Summary
During leaf development, plastids undergo dynamic changes in morphology. Chloroplasts develop from proplastids during leaf growth: this process includes synthesis, import, and maturation of numerous chloroplast proteins. During leaf senescence, chloroplasts change gradually into a senescing form termed gerontoplast, with the breakdown of thylakoid membranes and the degradation of photosynthetic proteins. In these developmental processes, it is apparent that the proteolytic activity within chloroplasts is a key to control such remarkable morphological/functional changes. Processing and maturation of chloroplast proteins are very important since chloroplast development requires numerous proteins that are imported from the cytosol. Various efforts to elucidate the functions of chloroplast proteases have revealed the existence of signal peptidases (SPP, PreP, TPP, and PlsP1) that are involved in the processing and the maturation steps. In addition, the quality control of proteins is necessary for proper chloroplast development. Recent studies using Arabidopsis mutants have identified several important chloroplastic proteases (Clp, FtsH, Deg, and some intramembrane-proteases), which originated from bacterial homologs, in the quality control of proteins during chloroplast development. In contrast, studies on the degradation of chloroplast proteins during senescence implied that multiple pathways, not limited to chloroplast proteases, control protein degradation in this process. In addition to protein degradation inside the chloroplasts, degradation of engulfed whole-chloroplasts within the vacuole, and small spherical bodies like senescence-associated vacuoles (SAV), and Rubisco-containing bodies (RCB) that include chloroplast stromal proteins are known to occur during leaf senescence. The latter implicates that autophagy plays an important role in delivering chloroplast proteins into the vacuole. This chapter provides an integrated summary on the roles of chloroplast proteases during chloroplast development, and the current view of the chloroplast protein degradation during senescence.
Access provided by Autonomous University of Puebla. Download chapter PDF
Similar content being viewed by others
Keywords
These keywords were added by machine and not by the authors. This process is experimental and the keywords may be updated as the learning algorithm improves.
I. Introduction
Along with protein synthesis, proteolysis is necessary for biological activities. Because, proteases are involved widely in various activities of living cells: they play important roles in proper protein maturation, quality control of proteins, and unnecessary protein degradation. In cellular organelles such as chloroplasts, proteases play crucial roles during change in the plants’ morphology and function dynamically in response to leaf developmental status and environmental signals. During leaf development, rapid differentiation of proplastids into chloroplasts occurs; during leaf senescence, chloroplasts change gradually into a senescing form designated as gerontoplasts (Mulisch and Krupinska, Chap. 14; Lichtenthaler, Chap. 15). These conversions of chloroplasts accompany dynamic changes in the composition of chloroplast proteins.
To date, more than 16 kinds of proteases have been identified in chloroplasts using various experimental and in silico approaches (Kato and Sakamoto 2010); the proteases that have been identified in Arabidopsis chloroplast are listed in Table 20.1. Chloroplasts are evolved from a cyanobacterial ancestor by a primary endosymbiotic event 1 billion years ago (Archibald 2009). It seems reasonable to consider that the vast majority of these proteases are homologs of known bacterial proteases. Mounting evidence indicates that many of these proteases are actually involved in the processing and maturation of polypeptides, and in the quality control of proteins during plastid differentiation and chloroplast homeostasis. In contrast, the participation of these proteases in degrading chloroplast proteins during leaf senescence is poorly understood. During leaf senescence, in addition to protein degradation inside chloroplasts, protein degradation in other organelles is known to occur. Results of recent studies imply that multiple degradation pathways of chloroplast proteins and their fine-tuning contribute to nutrient recycling, which is important for proper plant growth and possibly for reproduction as well. In this chapter, we first describe our knowledge of the chloroplast proteolytic machineries in leaf development, and subsequently we describe degradation mechanisms of chloroplast proteins in leaf senescence. For further background informations, we refer the readers to other recent reviews, some of which provide comprehensive information about plastid proteases and their physiological roles in chloroplast homeostasis (Adam 2000; Adam and Clarke 2002; Clarke et al. 2005; Richter et al. 2005; Adam et al. 2006; Sakamoto 2006; Kato and Sakamoto 2009, 2010; Chi et al. 2011; Olinares et al. 2011).
II. Plastid Protein Degradation During Leaf Development
During leaf development, proplastids are converted to mature chloroplasts in a light-dependent manner. Because chloroplast differentiation from proplastids occurs rapidly and dynamically, the synthesis and import of numerous proteins (see also Ling et al., Chap. 12) are necessary for this process. Concomitantly, synthesis of plastid-encoded proteins is activated. Finally the imported proteins from the cytosol and plastid-encoded proteins assemble into various protein complexes coordinately for the proper chloroplast function. Generation of abnormal peptides and proteins is unavoidable during these comprehensive protein dynamics. Therefore, quality control of proteins by proteases is a necessary feature of chloroplast maturation.
A. Proteases Involved in Protein Import
Proteins found in chloroplasts of mature leaves are encoded either by the chloroplast or by the nuclear genome. During differentiation of proplastids to chloroplasts, only a few chloroplast proteins are produced within the organelle; the larger share of chloroplast proteins are synthesized in the cytosol as precursors containing N-terminal transit sequences. These precursors are imported from the cytosol rapidly to developing chloroplasts through the general import machinery called the translocon at the outer envelope membrane of chloroplasts (TOC) and the translocon at the inner envelope membrane of chloroplasts (TIC) (Andres et al. 2010; Kovacs-Bogdan et al. 2010). Mutants lacking a component of the TOC/TIC protein import apparatus frequently show non-photosynthetic albino phenotypes, suggesting the necessity of protein transport into chloroplasts for chloroplast differentiation and plant viability (Andres et al. 2010; Kovacs-Bogdan et al. 2010). After import to the stromal space, their transit peptides are removed by stromal processing peptidase (SPP) (Richter et al. 2005). Originally, SPP was purified from pea as a member of soluble metalloprotease that contains an inverted zinc-binding motif HXXEH at the catalytic site (VanderVere et al. 1995). The cleavage of transit peptides by SPP proceeds in a two-step process. In the first step, SPP binds to the transit peptide of precursors and cleaves it from the mature form. In the second step, the transit peptide is further cleaved by SPP into subfragments and finally released from SPP (Richter et al. 2005). Studies using antisense SPP transgenic plants have elucidated the crucial role of SPP in chloroplast biogenesis. The SPP antisense transgenic tobacco plants display chlorosis and retardation of plant growth (Wan et al. 1998). Similarly, a large share of antisense transgenic plants in Arabidopsis cause seedling lethality (Zhong et al. 2003). Furthermore, the import capacity of precursors is markedly impaired in chloroplasts isolated from the antisense transgenic tobacco; N-terminal transit sequences fused to a reporter Green Fluorescent Protein (GFP) were not transported into chloroplasts but accumulated in the cytosol in these antisense transgenic plants (Zhong et al. 2003). These results verify experimentally that the loss of SPP function affects not only the removal of transit peptides in chloroplasts, but also a series of protein import mechanisms required for chloroplast development.
Subfragments of transit peptides released from imported precursor proteins are potentially toxic for the integrity of plastid membrane structures and its proper function. Evidence was provided to suggest that the presequence protease (PreP) is responsible for degrading the released subfragments (Ståhl et al. 2005). An ATP-independent metalloprotease, PreP, contains an inverted version of the common zinc-binding motif HXXEH; it has been identified initially as a protease involved in degrading mitochondrial presequences in potato (mitochondrial proteins imported from the cytosol also undergo maturation, and transit peptide sequences of these precursors are termed presequences) (Ståhl et al. 2002). Two homologs, AtPreP1 and AtPreP2, are found in the Arabidopsis genome. Both are dual-targeted to chloroplasts and mitochondria (Bhushan et al. 2003, 2005; Moberg et al. 2003). The unique chamber structure by two halves of this protease connected by a hinge region appears proper for the degradation of the peptide substrates because the chamber size is suitable to hold a small peptide and to exclude larger proteins (Fig. 20.1) (Johnson et al. 2006). Actually, PreP has the capacity to degrade the cleaved precursor peptides that are between 10 and 65 amino acid residues without substrate specificity (Ståhl et al. 2005). Nilsson Cederholm et al. (2009) showed that Arabidopsis double mutants lacking both PreP homologs have a pale green phenotype and retarded plant growth, and, this was due to the presence of aberrant chloroplasts and mitochondria. These observations strongly imply that proper degradation of the subfragments by chloroplast protease is necessary for normal leaf development.
Chloroplast development accompanies biogenesis of thylakoid membranes where photosynthetic light reaction and ATP synthesis occur. Similar to stromal proteins, many proteins in protein complexes of thylakoid membranes and luminal proteins are also synthesized in the cytosol and then transported to other sites. After being moved into the stromal space, proteins targeting the thylakoid lumen are further transported by either the chloroplast secretory (cpSec) or the chloroplast twin-arginine translocation (cpTat) pathway. The proteins that are localized in thylakoid membranes are inserted by the chloroplast signal recognition particle (cpSRP) or via the spontaneous pathway (Cline and Dabney-Smith 2008). To be localized in the thylakoid membrane, many thylakoid proteins have a bipartite transit peptide, which is constituted by a plastid transit peptide and a thylakoid-targeting signal peptide. Proteases functioning for the removal of the thylakoid-targeting signal peptide are called thylakoidal processing peptidases (TPP). Chaal et al. (1998) demonstrated that membrane-anchored serine-type proteases that belong to the type I signal peptidase (SPase I) family function as TPP. In the Arabidopsis genome, at least three SPase I homologs, plastidic type I signal peptidase (Plsp), exist. In Arabidopsis, Plsp3 was first identified as TPP based on in vitro signal peptidase activity assay (Chaal et al. 1998). Subsequently, Plsp1 has been regarded as a peptidase responsible for maturation of the component of the translocon at the plastid outer envelope membrane: Toc75 (Inoue et al. 2005). Further studies using plsp1 mutants revealed that Plsp1 also contributes to the processing of several thylakoid luminal proteins (subunits of the oxygen-evolving complex of PSII [OEC33 and OEC23], and plastocyanin) (Shipman and Inoue 2009). These results are consistent with the character of Plsp1 localized not only in the envelope membranes but also in the thylakoid membranes. To date, the in vitro signal peptidase activity of Plsp1 has not been confirmed, but Plsp1 is likely to function as a TPP in vivo. Meanwhile, the result that the lack of Plsp1 caused an abnormal plastid membrane structure and a seedling lethal phenotype suggests, similarity observed in case of SPP, that the the proper processing of thylakoid lumenal proteins is necessary for chloroplast development during leaf growth (Shipman-Roston et al. 2010). Together with studies in SPP and PreP, these observations clearly indicate that a series of protease activities in protein maturation is involved in the early process of chloroplast development.
B. Protein Quality Control During Leaf Development
In addition to the significance of proteases in the protein maturation steps as described above, proteases are well known to play a crucial role in the quality control of proteins in chloroplasts. Presuming that the occurrence of the abnormal proteins that are caused by protein misfolding increases coincidentally with large-scale protein synthesis that is required during chloroplast differentiation, the quality control of proteins is expected to become more important in this step. Actually, the loss of chloroplast proteases often severely impairs chloroplast biogenesis and its homeostasis. In this section, we describe the function of chloroplast proteases that are involved in quality control.
