Singlet Oxygen in Plants: Generation, Detection, and Signaling Roles

Abstract

Singlet oxygen (¹O₂) refers to the lowest excited electronic state of molecular oxygen. It easily oxidizes biological molecules and, therefore, is cytotoxic. In plant cells, ¹O₂ is formed mostly in the light in thylakoid membranes by reaction centers of photosystem II. In high concentrations, ¹O₂ destroys membranes, proteins and DNA, inhibits protein synthesis in chloroplasts leading to photoinhibition of photosynthesis, and can result in cell death. However, ¹O₂ also acts as a signal relaying information from chloroplasts to the nucleus, regulating expression of nuclear genes. In spite of its extremely short lifetime, ¹O₂ can diffuse from the chloroplasts into the cytoplasm and the apoplast. As shown by recent studies, ¹O₂-activated signaling pathways depend not only on the levels but also on the sites of ¹O₂ production in chloroplasts, and can activate two types of responses, either acclimation to high light or programmed cell death. ¹O₂ can be produced in high amounts also in root cells during drought stress. This review summarizes recent advances in research on mechanisms and sites of ¹O₂ generation in plants, on ¹O₂-activated pathways of retrograde- and cellular signaling, and on the methods to study ¹O₂ production in plants.

1. Introduction

The most effective way to transform the energy of sunlight into chemical energy that has evolved naturally on Earth is oxygenic photosynthesis [1]. Its side-product is molecular oxygen in the ground triplet state (³O₂), which is generated during oxidation of water coupled to the activity of photosystem II (PS II). Oxygenic photosynthesis thus enabled aerobic respiration necessary for most eukaryotic organisms populating the Earth. However, the appearance of oxygen in the atmosphere also increased the emergence of reactive oxygen species (ROS) which can be harmful, and even dangerous, for cells.

Figure 1 shows that oxygen in the ground triplet state (³O₂) can be converted to ROS via two mechanisms, either via transfer of energy to an oxygen molecule, or via transfer of electrons. The first mechanism results in the formation of singlet oxygen (¹O₂), and the second mechanism leads to a sequential reduction of oxygen to the superoxide-anion-radical (O₂^•−), hydrogen peroxide (H₂O₂) and further to the hydroxyl radical (OH^•) [2]. Other ROS, such as atomic oxygen or ozone, are not produced in living cells. ROS often damage cell components, like proteins, lipids and nucleic acids; at the same time, ROS are critical players in several processes, for instance, in plant protection from pathogens or in cell signaling [3].

Contrariwise to other ROS, ¹O₂ which represents the first excited electronic state of molecular oxygen is not a free radical, and does not carry a high-energy electron. Nevertheless, it easily oxidizes biological molecules and therefore can become toxic [5]. It also serves as a signal in plant cells and possibly in animal cells as well [6,7,8].

Why is ¹O₂ much more reactive than oxygen in its ground state? The ground state of oxygen is a triplet, with two unpaired electrons with identical quantum spin numbers occupying different orbitals (Figure 1). Therefore, triplet oxygen can oxidize a non-radical (singlet) atom or molecule only when it contains a pair of electrons with parallel spins in free orbitals. However, electron pairs usually have opposite spin states. This limits the reactions of triplet oxygen with most organic molecules [9]. Singlet oxygen does not have a spin limitation (Figure 1), and this fact considerably increases its reactivity [9,10]. Figure 2 shows the main types of reactions involving ¹O₂.

In plant cells, ROS can be formed in many compartments including chloroplasts, mitochondria, peroxisomes and plasma membrane. Strong generation of ROS occurs in the light in chloroplasts during photosynthesis. Photosynthesizing leaves capture the energy of sunlight and use it to fix and reduce CO₂. This is accompanied by the translocation of electrons through the electron transport chain (ETC) and by transfer of light energy between chlorophyll molecules, which occurs via generation of excited states of chlorophyll. Both processes can result in the formation of ROS by transfer of electrons and/or energy to oxygen.

