, Sergeant K. Copper trafficking in plants and its implication on cell wall dynamics. Front Plant Sci. 2016;7(601)
  102. 102. Alengebawy A, Abdelkhalek ST, Qureshi SR, Wang M-Q. Heavy metals and pesticides toxicity in agricultural soil and plants: Ecological risks and human health implications. Toxics. 2021;9(3):42
  103. 103. Uwizeyimana H, Wang M, Chen W, Khan K. The eco-toxic effects of pesticide and heavy metal mixtures towards earthworms in soil. Environ Toxicol Pharmacol. 2017;55:20-9
  104. 104. Zhang H, Yuan X, Xiong T, Wang H, Jiang L. Bioremediation of co-contaminated soil with heavy metals and pesticides: Influence factors, mechanisms and evaluation methods. Chem Eng J. 2020;398:125657
  105. 105. Srivastava V, Sarkar A, Singh S, Singh P, de Araujo ASF, Singh RP. Agroecological responses of heavy metal pollution with special emphasis on soil health and plant performances. Front Environ Sci. 2017;5(64)
  106. 106. Defarge N, Spiroux de Vendômois J, Séralini GE. Toxicity of formulants and heavy metals in glyphosate-based herbicides and other pesticides. Toxicol Rep. 2018;5:156-63
  107. 107. Kumar S, Trivedi PK. Glutathione S-Transferases: Role in combating abiotic stresses including arsenic detoxification in plants. Front Plant Sci. 2018;9(751)

Written By

Ju-Chen Chia

Submitted: June 20th, 2021 Reviewed: June 25th, 2021 Published: September 14th, 2021