1. Protein Quality Control in Stroma
a. Clp Protease
To date, several proteases have been identified in the chloroplast stroma (Kato and Sakamoto 2010). Among these stromal-localized proteases, Clp is considered to play a central role in quality control as a stromal housekeeping protease (Clarke et al. 2005). Actually, Clp protease is an ATP-dependent serine-type protease complex that is present in almost all bacteria and in mitochondria and chloroplasts (Porankiewicz et al. 1999; Yu and Houry 2007). The functional Clp is constituted of a chaperone that belongs to AAA + ATPases and a proteolytic core component. In E. coli, the chaperone components comprise a homogeneous hexameric ring of the Clp/Hsp100 subunits, either ClpA or ClpX containing two and one AAA domains, respectively (Grimaud et al. 1998). The central proteolytic core of the Clp protease in E. coli comprises two stacked homogeneous heptameric rings of seven identical ClpP with serine-type proteolytic active sites (Fig. 20.2). These heptameric rings form a barrel-like structure enclosing a large chamber containing exposed proteolytic sites (Wang et al. 1997). The chaperone component docks on one or both ends of the barrel-like core component (Kessel et al. 1995; Grimaud et al. 1998). The connected chaperone components recognize denatured protein substrates; then they unfold and translocate the substrates through the narrow axial pore into the proteolytic chamber. Moreover, a small adapter protein, ClpS, is associated with the Clp chaperone component to prevent accidental degradation of functional proteins (Erbse et al. 2006; Wang et al. 2008). These structural features of the Clp protease complex indicate that the Clp complex employs common principles with the 26S proteasome proteolytic machinery in eukaryotes because both Clp and 26S proteasome use the unfolding-coupled processive protein degradation system. Consequently, Clp protease complexes are regarded as the counterparts of eukaryotic proteasomes.
The ClpP subunits are diversified and exist as multiple copies in photosynthetic organisms, in contrast to most bacteria containing a single copy of the proteolytic subunit. In chloroplasts, the proteolytic chamber is present as a heterocomplex; the proteolytic core comprises five ClpP isomers (ClpP1 and ClpP3–P6) and four ClpP-like subunits (ClpR1–ClpR4) that lack the conserved amino acid of the catalytic triad (Peltier et al. 2001, 2004; Clarke et al. 2005; Sjögren et al. 2006). In cyanobacteria, Andersson et al. (2009) have demonstrated that ClpR is indeed proteolytically inactive. Compared with the complexity and the diversity of the proteolytic chamber subunits, the subunits of the chaperone component in chloroplasts are rather simple. Among the four homologs of Clp/Hsp100 subunits (ClpB3, ClpC1, C2, and ClpD) that are localized in chloroplasts (Moore and Keegstra 1993; Weaver et al. 1999; Peltier et al. 2004) with two distinct AAA + domains, three (ClpC1, C2 and ClpD) seem to form a complex with a proteolytic chamber (Peltier et al. 2004). In addition, a homolog of an adapter protein ClpS has been discovered in chloroplast Clp complexes. Along with these subunits, two novel plant-specific subunits, ClpT1 and ClpT2, which share homology with the N-terminal domain of Clp/Hsp100 proteins, have been identified (Peltier et al. 2001, 2004). Further studies showed that the peripheral attachment of ClpT proteins to the proteolytic core components is likely to regulate the assembly of Clp protease complex (Sjögren and Clarke 2011).
The physiological importance of the Clp protease was initially demonstrated by studies showing that tobacco transgenic lines with significantly reduced levels of ClpC or ClpP1 could not survive (Shanklin et al. 1995; Shikanai et al. 2001). Additional studies using Arabidopsis mutants and antisense lines supported the results of early studies and revealed the indispensable function of the Clp protease (Rudella et al. 2006; Sjögren et al. 2006; Kim et al. 2009; Stanne et al. 2009; Zybailov et al. 2009). Knockout mutants showed that the defect of the ClpP subunit in protease complexes engenders a lethal phenotype in Arabidopsis. Therefore, the antisense strategy was employed for additional analysis of ClpP. The ClpP4 and P6 antisense plants showed leaf chlorosis and slow growth (Sjögren et al. 2006; Zheng et al. 2006). In particular, the phenotypes of mutants are severe in younger inner leaves. This impairment of chloroplast development by repression of Clp suggests a functional importance of Clp in the early phase of plastid differentiation. Of the clpr mutants, the clpr1 null mutant can survive because the ClpR1 function is partially complemented by the closely related ClpR3 protein (Koussevitzky et al. 2007; Kim et al. 2009; Stanne et al. 2009). The loss of ClpR1 brings about leaf chlorosis and reduces photosynthesis rates; further, the more severe phenotype of the clpr1 mutant in the younger leaves suggests the involvement of Clp function in chloroplast development. The proteomic analysis using isolated chloroplasts from ClpP6 antisense and clpr1 mutant revealed some potential substrates for Clp protease, which are involved in general homeostatic roles such as protein synthesis, protein maturation, and RNA maturation (Sjögren et al. 2006; Stanne et al. 2009). Furthermore, large-scale comparative proteomics, using the null-mutant clpr4 shows albino phenotype, that cannot survive beyond the seedling stage, but is able to grow under heterotrophic conditions, demonstrated that many chloroplast proteins had changed in the clpr4 mutant (Kim et al. 2009). Especially, the nearly complete loss of photosynthetic proteins in the mutant is thought to be the reason for the severe phenotype in clpr4. Similarly, the large-scale comparative proteomics of the clpr2 knockdown mutant and the wild-type showed that impaired protease activities are involved widely in various chloroplast protein accumulation including the methylerythritol phosphate (MEP) pathway proteins, which have been implicated in other reports as substrates of Clp protease (Zybailov et al. 2009). In addition, the loss of function of chaperone component subunit ClpC1 causes growth retardation and leaf chlorosis with reduced photosynthesis proteins (Constan et al. 2004; Sjögren et al. 2004; Kovacheva et al. 2005). Moreover, the lack of both ClpC1 and ClpC2 causes very early embryo lethality (Kovacheva et al. 2007). These results suggest important roles of the unfolding function of the Clp protease complex for plastid development and plant viability. Collectively, the studies of the Clp protease indicate that the derangement of protein degradation resulting from impairment of Clp causes the disruption of chloroplast development with disintegration of protein homeostasis.
b. Protein Degradation and Chaperones
We note that the loss of Clp subunits, not only Clp/Hsp100 subunits that are likely to function as a chaperone independently, but also Clp protease core subunits, causes accumulation of molecular chaperones (unfoldase ClpB3, chloroplast Hsp90, Hsp70, Cpn60 and so on) (Kim et al. 2009; Stanne et al. 2009; Zybailov et al. 2009). The mole-cular chaperones help in proper protein folding to prevent the generation of harmful polypeptides and aggregation of proteins. Apparently, the higher level of molecular chaperones results from the increased protein instability, which appears to be associated with the accumulation of undegraded harmful polypeptides in clp mutants. Therefore, the increased level of chaperones in clp mutants suggest the presence of a close relation between protein degradation and the folding for protein quality control in chloroplast protein synthesis and protein transport from the cytosol. To date, many research groups have identified molecular chaperones in chloroplasts; many reviews describe their functions (Jackson-Constan et al. 2001; Levy-Rimler et al. 2002; Weiss et al. 2009). Here, we briefly explain their roles and involvement in chloroplast development.
One chloroplast Clp/Hsp100 subunit, ClpB3, seems to function as a chaperone independently of Clp protease complexes because it lacks the conserved domain for binding to ClpP (Clarke et al. 2005). The mutant of ClpB3 is reported as one of the albino or pale-green (apg) mutants, apg6, and it shows severe defects in chloroplast development (Myouga et al. 2006; Lee et al. 2007). Further, ClpC1 and ClpC2, also known as Hsp93-V and Hsp93-III, have been identified as proteins associated with the chloroplast protein import apparatus (Akita et al. 1997; Nielsen et al. 1997). Because a large proportion of ClpC is present in the stroma in a soluble form, the primary function of ClpC is thought to serve as the chaperone component of the Clp protease complexes; however, a role as an independent chaperone in chloroplast protein import also seems feasible. Another Hsp protein, chloroplast Hsp90, was originally identified through a chlorate-resistant mutant that shows an altered response to red light (Cao et al. 2003). The mutant of chloroplast Hsp90 also shows delayed chloroplast development, suggesting the involvement of chloroplast Hsp90 in the maturation of newly imported or synthesized proteins during chloroplast development (Cao et al. 2003). Regarding Hsp70 homologs, four Hsp70 systems have been detected within the different compartments of chloroplasts (Jackson-Constan et al. 2001). Two of them, Com70 and IAP70, both localized in the envelope membrane, are apparently involved in protein import to chloroplasts (Schnell et al. 1994; Kourtz and Ko 1997). The other two Hsp70, cpHsc70-1 and cpHsc70-2, which have been shown to accumulate in clp mutants, are apparently present in stroma (Su and Li 2008). An Arabidopsis T-DNA insertion mutant of cpHsc70-1 shows variegated cotyledons and malformed leaves, although a T-DNA mutant of cpHsc70-2 shows no visible phenotype (Su and Li 2008). Furthermore, attempts to obtain a double mutant and the approach of co-suppression of both genes using RNAi interference showed their redundant functions and their important role in chloroplast development and plant viability (Latijnhouwers et al. 2010). In addition to these homologs, the homologs of the bacterial chaperone GroEL, Cpn60s, are reported to be proteins that accumulate in clp mutants. Similar to Hsp70s, Cpn60, which interacts with a component of the inner membrane import apparatus Tic110, helps the imported protein to fold into its native conformation (Kessler and Blobel 1996). The results demonstrating that the cpn60 mutants show abnormal development of embryos suggest the necessity of Cpn60 for plastid biogenesis and plant viability (Apuya et al. 2001). In addition to these typical molecular chaperones, the chaperone activity of Deg protease was recently reported as described below.
2. Protein Quality Control in Membranes
a. FtsH Protease
The quality control of membrane proteins is necessary for chloroplast biogenesis, especially in the formation of thylakoid membranes. Of the membrane proteases, FtsH protease is the best characterized one because the unique variegated phenotype of the ftsh mutants has been the subject of interest of many studies. FtsH protease is a membrane-bound ATP-dependent metalloprotease that was originally identified in E. coli as a necessary protein for growth (Tomoyasu et al. 1993). FtsH is a large complex that has a AAA + ATPases domain and a proteolytic core component (Krzywda et al. 2002; Niwa et al. 2002); however, in contrast to the Clp protease complex, it has both domains on the same polypeptide chain (Fig. 20.2). Crystal structure studies have revealed that six identical FtsH subunits form a large complex with unique catalytic site(s) located at the peripheral region of the hexamer ring (Bieniossek et al. 2006; Suno et al. 2006).