ROS production in chloroplasts is especially high when light is available in excess; under these conditions, H₂O₂ and ¹O₂ are generated [9,11]. The largest part of hydrogen peroxide is formed during the dismutation reaction of O₂^•− produced during the Mehler reaction via reduction of oxygen by electrons transferred from ferredoxin [12]. Small quantities of superoxide and hydrogen peroxide can be formed also in the lipid phase of thylakoid membrane in course of the reaction of oxygen with reduced plastoquinone [13]. A special role in ROS generation is played by photosystem II (PS II). The activity of PS II is driven by light energy captured via an ensemble of chlorophyll molecules and transferred to PS II reaction centers. PS II performs redox reactions with very high reducing, as well as oxidizing, redox potentials, including the unique reactions of water splitting. The latter process results in the release of oxygen, which is in its ground (triplet) state. However, PS II activity also leads to formation of ROS. The ROS which is predominantly generated at PS II is ¹O₂ [3,10]. This is due to the formation of long-lived excited triplet states of the P₆₈₀ chlorophyll “special pair” in the PS II reaction center, which are able to transfer their excitation energy to oxygen, for instance, under conditions when electron acceptors downstream are reduced (see below) [11]. Interaction of oxygen with triplet chlorophyll (³Chl^*) is the main pathway of ¹O₂ production in photosynthesizing organisms [3]. As PS II in chloroplasts is not only a site where light energy is transformed into chemical energy with occasional formation of ³Chl^*, but also the site of oxygen production during photosynthesis, the close proximity of both processes further increases the probability of ROS generation at PS II.

2. Formation of ¹O₂ at PS II

Most ¹O₂ in plants is produced in the mesophyll cells of leaves. There, the main sources of ³Chl^* are light harvesting antenna complexes (LHC) and PS II reaction centers [5]. LHC contain the largest portion of leaf chlorophyll; however, as they also contain most of the carotenoids, about 95% of ³Chl^* formed in LHC is quenched [14]. This quenching occurs by a spin exchange leading to the formation of triplet carotenoids which easily dissipate the energy as heat [15]. Furthermore, under excess light a non-radiative mechanism of ¹Chl^* inactivation, the energy-dependent non-photochemical quenching (qE), is activated in LHC which prevents the conversion of ¹Chl^* to ³Chl^* by dissipation of energy as heat [5]. Nevertheless, LHC can generate ¹O₂ in vitro [16].

PS II contains β-carotene but the distance between chlorophyll and β-carotene molecules in PS II reaction centers is too large for quenching to occur. For triplet state quenching, the electron orbitals should overlap, and the distance between the molecules should not exceed 3.6 Å (van-der-Waals distance). In PS II, in contrast to LHC, this distance exceeds 3.6 Å [15]. ¹O₂ is the main ROS formed in PS II reaction centers even at low light intensities [17,18]; however, in high light, when the dissipation of excess light energy can no longer maintain the acceptor side of PS II in a partially oxidized state, the probability of ¹O₂ formation increases considerably [2].

Figure 3 shows the pathways of ¹O₂ formation in PS II [15]. Chlorophyll molecules in LHC and in photosystems are in the ground singlet state. Chlorophyll excited singlet states have a lifetime long enough for conversion of excitation energy into the energy of electrochemical potential by means of charge separation in reaction centers of photosystems. This process occurs in chlorophylls of the ‘special pairs’ designated P₇₀₀ for PS I and P₆₈₀ for PS II, respectively, according to their spectral characteristics [18]. The first detected ion-radical pair formed in the reaction center of PS II after light excitation is the pair of a chlorophyll P₆₈₀^•+ and a pheophytin Pheo^•−. If the transfer of an electron from Pheo^•− to the next acceptor is limited, charge recombination takes place, which can be accompanied by spin conversion and formation of a triplet excited state of ³P^*₆₈₀ with lower energy (1 in Figure 3). Triplet excited chlorophyll has a longer lifetime (10⁻³ s) than singlet excited chlorophyll (10⁻⁸ s), and can interact with oxygen and form ¹O₂ (2 in Figure 3). Thus, charge recombination in reaction centers of PS II leading to formation of ³P^*₆₈₀ promotes ¹O₂ formation [18]. Direct interaction of ³P^*₆₈₀ with triplet oxygen is supported, for instance, by the fact that addition of oxygen shortens the lifetime of ³P^*₆₈₀ from 1 ms to 30 µs; this also lowers the stability of PS II, presumably due to ¹O₂ formation [10].