We note that FtsH is highly conserved in all organisms. In plants, FtsH homologs have been isolated and characterized from, e.g., spinach, tobacco and peas (Lindahl et al. 1996; Seo et al. 2000; Yue et al. 2010). In Arabidopsis, among the enumerated 12 homologous genes, 9 homologs (FtsH1, 2, 5, 6, 7, 8, 9, 11, and 12) are located in the chloroplast (Sakamoto et al. 2003). Of these homologs, FtsH1, 2, 5, and 8 are identified by immunoblot and proteomic analyses of the isolated thylakoid membrane (Sakamoto et al. 2003; Friso et al. 2004; Sinvany-Villalobo et al. 2004; Yu et al. 2004). Immunoblot analysis showed that the proteolytic domain faces the stroma side of the membrane (Lindahl et al. 1996; Sakamoto et al. 2003). The four isomers, mentioned above, have been regarded as major isomers of chloroplast FtsH complexes. They are divided into closely related pairs of two types, FtsH1 and FtsH5 (type A), FtsH2 and FtsH8 (type B), which are likely duplicated (Sakamoto et al. 2003). Among them, FtsH2 is the most abundant isomer, followed by FtsH5, FtsH8, and FtsH1. Originally, FtsH2 and FtsH5 were reported as responsible genes of leaf-variegated mutants, which have long been known in Arabidopsis (Chen et al. 2000; Takechi et al. 2000; Sakamoto et al. 2002). The mutants of FtsH2 and FtsH5 are called yellow variegated 2 (var2) and var1; var2 shows severe variegated phenotype and var1 shows weak leaf-variegation. On the other hand, mutants with a loss of FtsH1 and FtsH8 show no visible change in their phenotype. The difference in the degree of leaf-variegation among these mutants is considered to be dependent on the abundance of isomers in the FtsH heterocomplexes. The variegated phenotypes in var1 and var2 mutants are rescued, respectively, by overexpression of FtsH1 and FtsH8; this suggests functional redundancy of each type A and type B FtsH isomers (Yu et al. 2004, 2005). Furthermore, the results that ftsh2 ftsh8 and ftsh1 ftsh5 double mutants showing an albino-like phenotype underscore the possibility that the existence of both type A and type B isomers is required for the proper function of FtsH (Zaltsman et al. 2005b). Together with the studies by proteomics and the biochemical approaches, the construction of heterohexameric FtsH complex by type A and type B isomers in chloroplasts has been published.
Additionally, the observations that overall FtsH levels correlate with the degree of white sectors in leaves led to the proposal of a threshold model of leaf variegation; subthreshold amounts of the FtsH complex block thylakoid formation in leaf development, leading to the failure of chloroplast development (Yu et al. 2004). In this threshold model, it was expected that FtsH would have a decisive role at a particular stage of chloroplast development. The result that white viable sectors of var2 mutants have undifferentiated plastids, and the observations that the variegated pattern is irreversible once developed, supports this expectation (Zaltsman et al. 2005a; Kato et al. 2007). Furthermore, recent careful observation of plastid ultrastructures during the early stage of leaf development demonstrated that the abnormal plastids in white sectors is formed as a result of the arrest of chloroplast development at its initial steps (Sakamoto et al. 2009). To summarize, these results demonstrate that the early stage of chloroplast development requires sufficient levels of FtsH for thylakoid formation.
Further studies have shown that several genetic defects cause the suppression of leaf-variegation. Most identified mutant genes are involved in the chloroplast translation (chloroplast rRNA processing and protein synthesis), which implies that the delay in chloroplast development, which results from the impairment of chloroplast translation, lowers the requirement of FtsH for protein quality control in chloroplast biogenesis (Park and Rodermel 2004; Miura et al. 2007; Yu et al. 2008; Liu et al. 2010). Electron-microscopic observations of plastids revealed that the loss of FtsH in var2 mutant causes slow progression of chloroplast development in the prospective green sectors (Sakamoto et al. 2009). In other words, the variegated mutant seems to avoid the serious dysfunction of chloroplasts by limiting the progression of chloroplast differentiation in early leaf development. Taken together, these results indicate that the balance between the speed of thylakoid development and the protein quality control by FtsH is an important point for proper chloroplast development and that it is regulated strictly by communication between the nucleus and the chloroplasts.
Using transgenic plants that ectopically expressed a proteolytically inactive FtsH2, Zhang et al. (2010) posed an interesting question for the FtsH function in leaf variegation; the result that expression of proteolytically inactive FtsH2 rescued not only leaf variegation in var2, but also seedling lethality in ftsh2 ftsh8 double mutant suggests that not all proteolytic activities of FtsH heterocomplexes are necessary for their function in chloroplasts (Zhang et al. 2010). Further analysis of var1 var2 mutants, with expression of proteolytically inactive FtsH2, and a study using an inducible FtsH2, show that the overall amount of FtsH complexes predominantly determines the threshold of chloroplast development when the protease activity is excessive (Zhang et al. 2010).
What is the substrate of FtsH in chloroplast development? Using mature chloroplasts, several studies suggest only a partial answer to this question. In vitro studies showed the involvement of FtsH in the degradation of unassembled Rieske Fe-S protein and in the degradation fragment of the PSII reaction center D1 protein (Ostersetzer and Adam 1997; Lindahl et al. 2000). Additional in vivo analyses using mutants lacking FtsH2 or FtsH5 also indicated the involvement of FtsH in D1 degradation (Bailey et al. 2002; Kato et al. 2009). Most of the available evidence point to the central role of FtsH in D1 degradation in the PSII repair cycle in mature chloroplasts. However, the study of the substrates of FtsH in the chloroplast developmental stage has scarcely been made. Consequently, although D1 protein might be a possible substrate in developing thylakoids as well as that in mature chloroplasts, the substrates of FtsH in the chloroplast developmental stage remain largely unknown.
b. Deg Protease
DegP protease is an ATP-independent serine type protease that was originally identified in E. coli as the protease necessary for survival at high temperatures (Skorko-Glonek et al. 1995). It has two domains: the proteolytic domain at the N-terminus and the PDZ domain(s), which are involved in protein–protein interactions, at the C-terminus (Clausen et al. 2002). It is noteworthy that DegP has not only a proteolytic activity, but also a chaperone activity to prevent the accumulation of abnormal proteins (Spiess et al. 1999). The switch between protease and chaperone function seems be regulated by a conformation change of the protein caused by a temperature shift. The chaperone activity is predominant at low temperatures; protease activity is increased at elevated temperatures (Spiess et al. 1999). In Arabidopsis, among the 16 DegP homologous genes, five homologs (Deg1, 2, 5, 7, and 8) have already been found in the chloroplast (Itzhaki et al. 1998; Haussühl et al. 2001; Peltier et al. 2002; Schubert et al. 2002; Huesgen et al. 2005; Sun et al. 2007, 2010a). Furthermore, the presence of Deg11 in the chloroplast stroma has also been suggested (L. Zhang and X. Sun, personal communication, 2011). These homologs are generally peripherally attached to the stromal (Deg2 and 7) or the lumenal sides (Deg1, 5, and 8) of thylakoid membranes. In E. coli DegP peripherally attaches to the plasma membrane. Early in vitro studies using recombinant proteins showed that Deg1 proteases are involved in the degradation of several thylakoid lumen proteins, such as plastocyanin and OEC33 (Chassin et al. 2002), and Deg2 functions in the initial endoproteolytic cleavage of the D1 protein (Haussühl et al. 2001), although the in vivo contributions of these Deg proteases to the degradation of these proteins remain unconfirmed (Huesgen et al. 2006). Meanwhile, there is evidence that several Deg proteases (Deg1, 5, 7, and 8) play an important role in the in vivo PSII repair under high-light conditions (Sun et al. 2007, 2010a, b). The work of Kapri-Pardes et al. (2007) suggests the importance of Deg protease for plant viability since the authors failed to obtain homozygous knockout lines of Deg1. Furthermore, antisense lines with a reduced level of the Deg1 protein showed pale-green phenotypes, suggesting the requirement of Deg1 for chloroplast biogenesis and homeostasis (Kapri-Pardes et al. 2007). It is particularly interesting that Sun et al. (2010b) show the existence of chaperone activity of Deg1, like it is known for E. coli homolog DegP. However, the functions of Deg1 in chloroplast development are largely unknown, although the chaperone activity of Deg1 seems to be very important for proper protein assembly that is needed in thylakoid development.
c. Intramembrane Proteases
Chloroplasts have several intramembrane proteases to degrade membrane proteins for proper chloroplast biogenesis. Of these intramembrane proteases, the loss of the homologs of the sterol-regulatory element binding protein site 2 protease (SREBP S2P protease) causes the impairment of chloroplast biogenesis. One homolog of SREBP S2P proteases, ethylene-dependent gravitopism-deficient and yellow-green 1 (EGY1), is an ATP-independent metalloprotease with eight putative transmembrane helices in its C-terminus (Chen et al. 2005). The egy1 mutant was originally identified as a mutant that shows abnormal gravicurvature in hypocotyls and a pale-yellow phenotype. The development of the thylakoid membrane system is severely impaired in the mutants. In particular, the remarkable decrease of the levels of the chlorophyll-binding proteins in the egy1 mutants seems to cause the loss of grana stacks because it is considered that the LHCII-mediated physical connection contributes to the stability of grana stacking (Chen et al. 2005). The association of EGY1 with chloroplast membranes has been confirmed by immunoblotting analysis, but the detailed localization of EGY1 in chloroplasts has not yet been identified. However, another homolog of the SREBP S2P proteases, AraSP, is localized in the chloroplast inner envelope membrane (Bölter et al. 2006). The deduced amino acid sequence of AraSP indicates 4–5 transmembrane helices and a conserved catalytic motif, which is localized between the first two helices. The T-DNA knockout mutant of AraSP cannot germinate and the heterozygous T-DNA insertion mutant still shows severely impaired plant growth (Bölter et al. 2006). Together with the defective phenotype of chloroplast biogenesis in the AraSP antisense lines, these results underscore the important role of AraSP during leaf development (Bölter et al. 2006).
III. Plastid Protein Degradation During Leaf Senescence
In response to organ developmental status and various environmental signals, chloroplasts change their morphology and convert the plastid type from one form to another. This happens also in the final stage of leaf development, when photosynthesis is no longer required, but senescence is initiated. Chloroplasts in senescing leaves gradually shrink and transform themselves into gerontoplasts (Wise 2007). Breakdown of thylakoid membranes, degradation of photosynthetic proteins, and accumulation of a remarkable number of plastglobuli occur during leaf senescence (Krupinska 2007). Although the chloroplast-to-gerontoplast transition occurs in senescing leaves, it is an extremely important event for plant growth because the chloroplast nutrients that are generated by degradation of accumulated proteins during leaf senescence contribute to crop yields and biomass accumulation (Mae 2004). Despite numerous studies on the degradation of chloroplast proteins and the change of chloroplast structure during senescence, the fate of chloroplasts and the degradation mechanism of chloroplast proteins during senescence remain poorly understood. In the following sections, degradation processes of chloroplast proteins mediated by the proteases are summarized. For additional information, we refer the readers to several reviews on chloroplast component degradation during leaf senescence (Hortensteiner and Feller 2002; Feller et al. 2008; Gregersen et al. 2008; Martinez et al. 2008b).
A. Degradation of Stromal Proteins
Available results suggest that different mechanisms exist for chloroplast protein degradation during leaf senescence (Minamikawa et al. 2001; Chiba et al. 2003; Kato et al. 2004; Otegui et al. 2005). Chloroplast protein degradation mechanisms may be divided broadly into two categories: the degradation of proteins inside the chloroplasts and the degradation of chloroplast proteins in other organelles such as lytic vacuoles (see also Wada and Ishida, Chap. 19). Chloroplast protein degradation pathways that interact with other organelles can be divided further into at least three categories: degradation of chloroplast proteins via chloroplast-derived vesicles, the degradation of engulfed whole-chloroplasts within the vacuole, and the degradation of chloroplasts as a result of tonoplast rupture. It is particularly interesting that studies of Arabidopsis mutants show multiple degradation pathways of chloroplast stromal proteins and their fine-tuning (Hortensteiner and Feller 2002; Feller et al. 2008; Gregersen et al. 2008; Martinez et al. 2008b). We provide below an overview of stromal protein degradation.
1. Protein Degradation Inside Plastids
The idea that proteins are degraded inside chloroplasts is supported by the finding that the protein level decreases rapidly in the early phase of leaf senescence prior to the decline of the chloroplast number (Friedrich and Huffaker 1980; Mae et al. 1984). In particular, stromal enzymes, known to be involved in carbon and nitrogen assimilation, such as glutamine synthetase and ribulose 1, 5-bisphosphate carboxylase-oxygenase (Rubisco), are lost in the early phases of leaf senescence. During this process, soluble proteins are gradually degraded as leaves age; then degraded products are exported to reproductive organs to salvage nutrients. Furthermore, experiments using isolated chloroplasts, which exclude contamination of proteases derived from other cellular components, showed that hydrolysis of Rubisco takes place inside the isolated organelles (Ragster and Chrispeels 1981; Mitsuhashi and Feller 1992).
Although the importance of proteolysis inside chloroplasts has been recognized, plastid proteases involved in protein degradation in senescent leaves remain poorly understood. Early biochemical approaches for the identification of plastid proteases, involved in degradation of Rubisco, suggest that a stromal metalloprotease, that has been partially purified from pea chloroplasts, is able to degrade the large subunit of isolated Rubisco to smaller polypeptides in vitro (Bushnell et al. 1993). A further study using isolated chloroplasts also showed that metalloprotease activities are involved in stromal protein degradation under dark or nitrogen-starvation conditions (Roulin and Feller 1998). However, the metalloprotease that actually functions in chloroplast protein degradation in vivo during leaf senescence remains unidentified.
Various proteases localized in chloroplasts are known to participate in proper organellar functioning through protein quality control. Of these chloroplast proteases, Clp and Lon are considered to participate in protein degradation in the stroma, and FtsH and Deg are known to be involved in protein degradation in thylakoid membranes (Kato and Sakamoto 2010). Of these proteases, one Clp chaperone subunit, ClpD, was first reported to show early response to dehydration (ERDs) at the mRNA level (Kiyosue et al. 1993); ClpD/ERD corresponds to SAG15 (senescence-associated gene 15), whose transcripts have been known to accumulate during leaf senescence (Nakashima et al. 1997). Although several research groups have reported up-regulation of the mRNA levels of clpD during leaf senescence, the ClpD protein does not show any significant accumulation; instead, it declines during senescence (Nakabayashi et al. 1999; Weaver et al. 1999). In spite of up-regulation of genes corresponding to several other subunits of the Clp protease core complex (ClpP3 and ClpP5) has been reported, ClpP protein levels remained almost constant or declined during leaf senescence (Nakabayashi et al. 1999). Consequently, further research is necessary to examine if Clp participates in the degradation of stromal proteins during leaf senescence.
It is noteworthy that the aspartic protease CND41 has been localized in plastids and shown to be up-regulated in natural leaf senescence (Kato et al. 2004). In contrast to Clp, its up-regulation has been detected at both transcriptional and protein levels. This CND41 was originally isolated from chloroplast nucleoids, a large complex of chloroplast DNA and proteins in photomixotrophically cultured tobacco cells (Nakano et al. 1997). Unlike many other major chloroplastic proteases, CND41 that belongs to A1 aspartic protease family (pepsin-like family), appears to be of eukaryotic origin. Studies on the proteolytic activity of CND41, that had been purified from cultured tobacco cells, showed that CND41 can degrade denatured inactive Rubisco at physiological pH (Murakami et al. 2000). However, native active Rubisco appeared to be a poor substrate for it. Furthermore, characterization of transgenic tobacco lines over-expressing CND41 implied that there is a post-translational activation mechanism for CND41 to degrade chloroplast proteins during leaf senescence in vivo (Kato et al. 2005). Aside from tobacco, up-regulation of CND41 homologs during senescence has been observed in Arabidopsis and barley (Parrott et al. 2007; Diaz et al. 2008). It is particularly interesting that immunoblot analysis of Arabidopsis recombinant inbred lines, which were selected based on the differential leaf senescence phenotypes, revealed that the CND41 homolog appeared to accumulate in early senescing Arabidopsis lines, suggesting that the CND41 homolog is associated with senescence (Diaz et al. 2008). These results imply that CND41 contributes to protein degradation inside chloroplasts during leaf senescence in many plant species.
2. Protein Degradation in Other Organelles
The chloroplast number per cell decreases during leaf senescence (Ono et al. 1995; Inada et al. 1998; see also Mulisch and Krupinska, Chap. 14). This decrease was suggested to indicate the presence of a whole chloroplast degradation system, possibly conducted by other organelles. Furthermore studies revealed the presence of small spherical bodies containing chloroplast stromal proteins during leaf senescence (Chiba et al. 2003; Martinez et al. 2008a). We summarize below the degradation pathways of chloroplast proteins via chloroplast-derived vesicles and the degradation of engulfed whole-chloroplasts within the vacuole (see also Wada and Ishida, Chap. 19). These degradation pathways participate in leaf senescence, although chloroplast protein degradation after tonoplast rupture seems to occur mainly during programmed cell death.
a. Rubisco-Containing Bodies
Immunocytochemical detection of Rubisco in naturally senescing wheat leaves showed the existence of distinct small spherical bodies, termed Rubisco-containing bodies (RCBs), in the cytoplasm and in the vacuole (Chiba et al. 2003). In fact, RCB-like structures have been observed in senescent leaves of tobacco (Prins et al. 2008). They also contain another stromal protein, glutamine synthetase, but do not include thylakoid membrane proteins and chlorophylls. The RCBs are 0.4–1.2 μm in diameter and are surrounded by double membranes. Careful observation of RCBs revealed that they are further surrounded by the other membrane structures, suggesting that an autophagy mechanism is involved in degrading chloroplast proteins (Chiba et al. 2003). Arabidopsis mutants that are defective in autophagy-related genes (atg mutant) were recently examined for the relevance of autophagy for RCB formation (Ishida et al. 2008). The analysis of visualized RCBs using GFP-labeled Rubisco shows that RCBs are not observed in leaves of atg mutant, although RCBs are observed in the lumen of the vacuoles in the wild-type. Furthermore, characterization of a GFP-linked ATG protein as an autophagy marker demonstrated that the GFP signals are co-localized in autophagic bodies with chloroplast stroma-targeted DsRed. These results show that transfer of stromal proteins to the central vacuole via RCBs pathway requires ATG-dependent autophagy. Another study using an atg mutant showed that the size of chloroplasts did not decrease in the atg mutant during leaf senescence, suggesting that ATG-dependent autophagy mediated degradation of chloroplast proteins is responsible for chloroplast shrinkage in the senescent stage (Wada et al. 2009). It is particularly interesting that the defect in the generation of RCBs in the atg mutant induced the increase of stromules as compared to the stromules in the wild-type (Ishida et al. 2008). The release of small vesicles from the ends of stromules has been observed, and the vesicle diameter is similar to that of RCBs (Gunning 2005). These observations imply the possible association between the release of small bodies from stromules and RCBs.
b. Senescence-Associated Vacuoles
Senescence-associated vacuoles (SAVs) are another type of vesicles that were originally identified in the senescent leaves of soybean and Arabidopsis using the SAG12-GFP fusion protein as a fluorescent marker (Otegui et al. 2005; see also Costa et al., Chap. 18). Distinguishable from the central vacuole with respect to their acidic pH, SAVs have intense proteolytic activity. A typical SAV is approximately 0.7 μm in diameter. In addition, the senescence specific cysteine protease SAG12 is localized selectively within SAVs. Despite the strong relationship of SAG12 and senescence, however, the Arabidopsis sag12 mutant lacking SAG12 shows no altered senescence phenotypes and has SAVs, indicating that SAG12 is not directly required for SAV formation (Otegui et al. 2005). Direct evidence of the involvement of SAVs in chloroplast protein degradation was obtained by using tobacco transformants expressing chloroplast-targeted GFP (Martinez et al. 2008a). During leaf senescence, GFP that is targeted to the chloroplast stroma was relocalized to SAVs. Furthermore, apart from GFP, Rubisco and glutamine synthetase are contained in isolated SAVs and are degraded within SAVs. Although the D1 protein of the photosystem II reaction center and the light-harvesting complex II (LHC-II) are not contained in SAVs, some SAVs with chlorophyll autofluorescence have been detected (Martinez et al. 2008a). The SAVs are known to be surrounded by a single membrane in contrast to RCBs that have double membranes, but there are several known similarities between RCBs and SAVs. Although the possible relation between these two types of vesicles is currently unknown, SAVs appear to be formed in atg7 (Otegui et al. 2005), which is defective in the ATG-gene-dependent autophagy and the formation of RCB. The selectivity of proteins that are carried in these compartments as substrates, is still an unanswered question.
c. Degradation Inside the Central Vacuole
In addition to the above-mentioned specific vesicles associated with leaf senescence, the central vacuole, the largest lytic compartment in mature cells, is an important compartment related to chloroplast degradation. An early study using electron microscopy showed the possible physical interaction between the outer envelope of the chloroplast and the tonoplast (Peoples et al. 1980); in this report, the outer envelope of some chloroplasts flanked by the tonoplast was apparently degraded and merged with the tonoplast, but the inner envelope of the chloroplasts appeared to remain intact. However, another ultrastructural study showed that some chloroplasts observed in mesophyll cells appeared to move toward the center of the cell as leaf senescence proceeded (Wittenbach et al. 1982). This movement was concomitant with the decrease of chlorophylls and soluble proteins and the decline of chloroplast number per cell, suggesting degradation of engulfed whole-chloroplasts within the vacuole. These observations have been supported by an electron microscopic examination of dark-induced senescence of French bean leaves (Minamikawa et al. 2001). Electron microscopic observations indicates chloroplast internalization into vacuoles, and the disruption of the outer membranes of chloroplasts in vacuoles. In this study, the possible involvement of vacuolar cysteine proteases in degradation of chloroplast proteins was suggested. Although the debate about the degradation of proteins in vacuoles and the uptake of chloroplasts by vacuoles under natural leaf senescence continues, it seems that the degradation of whole chloroplasts inside vacuoles is a key step for chloroplast protein degradation. Apparently, the question arises of how chloroplasts are transferred into vacuoles. Wada et al. (2009) have provided a novel finding related to this question: Their observations showed that chloroplasts were found within some vacuoles that were isolated from individually darkened leaves of the wild type, but no chloroplasts were found in the vacuole of an atg mutant. Furthermore, the decrease in the chloroplast population was inhibited in atg mutant, whereas the loss of chlorophylls and the decrease of soluble proteins in the mutant were comparable to those in the wild-type. These results demonstrate that autophagy also plays a key role in the transport of whole chloroplasts into vacuoles during leaf senescence.