The life span of oxidized P^•+₆₈₀ is very short due to a fast transfer of electrons from water to P^•+₆₈₀, but also due to a possibility of charge recombination of P^•+₆₈₀ with, apart from Pheo^•−, other primary electron acceptors, Q_A^•− and Q_B^•− (3 in Figure 3), which sometimes leads to the formation of ³P^*₆₈₀ (1 in Figure 3). The probability of recombination increases under conditions when the ETC is over-reduced. Figure 3 shows that this can increase the rate of ¹O₂ formation via reactions 1 and 2.

The redox potential of the plastoquinone Q_A in PS II can vary (Figure 3); for instance, it increases upon 3-(3′, 4′-dichlorophenyl)-1, 1-dimethylurea (DCMU) binding to PS II [10]. A positive shift of the Q_A potential also occurs under cold stress [19,20,21,22] and in high light when a strong acidification of the thylakoid lumen leads to Ca²⁺ release from the oxygen-evolving complex (OEC) of PS II [15,23]. These data were obtained not only with isolated thylakoid membranes but also in vivo. As Figure 3 shows, the probability of charge recombination between P^•+₆₈₀ and high-potential Q_A^•− with formation of the P^•+₆₈₀Pheo^•− pair is very low; the probability of a non-radiative charge recombination to the ground states is much higher (4 in Figure 3). Accordingly, the probability of ¹O₂ formation decreases as well. Apart from this, high-potential Q_A^•− can recombine with oxidized components of the OEC [15,23]. Thus, an increase in the potential of Q_A under stress protects PS II from photoinhibition by means of lowering ¹O₂ production while increasing the probability of “safe” charge recombination for the ion-radical pair P^•+₆₈₀Q_A^•− [15]. Another ‘safety valve’ is a direct non-radiative charge recombination of P^•+₆₈₀Pheo^•− which results in the formation of ¹P₆₈₀ and Pheo (5 in Figure 3).

A positive shift of the Q_A potential also occurs in inactive reaction centers of PS II, where the Mn cluster within the OEC has been destroyed by light [24,25]. According to Johnson et al. [24], non-radiative recombination (4 in Figure 3) takes place in such complexes, lowering the probability of ¹O₂ formation.

On the other hand, some stresses, for instance, drought, that cause stomata closure and a drop of the CO₂ concentration in chloroplasts, lead to over-reduction of the ETC and enhance the probability of charge recombination between P^•+₆₈₀ and low-potential Q_A^•− in PS II [15,26,27]. This leads to an increase in ¹O₂ production.

A special case is represented by inactive reaction centers of PS II which lack an OEC: immature PS II during de novo assembly, and damaged PS II in the course of repair [6]. While functional PS II complexes locate in stacked parts of chloroplast grana membranes (grana cores), de novo assembly and repair of PS II occur in grana margins (Figure 4). As mentioned above, in PS II reaction centers lacking OEC, the redox potential of Q_A is shifted to positive values, and the probability of ¹O₂ generation via formation of ³P^*₆₈₀ is negligible [23]. At the same time, PS II reaction centers are sites of ¹O₂ production not only in grana cores, where functionally active PS II complexes are situated, but also in grana margins [6]. Moreover, ¹O₂ can elicit contrasting signaling pathways in plant cells depending on the site of production—either grana cores or grana margins (see below). Thus far, the exact mechanism of ¹O₂ generation in grana margins remains elusive; supposedly, ¹O₂ can be produced by chlorophyll molecules during their incorporation into PS II complexes in the course of their repair or de novo assembly [6,25]. Both incomplete PS II complexes and enzymes of chlorophyll biosynthesis are located in unstacked marginal parts of the grana [28] (Figure 4). Chlorophyll molecules as well as their precursors can function as photosensitizers and lead to ROS production when not bound to proteins. To avoid this, chlorophyll precursors as well as products of chlorophyll catabolism are bound to special Light-harvesting CP-like proteins (LIL proteins) [25]. Nevertheless, production of ROS, especially ¹O₂, during assembly, repair and disassembly of PS II cannot be excluded [6].