B. Degradation of Thylakoid Membrane Proteins
Thylakoid membranes contain multiple protein complexes (e.g., Photosystem I, Photosystem II, the cytochrome b 6 f complex and the light-harvesting complex), which play an important role in light-harvesting and the light-dependent reactions of photosynthesis (see Joshi et al., Chap. 28 in this book). More than 30% of the chloroplast proteins are in the protein complexes of the thylakoid membranes. Therefore, the proteins in these complexes are also considered important as nutrient sources during leaf senescence (Krupinska 2007). During leaf senescence, the structure of thylakoid membranes changes dramatically. The progressive loss of grana stacking, disappearance of thylakoid membranes and massive accumulation of plastoglobuli occur at this stage (Krupinska 2007; see also Mulisch and Krupinska, Chap. 14). These structural changes are caused by the massive degradation of the protein complexes and the lipids in the thylakoid membranes. In this section, we describe the current knowledge of the degradation mechanisms of proteins in the thylakoid membranes and the participation of proteases during leaf senescence.
1. Degradation Mechanisms of Thylakoid Proteins
Of the chloroplast-protein degradation pathways described above, RCBs do not exhibit chlorophyll autofluorescence and SAVs do not contain thylakoid proteins, whereas chlorophyll a was detected in isolated SAVs (Ishida et al. 2008; Martinez et al. 2008a; see also Costa et al., Chap. 18). Consequently, the degradation of proteins inside chloroplasts and the uptake of chloroplasts by vacuoles are expected to become more important in the degradation of thylakoid membrane proteins. Of thylakoid membrane protein complexes, most thylakoid membrane proteins appear to bind chlorophylls and carotenoids. Accumulating evidence points to fine-tuned regulation between the breakdown of chlorophylls and degradation of apoproteins during leaf senescence (Hörtensteiner, Chap. 16). Loss of chlorophyll b reductase in Arabidopsis (NYC1 and NOL), which catalyzes the first step of chlorophyll b degradation, results in a non-functional stay-green phenotype that impairs chlorophyll catabolism but shows other senescence processes (Kusaba et al. 2007; Sato et al. 2009). In addition, pheophorbide a oxygenase (PAO) and pheophytin pheophorbide hydrolase (PPH) deficiencies result in a non-functional stay-green phenotype (Pruzinska et al. 2003; Schelbert et al. 2009). These stay-green mutants, which retain chlorophylls in senescent leaves, show highly stable LHC proteins, suggesting the requirement of chlorophyll degradation for the full degradation of thylakoid membrane proteins, especially LHC proteins. These findings indicate a close relation between chlorophylls and apoproteins and suggest that the degradation of thylakoid membrane proteins is strictly controlled. Because free chlorophyll is potentially phototoxic, the degradation of chlorophylls during the degradation of thylakoid membrane proteins needs to be tightly controlled. In spite of rapid progress made towards the understanding of chlorophyll degradation (see Hörtensteiner, Chap. 16 in this book), elucidation of the degradation mechanism of thylakoid membrane proteins is lagging.
2. Proteases Involved in Degradation of Membrane Proteins
The best characterized protein-degradation mechanism in thylakoid membranes is the degradation of the PSII reaction center D1 protein in the PSII repair cycle. In higher plants, as described above, much evidence indicates that the thylakoid membrane-bound FtsH and Deg proteases play crucial roles in this process (Kato and Sakamoto 2009). Meanwhile, a study of the Clp protease suggested the cytochrome b 6 f complex to be a putative substrate for Clp during nitrogen starvation in the green alga Chlamydomonas reinhardtii (Majeran et al. 2000). Lon protease, an ATP-dependent serine protease, and SppA protease, an ATP-independent serine protease, are closely associated with the stromal side of thylakoid membranes (Lensch et al. 2001; Ostersetzer et al. 2007). These proteases also seem to play roles in proteolysis of the thylakoid membrane (Wetzel et al. 2009), although their substrates are poorly understood. These reports specifically address protease functions in the mechanism of protein homeostasis, but do not explain the role of the protease during leaf senescence. We hope that further studies will reveal the role of the major chloroplast proteases in the degradation of thylakoid membrane proteins in leaf senescence.
IV. Concluding Remarks
Over the past two decades, much effort has been devoted to identify and characterize chloroplast proteases. Consequently, numerous chloroplast proteases that are homologous with known bacterial proteases have been identified. The analyses of Arabidopsis mutants has revealed, as described in this chapter, that some are necessary not only for chloroplast biogenesis but also for plant viability. However, the specific substrates of these proteases during leaf development remain unclear. Exploring the recognition mechanisms of substrates in these proteases constitutes an important area of future studies in this field. Additionally, communications between proteolytic activities and chloroplast development, like the delayed chloroplast development that is observed in the variegated mutants, is expected to become an interesting area of investigation. Our knowledge about chloroplast protein degradation during leaf senescence remains poor despite recent efforts in unravelling the mechanisms of protein degradation. The difficulty in elucidation of the mechanism of protein degradation during leaf senescence is apparently due to the complexity of leaf senescence that results from the involvement of multiple factors (e.g., light, nutrition, and the developmental stage of the plant). The contribution of chloroplast proteases in protein degradation during leaf senescence is an important question that should be examined critically in future studies. We hope that greater efforts in this field will answer these questions.
Abbreviations
- AAA:
-
ATPases associated with diverse cellular activities;
- ATG:
-
Autophagy-related gene;
- Cpn60:
-
Chaperonin 60;
- cpSec:
-
Chloroplast secretory pathway;
- cpSRP:
-
Chloroplast signal recognition particle;
- cpTat:
-
Chloroplast twin-argnine translocation;
- GroEL:
-
Hsp60 class oligomeric molecular chaperone;
- Hsc:
-
Heat shock cognate protein;
- Hsp:
-
Heat shock protein;
- LHC:
-
Light-harvesting complex;
- MEP:
-
Methylerythritol phosphate;
- OEC:
-
Oxygen-evolving complex of photosystem II;
- PAO:
-
Pheophorbide a oxygenase;
- Plsp:
-
Plastidic type I signal peptidase;
- PPH:
-
Pheophytin pheophorbide hydrolase;
- PreP:
-
Presequence protease;
- PSII:
-
Photosystem II;
- RCB:
-
Rubisco-containing body;
- Rubisco:
-
Ribulose 1,5-bisphosphate carboxylase-oxygenase;
- SAG:
-
Senescence-associated gene;
- SAV:
-
Senescence-associated vacuoles;
- SPaseI:
-
Type I signal peptidase;
- SPP:
-
Stromal processing peptidase;
- SREBP:
-
Sterol-regulatory element binding protein;
- TIC:
-
Translocon at the inner envelope membrane of chloroplasts;
- TOC:
-
Translocon at the outer envelope membrane of chloroplasts;
- TPP:
-
Thylakoidal processing peptidase
References
Adam Z (2000) Chloroplast proteases: possible regulators of gene expression? Biochimie 82:647–654
Adam Z, Clarke AK (2002) Cutting edge of chloroplast proteolysis. Trends Plant Sci 7:451–456
Adam Z, Rudella A, van Wijk KJ (2006) Recent advances in the study of Clp, FtsH and other proteases located in chloroplasts. Curr Opin Plant Biol 9:234–240
Akita M, Nielsen E, Keegstra K (1997) Identification of protein transport complexes in the chloroplastic envelope membranes via chemical cross-linking. J Cell Biol 136:983–994
Andersson FI, Tryggvesson A, Sharon M, Diemand AV, Classen M, Best C, Schmidt R, Schelin J, Stanne TM, Bukau B, Robinson CV, Witt S, Mogk A, Clarke AK (2009) Structure and function of a novel type of ATP-dependent Clp protease. J Biol Chem 284:13519–13532
Andres C, Agne B, Kessler F (2010) The TOC complex: preprotein gateway to the chloroplast. Biochim Biophys Acta 1803:715–723
Apuya NR, Yadegari R, Fischer RL, Harada JJ, Zimmerman JL, Goldberg RB (2001) The Arabidopsis embryo mutant schlepperless has a defect in the chaperonin-60alpha gene. Plant Physiol 126:717–730
Archibald JM (2009) The puzzle of plastid evolution. Curr Biol 19:81–88
Bailey S, Thompson E, Nixon PJ, Horton P, Mullineaux CW, Robinson C, Mann NH (2002) A critical role for the Var2 FtsH homologue of Arabidopsis thaliana in the photosystem II repair cycle in vivo. J Biol Chem 277:2006–2011
Bhushan S, Lefebvre B, Ståhl A, Wright SJ, Bruce BD, Boutry M, Glaser E (2003) Dual targeting and function of a protease in mitochondria and chloroplasts. EMBO Rep 4:1073–1078
Bhushan S, Ståhl A, Nilsson S, Lefebvre B, Seki M, Roth C, McWilliam D, Wright SJ, Liberles DA, Shinozaki K, Bruce BD, Boutry M, Glaser E (2005) Catalysis, subcellular localization, expression and evolution of the targeting peptides degrading protease, AtPreP2. Plant Cell Physiol 46:985–996
Bieniossek C, Schalch T, Bumann M, Meister M, Meier R, Baumann U (2006) The molecular architecture of the metalloprotease FtsH. Proc Natl Acad Sci USA 103:3066–3071
Bölter B, Nada A, Fulgosi H, Soll J (2006) A chloroplastic inner envelope membrane protease is essential for plant development. FEBS Lett 580:789–794
Bushnell TP, Bushnell D, Jagendorf AT (1993) A purified zinc protease of pea chloroplasts, EP1, degrades the large subunit of ribulose-1,5-bisphosphate carboxylase/oxygenase. Plant Physiol 103:585–591
Cao D, Froehlich JE, Zhang H, Cheng CL (2003) The chlorate-resistant and photomorphogenesis-defective mutant cr88 encodes a chloroplast-targeted HSP90. Plant J 33:107–118
Chaal BK, Mould RM, Barbrook AC, Gray JC, Howe CJ (1998) Characterization of a cDNA encoding the thylakoidal processing peptidase from Arabidopsis thaliana. Implications for the origin and catalytic mechanism of the enzyme. J Biol Chem 273:689–692
Chassin Y, Kapri-Pardes E, Sinvany G, Arad T, Adam Z (2002) Expression and characterization of the thylakoid lumen protease DegP1 from Arabidopsis. Plant Physiol 130:857–864
Chen M, Choi Y, Voytas DF, Rodermel S (2000) Mutations in the Arabidopsis VAR2 locus cause leaf variegation due to the loss of a chloroplast FtsH protease. Plant J 22:303–313
Chen G, Bi YR, Li N (2005) EGY1 encodes a membrane-associated and ATP-independent metalloprotease that is required for chloroplast development. Plant J 41:364–375
Chen J, Burke JJ, Velten J, Xin Z (2006) FtsH11 protease plays a critical role in Arabidopsis thermotolerance. Plant J 48:73–84
Chi W, Sun X, Zhang L (2011) The roles of chloroplast proteases in the biogenesis and maintenance of photosystem II. Biochim Biophys Acta 1817:239–246
Chiba A, Ishida H, Nishizawa NK, Makino A, Mae T (2003) Exclusion of ribulose-1,5-bisphosphate carboxylase/oxygenase from chloroplasts by specific bodies in naturally senescing leaves of wheat. Plant Cell Physiol 44:914–921
Clarke AK, MacDonald MT, Sjögren LLE (2005) The ATP-dependent Clp protease in chloroplasts of higher plants. Physiol Plant 123:406–412
Clausen T, Southan C, Ehrmann M (2002) The HtrA family of proteases: implications for protein composition and cell fate. Mol Cell 10:443–455
Cline K, Dabney-Smith C (2008) Plastid protein import and sorting: different paths to the same compartments. Curr Opin Plant Biol 11:585–592
Constan D, Froehlich JE, Rangarajan S, Keegstra K (2004) A stromal Hsp100 protein is required for normal chloroplast development and function in Arabidopsis. Plant Physiol 136:3605–3615
Diaz C, Lemaitre T, Christ A, Azzopardi M, Kato Y, Sato F, Morot-Gaudry JF, Le Dily F, Masclaux-Daubresse C (2008) Nitrogen recycling and remobilization are differentially controlled by leaf senescence and development stage in Arabidopsis under low nitrogen nutrition. Plant Physiol 147:1437–1449
Erbse A, Schmidt R, Bornemann T, Schneider-Mergener J, Mogk A, Zahn R, Dougan DA, Bukau B (2006) ClpS is an essential component of the N-end rule pathway in Escherichia coli. Nature 439:753–756
Feller U, Anders I, Mae T (2008) Rubiscolytics: fate of Rubisco after its enzymatic function in a cell is terminated. J Exp Bot 59:1615–1624
Friedrich JW, Huffaker RC (1980) Photosynthesis, leaf resistances, and ribulose-1,5-bisphosphate carboxylase degradation in senescing barley leaves. Plant Physiol 65:1103–1107
Friso G, Giacomelli L, Ytterberg AJ, Peltier JB, Rudella A, Sun Q, Wijk KJ (2004) In-depth analysis of the thylakoid membrane proteome of Arabidopsis thaliana chloroplasts: new proteins, new functions, and a plastid proteome database. Plant Cell 16:478–499
Gregersen PL, Holm PB, Krupinska K (2008) Leaf senescence and nutrient remobilisation in barley and wheat. Plant Biol (Stuttg) 10(Suppl 1):37–49
Grimaud R, Kessel M, Beuron F, Steven AC, Maurizi MR (1998) Enzymatic and structural similarities between the Escherichia coli ATP-dependent proteases, ClpXP and ClpAP. J Biol Chem 273:12476–12481
Gunning B (2005) Plastid stromules: video microscopy of their outgrowth, retraction, tensioning, anchoring, branching, bridging, and tip-shedding. Protoplasma 225:33–42
Haussühl K, Andersson B, Adamska I (2001) A chloroplast DegP2 protease performs the primary cleavage of the photodamaged D1 protein in plant photosystem II. EMBO J 20:713–722
Hortensteiner S, Feller U (2002) Nitrogen metabolism and remobilization during senescence. J Exp Bot 53:927–937
Huesgen PF, Schuhmann H, Adamska I (2005) The family of Deg proteases in cyanobacteria and chloroplasts of higher plants. Physiol Plant 123:413–420
Huesgen PF, Schuhmann H, Adamska I (2006) Photodamaged D1 protein is degraded in Arabidopsis mutants lacking the Deg2 protease. FEBS Lett 580:6929–6932
Inada N, Sakai A, Kuroiwa H, Kuroiwa T (1998) Three-dimensional analysis of the senescence program in rice (Oryza sativa L.) coleoptiles. Investigations of tissues and cells by fluorescence microscopy. Planta 205:153–164
Inoue K, Baldwin AJ, Shipman RL, Matsui K, Theg SM, Ohme-Takagi M (2005) Complete maturation of the plastid protein translocation channel requires a type I signal peptidase. J Cell Biol 171:425–430
Ishida H, Yoshimoto K, Izumi M, Reisen D, Yano Y, Makino A, Ohsumi Y, Hanson MR, Mae T (2008) Mobilization of rubisco and stroma-localized fluorescent proteins of chloroplasts to the vacuole by an ATG gene-dependent autophagic process. Plant Physiol 148:142–155
Itzhaki H, Naveh L, Lindahl M, Cook M, Adam Z (1998) Identification and characterization of DegP, a serine protease associated with the luminal side of the thylakoid membrane. J Biol Chem 273:7094–7098
Jackson-Constan D, Akita M, Keegstra K (2001) Molecular chaperones involved in chloroplast protein import. Biochim Biophys Acta 1541:102–113
Johnson KA, Bhushan S, Ståhl A, Hallberg BM, Frohn A, Glaser E, Eneqvist T (2006) The closed structure of presequence protease PreP forms a unique 10,000 Å3 chamber for proteolysis. EMBO J 25:1977–1986
Kapri-Pardes E, Naveh L, Adam Z (2007) The thylakoid lumen protease Deg1 is involved in the repair of photosystem II from photoinhibition in Arabidopsis. Plant Cell 19:1039–1047
Kato Y, Sakamoto W (2009) Protein quality control in chloroplasts: a current model of D1 protein degradation in the photosystem II repair cycle. J Biochem 146:463–469
Kato Y, Sakamoto W (2010) New insight into the type and function of proteases in plastids. In: Jeon KW (ed) International review of cell and molecular biology, vol 161. Burlington Academic Press, Burlington, pp 185–218
Kato Y, Murakami S, Yamamoto Y, Chatani H, Kondo Y, Nakano T, Yokota A, Sato F (2004) The DNA-binding protease, CND41, and the degradation of ribulose-1,5-bisphosphate carboxylase/oxygenase in senescent leaves of tobacco. Planta 220:97–104
Kato Y, Yamamoto Y, Murakami S, Sato F (2005) Post-translational regulation of CND41 protease activity in senescent tobacco leaves. Planta 222:643–651
Kato Y, Miura E, Matsushima R, Sakamoto W (2007) White leaf sectors in yellow variegated2 are formed by viable cells with undifferentiated plastids. Plant Physiol 144:952–960
Kato Y, Miura E, Ido K, Ifuku K, Sakamoto W (2009) The variegated mutants lacking chloroplastic FtsHs are defective in D1 degradation and accumulate reactive oxygen species. Plant Physiol 151:1790–1801
Kessel M, Maurizi MR, Kim B, Kocsis E, Trus BL, Singh SK, Steven AC (1995) Homology in structural organization between E. coli ClpAP protease and the eukaryotic 26S proteasome. J Mol Biol 250:587–594
Kessler F, Blobel G (1996) Interaction of the protein import and folding machineries of the chloroplast. Proc Natl Acad Sci USA 93:7684–7689
Kim J, Rudella A, Ramirez Rodriguez V, Zybailov B, Olinares PD, van Wijk KJ (2009) Subunits of the plastid ClpPR protease complex have differential contributions to embryogenesis, plastid biogenesis, and plant development in Arabidopsis. Plant Cell 21:1669–1692
Kimec-Wisniewska B, Krumpe K, Urantowka A, Sakamoto W, Pratje E, Janska H (2008) Plant mitochondrial rhomboid, AtRBL12, has different substrate specificity from its yeast counterpart. Plant Mol Biol 68:159–171
Kiyosue T, Yamaguchi-Shinozaki K, Shinozaki K (1993) Characterization of cDNA for a dehydration-inducible gene that encodes a CLP A, B-like protein in Arabidopsis thaliana L. Biochem Biophys Res Commun 196:1214–1220
Kourtz L, Ko K (1997) The early stage of chloroplast protein import involves Com70. J Biol Chem 272:2808–2813
Koussevitzky S, Stanne TM, Peto CA, Giap T, Sjogren LL, Zhao Y, Clarke AK, Chory J (2007) An Arabidopsis thaliana virescent mutant reveals a role for ClpR1 in plastid development. Plant Mol Biol 63:85–96
Kovacheva S, Bedard J, Patel R, Dudley P, Twell D, Rios G, Koncz C, Jarvis P (2005) In vivo studies on the roles of Tic110, Tic40 and Hsp93 during chloroplast protein import. Plant J 41:412–428
Kovacheva S, Bedard J, Wardle A, Patel R, Jarvis P (2007) Further in vivo studies on the role of the molecular chaperone, Hsp93, in plastid protein import. Plant J 50:364–379
Kovacs-Bogdan E, Soll J, Bolter B (2010) Protein import into chloroplasts: the Tic complex and its regulation. Biochim Biophys Acta 1803:740–747
Krupinska K (2007) Fate and activity of plastids during leaf senescence. In: Wise RR, Hoober J (eds) The structure and function of plastids, advances in photosynthesis and respiration, vol 23, Series Ed., Govindjee. Springer, Dordrecht, pp 433–449
Krzywda S, Brzozowski AM, Verma C, Karata K, Ogura T, Wilkinson AJ (2002) The crystal structure of the AAA domain of the ATP-dependent protease FtsH of Escherichia coli at 1.5 Å resolution. Structure 10:1073–1083
Kusaba M, Ito H, Morita R, Iida S, Sato Y, Fujimoto M, Kawasaki S, Tanaka R, Hirochika H, Nishimura M, Tanaka A (2007) Rice NON-YELLOW COLORING1 is involved in light-harvesting complex II and grana degradation during leaf senescence. Plant Cell 19:1362–1375
Latijnhouwers M, Xu XM, Moller SG (2010) Arabidopsis stromal 70-kDa heat shock proteins are essential for chloroplast development. Planta 232:567–578
Lee U, Rioflorido I, Hong SW, Larkindale J, Waters ER, Vierling E (2007) The Arabidopsis ClpB/Hsp100 family of proteins: chaperones for stress and chloroplast development. Plant J 49:115–127
Lensch M, Herrmann RG, Sokolenko A (2001) Identification and characterization of SppA, a novel light-inducible chloroplast protease complex associated with thylakoid membranes. J Biol Chem 276:33645–33651