In some studies, generation of ¹O₂ in vitro was demonstrated in isolated thylakoid membranes containing PS II complexes lacking an OEC [29,30]. In such complexes, the long-lived ion-radical pair P₆₈₀^•+TyrZ^• (where TyrZ is the tyrosine residue in the D1 protein which transfers the electrons from OEC to P₆₈₀^•+) was formed in the light which led to the generation of lipid and protein hydroperoxides [29,30]. Oxidation of these hydroperoxides led to the production of peroxyl-radicals and tetrahydroperoxides; the latter can decompose leading to the formation of triplet carbonyls able to perform energy transfer to ³O₂ thereby producing ¹O₂ [29,30]. The importance of this mechanism in vivo has not been studied yet. Notably, in a similar study, no ¹O₂ generation was observed in thylakoid membranes enriched with PS II complexes lacking OEC [31]. To sum up, functional PS II reaction centers in grana cores generate ¹O₂ via charge recombination with the participation of low-potential forms of Q_A^•− [15], while the mechanism of ¹O₂ formation at grana margins is not yet completely clarified [28].

3. Photoinhibition and the Role of ¹O₂

Photoinhibition is the phenomenon of down-regulation of photosynthesis, primarily of the rate of photosynthetic fixation of CO₂, in the light caused by irreversible damage to PS II [32,33]. Of all components of the photosynthetic machinery, PS II has the shortest lifetime and the highest susceptibility to damage; moreover, plants might “sacrifice” PS II to protect PS I from over-reduction and photooxidation, as the repair of PS I is more complicated and energy-demanding than that of PS II [34,35]. Photoinhibition mostly occurs under high light; a term “midday depression of photosynthesis” has been related to this phenomenon [32]. A decrease in photosynthesis observed during long exposure of plants to high light can become more severe under limitation of photosynthetic electron transport. For instance, the reason for “midday depression” is the closure of stomata caused by increasing water loss around noon, which limits the concentration of CO₂, and thereby of the final electron acceptor 1,3-diphosphoglycerate, and leads to over-reduction of the ETC [33].

During photosynthesis, two processes continuously occur: (1) the damage of PS II reaction centers, and (2) their repair. Photoinhibition is observed when process (1) occurs faster than process (2). The D1 protein, the core components of a PS II reaction center, is prone to the highest damage, although other PS II components can also be damaged, for instance, D2, CP43, and CP47 proteins [6]. In chloroplasts, D1 is the protein synthesized at the highest levels. Studies of photoinhibition using plants and cyanobacterial models led to two main hypotheses about the mechanism of D1 damage in the light. The first hypothesis postulates that the primary damaging agent is ¹O₂, production of which increases in excess light. The second hypothesis considers the Mn cluster of the OEC as the site of primary damage, which then leads to the formation of long-lived oxidized cation-radicals TyrZ^•+ at the donor side of PS II, resulting in the oxidation of nearby amino acid residues of the D1 protein [6,36,37].

The decrease in photosynthesis during photoinhibition depends on the light intensity but not on the light spectrum [37]. In contrast, light-induced damage of D1 proteins is proportional to light intensity and to photon energy: UV and blue light cause the highest damage [36]. This action spectrum corresponds to the light spectrum causing damage to the OEC Mn cluster [36]. Obviously, as long as the rate of D1 biosynthesis is sufficient for the repair of PS II, there will be no photoinhibition. However, D1 biosynthesis can be inhibited in excess light, and this inhibition correlates with an increase in ¹O₂ generation [36]. In excess light, over-reduction of the ETC leads to an increase in ROS formation, primarily of ¹O₂, at PS II complexes (Figure 3) [6,37]. ¹O₂ attacks the histidine residues of PS II proteins, which can lead to modifications of PS II reaction centers and exposure of D1 to proteolytic degradation [31,38]. However, the strongest effect on the development of photoinhibition is related to the suppression of protein biosynthesis in chloroplasts by ¹O₂ which oxidizes cysteine residues of the elongation factors EF-G [36,39] and EF-Tu [40]. This suppression of protein biosynthesis in chloroplasts is fully reversible in that the oxidized cysteine residues can be reduced by thioredoxins [36].