Levy-Rimler G, Bell RE, Ben-Tal N, Azem A (2002) Type I chaperonins: not all are created equal. FEBS Lett 529:1–5
Lindahl M, Tabak S, Cseke L, Pichersky E, Andersson B, Adam Z (1996) Identification, characterization, and molecular cloning of a homologue of the bacterial FtsH protease in chloroplasts of higher plants. J Biol Chem 271:29329–29334
Lindahl M, Spetea C, Hundal T, Oppenheim AB, Adam Z, Andersson B (2000) The thylakoid FtsH protease plays a role in the light-induced turnover of the photosystem II D1 protein. Plant Cell 12:419–431
Liu X, Yu F, Rodermel S (2010) An Arabidopsis pentatricopeptide repeat protein, SVR7, is required for FtsH-mediated chloroplast biogenesis. Plant Physiol 154:1588–1601
Mae T (2004) Leaf senescence and nitrogen metabolism. In: Nooden L (ed) Plant cell death processes. Elsevier Academic Press, San Diego, pp 157–168
Mae T, Kai N, Makino A, Ohira S (1984) Relation between riblose bisphosphate carboxylase content and chloroplast number in naturally senescing primary leaves of wheat. Plant Cell Physiol 25:333–336
Majeran W, Wollman FA, Vallon O (2000) Evidence for a role of ClpP in the degradation of the chloroplast cytochrome b6f complex. Plant Cell 12:137–150
Martinez DE, Costa ML, Gomez FM, Otegui MS, Guiamet JJ (2008a) ‘Senescence-associated vacuoles’ are involved in the degradation of chloroplast proteins in tobacco leaves. Plant J 56:196–206
Martinez DE, Costa ML, Guiamet JJ (2008b) Senescence-associated degradation of chloroplast proteins inside and outside the organelle. Plant Biol 10:15–22
Minamikawa T, Toyooka K, Okamoto T, Hara-Nishimura I, Nishimura M (2001) Degradation of ribulose-bisphosphate carboxylase by vacuolar enzymes of senescing French bean leaves: immunocytochemical and ultrastructural observations. Protoplasma 218:144–153
Mitsuhashi W, Feller U (1992) Effects of light and external solutes on the catabolism of nuclear-encoded stromal proteins in intact chloroplasts isolated from pea leaves. Plant Physiol 100:2100–2105
Miura E, Kato Y, Matsushima R, Albrecht V, Laalami S, Sakamoto W (2007) The balance between protein synthesis and degradation in chloroplasts determines leaf variegation in Arabidopsis yellow variegated mutants. Plant Cell 19:1313–1328
Moberg P, Stahl A, Bhushan S, Wright SJ, Eriksson A, Bruce BD, Glaser E (2003) Characterization of a novel zinc metalloprotease involved in degrading targeting peptides in mitochondria and chloroplasts. Plant J 36:616–628
Moore T, Keegstra K (1993) Characterization of a cDNA clone encoding a chloroplast-targeted Clp homologue. Plant Mol Biol 21:525–537
Murakami S, Kondo Y, Nakano T, Sato F (2000) Protease activity of CND41, a chloroplast nucleoid DNA-binding protein, isolated from cultured tobacco cells. FEBS Lett 468:15–18
Myouga F, Motohashi R, Kuromori T, Nagata N, Shinozaki K (2006) An Arabidopsis chloroplast-targeted Hsp101 homologue, APG6, has an essential role in chloroplast development as well as heat-stress response. Plant J 48:249–260
Nakabayashi K, Ito M, Kiyosue T, Shinozaki K, Watanabe A (1999) Identification of clp genes expressed in senescing Arabidopsis leaves. Plant Cell Physiol 40:504–514
Nakano T, Murakami S, Shoji T, Yoshida S, Yamada Y, Sato F (1997) A novel protein with DNA binding activity from tobacco chloroplast nucleoids. Plant Cell 9:1673–1682
Nakashima K, Kiyosue T, Yamaguchi-Shinozaki K, Shinozaki K (1997) A nuclear gene, erd1, encoding a chloroplast-targeted Clp protease regulatory subunit homolog is not only induced by water stress but also developmentally up-regulated during senescence in Arabidopsis thaliana. Plant J 12:851–861
Nielsen E, Akita M, Davila-Aponte J, Keegstra K (1997) Stable association of chloroplastic precursors with protein translocation complexes that contain proteins from both envelope membranes and a stromal Hsp100 molecular chaperone. EMBO J 16:935–946
Nilsson CS, Backman HG, Pesaresi P, Leister D, Glaser E (2009) Deletion of an organellar peptidasome PreP affects early development in Arabidopsis thaliana. Plant Mol Biol 71:497–508
Niwa H, Tsuchiya D, Makyio H, Yoshida M, Morikawa K (2002) Hexameric ring structure of the ATPase domain of the membrane-integrated metalloprotease FtsH from Thermus thermophilus HB8. Structure 10:1415–1423
Olinares PD, Kim J, van Wijk KJ (2011) The Clp protease system; a central component of the chloroplast protease network. Biochim Biophys Acta 1807:999–1011
Ono K, Hashimoto H, Katoh S (1995) Changes in the number and size of chloroplasts during senescence of primary leaves of wheat grown under different conditions. Plant Cell Physiol 36:9–17
Ostersetzer O, Adam Z (1997) Light-stimulated degradation of an unassembled Rieske FeS protein by a thylakoid-bound protease: the possible role of the FtsH protease. Plant Cell 9:957–965
Ostersetzer O, Kato Y, Adam Z, Sakamoto W (2007) Multiple intracellular locations of Lon protease in Arabidopsis: evidence for the localization of AtLon4 to chloroplasts. Plant Cell Physiol 48:881–885
Otegui MS, Noh YS, Martinez DE, Vila Petroff MG, Staehelin LA, Amasino RM, Guiamet JJ (2005) Senescence-associated vacuoles with intense proteolytic activity develop in leaves of Arabidopsis and soybean. Plant J 41:831–844
Park S, Rodermel SR (2004) Mutations in ClpC2/Hsp100 suppress the requirement for FtsH in thylakoid membrane biogenesis. Proc Natl Acad Sci USA 101:12765–12770
Parrott DL, McInnerney K, Feller U, Fischer AM (2007) Steam-girdling of barley (Hordeum vulgare) leaves leads to carbohydrate accumulation and accelerated leaf senescence, facilitating transcriptomic analysis of senescence-associated genes. New Phytol 176:56–69
Peltier JB, Ytterberg J, Liberles DA, Roepstorff P, van Wijk KJ (2001) Identification of a 350-kDa ClpP protease complex with 10 different Clp isoforms in chloroplasts of Arabidopsis thaliana. J Biol Chem 276:16318–16327
Peltier JB, Emanuelsson O, Kalume DE, Ytterberg J, Friso G, Rudella A, Liberles DA, Soderberg L, Roepstorff P, von Heijne G, van Wijk KJ (2002) Central functions of the lumenal and peripheral thylakoid proteome of Arabidopsis determined by experimentation and genome-wide prediction. Plant Cell 14:211–236
Peltier JB, Ripoll DR, Friso G, Rudella A, Cai Y, Ytterberg J, Giacomelli L, Pillardy J, van Wijk KJ (2004) Clp protease complexes from photosynthetic and non-photosynthetic plastids and mitochondria of plants, their predicted three-dimensional structures, and functional implications. J Biol Chem 279:4768–4781
Peoples MB, Beilharz VC, Waters SP, Simpson RJ, Dalling MJ (1980) Nitrogen redistribution during grain growth in wheat (Triticum aestivum L.). Planta 149:241–251
Porankiewicz J, Wang J, Clarke AK (1999) New insights into the ATP-dependent Clp protease: Escherichia coli and beyond. Mol Microbiol 32:449–458
Prins A, van Heerden PD, Olmos E, Kunert KJ, Foyer CH (2008) Cysteine proteinases regulate chloroplast protein content and composition in tobacco leaves: a model for dynamic interactions with ribulose-1,5-bisphosphate carboxylase/oxygenase (Rubisco) vesicular bodies. J Exp Bot 59:1935–1950
Pruzinska A, Tanner G, Anders I, Roca M, Hortensteiner S (2003) Chlorophyll breakdown: pheophorbide a oxygenase is a Rieske-type iron-sulfur protein, encoded by the accelerated cell death 1 gene. Proc Natl Acad Sci USA 100:15259–15264
Ragster LE, Chrispeels MJ (1981) Autodigestion in crude extracts of soybean leaves and isolated chloroplasts as a measure of proteolytic activity. Plant Physiol 67:104–109
Richter S, Zhang R, Lamppa GK (2005) Function of the stromal processing peptidase in the chloroplast import pathway. Physiol Plant 123:362–368
Roulin S, Feller U (1998) Light-independent degradation of stromal proteins in intact chloroplasts isolated from Pisum sativum L. leaves: requirement for divalent cations. Planta 205:297–304
Rudella A, Friso G, Alonso JM, Ecker JR, van Wijk KJ (2006) Downregulation of ClpR2 leads to reduced accumulation of the ClpPRS protease complex and defects in chloroplast biogenesis in Arabidopsis. Plant Cell 18:1704–1721
Sakamoto W (2006) Protein degradation machineries in plastids. Annu Rev Plant Biol 57:599–621
Sakamoto W, Tamura T, Hanba-Tomita Y, Murata M (2002) The VAR1 locus of Arabidopsis encodes a chloroplastic FtsH and is responsible for leaf variegation in the mutant alleles. Genes Cells 7:769–780
Sakamoto W, Zaltsman A, Adam Z, Takahashi Y (2003) Coordinated regulation and complex formation of yellow variegated1 and yellow variegated2, chloroplastic FtsH metalloproteases involved in the repair cycle of photosystem II in Arabidopsis thylakoid membranes. Plant Cell 15:2843–2855
Sakamoto W, Uno Y, Zhang Q, Miura E, Kato Y, Sodmergen (2009) Arrested differentiation of proplastids into chloroplasts in variegated leaves characterized by plastid ultrastructure and nucleoid morphology. Plant Cell Physiol 50:2069–2083
Sato Y, Morita R, Katsuma S, Nishimura M, Tanaka A, Kusaba M (2009) Two short-chain dehydrogenase/reductases, NON-YELLOW COLORING 1 and NYC1-LIKE, are required for chlorophyll b and light-harvesting complex II degradation during senescence in rice. Plant J 57:120–131
Schelbert S, Aubry S, Burla B, Agne B, Kessler F, Krupinska K, Hortensteiner S (2009) Pheophytin pheophorbide hydrolase (pheophytinase) is involved in chlorophyll breakdown during leaf senescence in Arabidopsis. Plant Cell 21:767–785
Schnell DJ, Kessler F, Blobel G (1994) Isolation of components of the chloroplast protein import machinery. Science 266:1007–1012
Schubert M, Petersson UA, Haas BJ, Funk C, Schroder WP, Kieselbach T (2002) Proteome map of the chloroplast lumen of Arabidopsis thaliana. J Biol Chem 277:8354–8365
Seo S, Okamoto M, Iwai T, Iwano M, Fukui K, Isogai A, Nakajima N, Ohashi Y (2000) Reduced levels of chloroplast FtsH protein in tobacco mosaic virus-infected tobacco leaves accelerate the hypersensitive reaction. Plant Cell 12:917–932
Shanklin J, DeWitt ND, Flanagan JM (1995) The stroma of higher plant plastids contain ClpP and ClpC, functional homologs of Escherichia coli ClpP and ClpA: an archetypal two-component ATP-dependent protease. Plant Cell 7:1713–1722
Shikanai T, Shimizu K, Ueda K, Nishimura Y, Kuroiwa T, Hashimoto T (2001) The chloroplast clpP gene, encoding a proteolytic subunit of ATP-dependent protease, is indispensable for chloroplast development in tobacco. Plant Cell Physiol 42:264–273
Shipman RL, Inoue K (2009) Suborganellar localization of plastidic type I signal peptidase 1 depends on chloroplast development. FEBS Lett 583:938–942
Shipman-Roston RL, Ruppel NJ, Damoc C, Phinney BS, Inoue K (2010) The significance of protein maturation by plastidic type I signal peptidase 1 for thylakoid development in Arabidopsis chloroplasts. Plant Physiol 152:1297–1308
Sinvany-Villalobo G, Davydov O, Ben-Ari G, Zaltsman A, Raskind A, Adam Z (2004) Expression in multigene families. Analysis of chloroplast and mitochondrial proteases. Plant Physiol 135:1336–1345
Sjögren LL, Clarke AK (2011) Assembly of the chloroplast ATP-dependent Clp protease in Arabidopsis is regulated by the ClpT accessory proteins. Plant Cell 23:322–332
Sjögren LL, MacDonald TM, Sutinen S, Clarke AK (2004) Inactivation of the clpC1 gene encoding a chloroplast Hsp100 molecular chaperone causes growth retardation, leaf chlorosis, lower photosynthetic activity, and a specific reduction in photosystem content. Plant Physiol 136:4114–4126
Sjögren LL, Stanne TM, Zheng B, Sutinen S, Clarke AK (2006) Structural and functional insights into the chloroplast ATP-dependent Clp protease in Arabidopsis. Plant Cell 18:2635–2649
Skorko-Glonek J, Wawrzynow A, Krzewski K, Kurpierz K, Lipinska B (1995) Site-directed mutagenesis of the HtrA (DegP) serine protease, whose proteolytic activity is indispensable for Escherichia coli survival at elevated temperatures. Gene 163:47–52
Spiess C, Beil A, Ehrmann M (1999) A temperature-dependent switch from chaperone to protease in a widely conserved heat shock protein. Cell 97:339–347
Ståhl A, Moberg P, Ytterberg J, Panfilov O, Brockenhuus Von Lowenhielm H, Nilsson F, Glaser E (2002) Isolation and identification of a novel mitochondrial metalloprotease (PreP) that degrades targeting presequences in plants. J Biol Chem 277:41931–41939
Ståhl A, Nilsson S, Lundberg P, Bhushan S, Biverstahl H, Moberg P, Morisset M, Vener A, Maler L, Langel U, Glaser E (2005) Two novel targeting peptide degrading proteases, PrePs, in mitochondria and chloroplasts, so similar and still different. J Mol Biol 349:847–860
Stanne TM, Sjogren LL, Koussevitzky S, Clarke AK (2009) Identification of new protein substrates for the chloroplast ATP-dependent Clp protease supports its constitutive role in Arabidopsis. Biochem J 417:257–268
Su PH, Li HM (2008) Arabidopsis stromal 70-kD heat shock proteins are essential for plant development and important for thermotolerance of germinating seeds. Plant Physiol 146:1231–1241
Sun X, Peng L, Guo J, Chi W, Ma J, Lu C, Zhang L (2007) Formation of DEG5 and DEG8 complexes and their involvement in the degradation of photodamaged photosystem II reaction center D1 protein in Arabidopsis. Plant Cell 19:1347–1361
Sun X, Fu T, Chen N, Guo J, Ma J, Zou M, Lu C, Zhang L (2010a) The stromal chloroplast Deg7 protease participates in the repair of photosystem II after photoinhibition in Arabidopsis. Plant Physiol 152:1263–1273
Sun X, Ouyang M, Guo J, Ma J, Lu C, Adam Z, Zhang L (2010b) The thylakoid protease Deg1 is involved in photosystem-II assembly in Arabidopsis thaliana. Plant J 62:240–249
Suno R, Niwa H, Tsuchiya D, Zhang X, Yoshida M, Morikawa K (2006) Structure of the whole cytosolic region of ATP-dependent protease FtsH. Mol Cell 22:575–585
Takechi K, Sodmergen, Motoyoshi F, Sakamoto W (2000) The YELLOW VARIEGATED (VAR2) locus encodes a homologue of FtsH, an ATP-dependent protease in Arabidopsis. Plant Cell Physiol 41:1334–1346
Tomoyasu T, Yuki T, Morimura S, Mori H, Yamanaka K, Niki H, Hiraga S, Ogura T (1993) The Escherichia coli FtsH protein is a prokaryotic member of a protein family of putative ATPases involved in membrane functions, cell cycle control, and gene expression. J Bacteriol 175:1344–1351
VanderVere PS, Bennett TM, Oblong JE, Lamppa GK (1995) A chloroplast processing enzyme involved in precursor maturation shares a zinc-binding motif with a recently recognized family of metalloendopeptidases. Proc Natl Acad Sci USA 92:7177–7181
Wada S, Ishida H, Izumi M, Yoshimoto K, Ohsumi Y, Mae T, Makino A (2009) Autophagy plays a role in chloroplast degradation during senescence in individually darkened leaves. Plant Physiol 149:885–893
Wan J, Bringloe D, lamppa GK (1998) Disruption of chloroplast biogenesis and plant development upon down-regulation of a chloroplast processing enzyme involved in the import pathway. Plant J 15:459–468
Wang J, Hartling JA, Flanagan JM (1997) The structure of ClpP at 2.3 A resolution suggests a model for ATP-dependent proteolysis. Cell 91:447–456
Wang KH, Oakes ES, Sauer RT, Baker TA (2008) Tuning the strength of a bacterial N-end rule degradation signal. J Biol Chem 283:24600–24607
Weaver LM, Froehlich JE, Amasino RM (1999) Chloroplast-targeted ERD1 protein declines but its mRNA increases during senescence in Arabidopsis. Plant Physiol 119:1209–1216
Weiss C, Bonshtien A, Farchi-Pisanty O, Vitlin A, Azem A (2009) Cpn20: siamese twins of the chaperonin world. Plant Mol Biol 69:227–238
Wetzel CM, Harmacek LD, Yuan LH, Woperieis JL, Chubb R, Turini P (2009) Loss of chloroplast protease SPPA function alters high light acclimation processes in Arabidopsis thaliana L (Heynh.). J Exp Bot 60:1715–1727
Wise RR (2007) The Structure and Function of Plastids. In: Wise RR, Hoober JK (eds) Advances in photosynthesis and respiration (Series Ed, Govindjee), vol 23. Springer, Dordrecht, pp 3–26
Wittenbach VA, Lin W, Hebert RR (1982) Vacuolar localization of proteases and degradation of chloroplasts in mesophyll protoplasts from senescing primary wheat leaves. Plant Physiol 69:98–102
Yin S, Sun X, Zhang L (2008) An Arabidopsis ctpA homologue is involved in the repair of photosystem II under high light. Chin Sci Bull 53:1021–1026
Yu AY, Houry WA (2007) ClpP: a distinctive family of cylindrical energy-dependent serine proteases. FEBS Lett 581:3749–3757
Yu F, Park S, Rodermel SR (2004) The Arabidopsis FtsH metalloprotease gene family: interchangeability of subunits in chloroplast oligomeric complexes. Plant J 37:864–876
Yu F, Park S, Rodermel SR (2005) Functional redundancy of AtFtsH metalloproteases in thylakoid membrane complexes. Plant Physiol 138:1957–1966
Yu F, Liu X, Alsheikh M, Park S, Rodermel S (2008) Mutations in SUPPRESSOR OF VARIEGATION1, a factor required for normal chloroplast translation, suppress var2-mediated leaf variegation in Arabidopsis. Plant Cell 20:1786–1804
Yue G, Hu X, He Y, Yang A, Zhang J (2010) Identification and characterization of two members of the FtsH gene family in maize (Zea mays L.). Mol Biol Rep 37:855–863
Zaltsman A, Feder A, Adam Z (2005a) Developmental and light effects on the accumulation of FtsH protease in Arabidopsis chloroplasts–implications for thylakoid formation and photosystem II maintenance. Plant J 42:609–617
Zaltsman A, Ori N, Adam Z (2005b) Two types of FtsH protease subunits are required for chloroplast biogenesis and photosystem II repair in Arabidopsis. Plant Cell 17:2782–2790
Zelisko A, Garcia-Lorenzo M, Jackowski G, Jansson S, Funk C (2005) AtFtsH6 is involved in the degradation of the light-harvesting complex II during high-light acclimation and senescence. Proc Natl Acad Sci USA 102:13699–13704
Zhang D, Kato Y, Zhang L, Fujimoto M, Tsutsumi N, Sodmergen, Sakamoto W (2010) The FtsH protease heterocomplex in Arabidopsis: dispensability of type-B protease activity for proper chloroplast development. Plant Cell 22:3710–3725
Zheng B, MacDonald TM, Sutinen S, Hurry V, Clarke AK (2006) A nuclear-encoded ClpP subunit of the chloroplast ATP-dependent Clp protease is essential for early development in Arabidopsis thaliana. Planta 224:1103–1115
Zhong R, Wan J, Jin R, Lamppa G (2003) A pea antisense gene for the chloroplast stromal processing peptidase yields seedling lethals in Arabidopsis: survivors show defective GFP import in vivo. Plant J 34:802–812
Zybailov B, Friso G, Kim J, Rudella A, Rodriguez VR, Asakura Y, Sun Q, van Wijk KJ (2009) Large scale comparative proteomics of a chloroplast Clp protease mutant reveals folding stress, altered protein homeostasis, and feedback regulation of metabolism. Mol Cell Proteomics 8:1789–1810
Acknowledgments
The authors thank Drs. Lixin Zhang and Xuwu Sun for sharing unpublished data on the deg mutants. The work from our group is supported by a Grant-in-Aid for Scientific Research from MEXT (No. 22380007 to W. S and No. 22770042 to Y.K.) and by the Oohara Foundation.
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2013 Springer Science+Business Media Dordrecht
About this chapter
Cite this chapter
Kato, Y., Sakamoto, W. (2013). Plastid Protein Degradation During Leaf Development and Senescence: Role of Proteases and Chaperones. In: Biswal, B., Krupinska, K., Biswal, U. (eds) Plastid Development in Leaves during Growth and Senescence. Advances in Photosynthesis and Respiration, vol 36. Springer, Dordrecht. https://doi.org/10.1007/978-94-007-5724-0_20
Download citation
DOI: https://doi.org/10.1007/978-94-007-5724-0_20
Published:
Publisher Name: Springer, Dordrecht
Print ISBN: 978-94-007-5723-3
Online ISBN: 978-94-007-5724-0
eBook Packages: Biomedical and Life SciencesBiomedical and Life Sciences (R0)