These data were obtained using cyanobacterial models. Although also in plants, inhibition of protein translation in chloroplasts by increasing ¹O₂ production is considered the main factor of suppression of D1 biosynthesis, there is no direct evidence for oxidation of elongation factors by ¹O₂ in plants thus far [6]. As discussed above, biosynthesis of D1 protein takes place at grana margins, where the newly synthesized D1 binds chlorophylls and is incorporated into PS II reaction centers during their repair. The FtsH protease, which is also localized at grana margins [41], performs the specific proteolysis and removal of oxidized D1 from PS II [42].

Thus, photodamage of PS II is unavoidable due to the fact that even under low light conditions, light has a damaging effect on the OEC Mn cluster. However, occurrence and extent of photoinhibition depend on the rate of PS II repair, i.e., primarily on the rate of D1 biosynthesis in chloroplasts, which can be inhibited by ROS, mostly by ¹O₂ [37]. Protection from photoinhibition thus should include prevention of ¹O₂ production at PS II. Accordingly, DCMU has a slight protective effect (Figure 3; [43]). Photoinhibition in pumpkin plants was lowered by a strong magnetic field interfering with spin conversion in oxygen molecules and thus with ¹O₂ formation. This effect was not observed in the presence of lincomycin, an inhibitor of protein synthesis in chloroplasts, confirming that ¹O₂ inhibits PS II repair via an effect on protein synthesis [44].

4. Other Sites of ¹O₂ Generation in Plant Cells

¹O₂ is typically formed during the transfer of energy from an excited triplet chromophore molecule (a photosensitizer) to ³O₂ [45,46]. Furthermore, a triplet-triplet transfer of energy from triplet carbonyls of lipids and proteins, ³C = O^*, to ³O₂ can occur [30]. ¹O₂ can form also during decomposition of tetrahydroperoxides of lipids and proteins, C-OOOO-C, via a mechanism proposed by Russell [47].

In chloroplasts, not only chlorophylls but also chlorophyll precursors such as chlorophyllide and protochlorophyllide, as well as chlorophyll catabolites, can function as photosensitizers and lead to ¹O₂ generation [10,25]. However, ¹O₂ is not produced at PS I [5]. When oxidized, the “special pair” chlorophylls of the PS I reaction centers, P⁺₇₀₀, do not perform recombination reactions. Under reducing conditions when the Fe-S clusters of PS I are reduced or phylloquinon is removed from the reaction center, charge recombination can occur and lead to formation of ³P₇₀₀ at room temperature [48]. However, the lifetime of ³P₇₀₀ in PS I is only about 6 µs (compared to 1 ms for ³P₆₈₀), and it does not decrease upon addition of ³O₂, suggesting that P₇₀₀ is shielded from O₂ [10,49]. Interestingly, an Arabidopsis mutant with low contents of β-carotene showed photoinhibition of PS I and formation of ¹O₂ in LHC of PS I [50]. In wild-type plants, photoinhibition of PS I can be induced by multiple saturating light pulses; this was suggested to result in the generation of not only O₂^•− and H₂O₂, but also ¹O₂ at PS I [51]. Altogether, more evidence is required to support this suggestion.

The cytochrome-b6f complex can produce ¹O₂ in the light [52]. Here, the Fe-S cluster of Rieske proteins, as well as a chlorophyll with unknown functions, are probably the sites of ¹O₂ generation [10].

¹O₂ can also be produced in cell compartments other than chloroplasts in a range of enzymatic reactions including those of heme proteins and lipoxygenases [53]. Other sources of ¹O₂ in plants can be phytoalexins, defense compounds that are synthesized upon pathogen attack and can accumulate in every plant organ. Phenalenone-like phytoalexins are photosensitizers, which function as phototoxins generating ¹O₂ to kill pathogens [54]. Phenalenone can generate ¹O₂ with a quantum yield around 1, which explains the fungicidal activity of phenyl-phenalenone phytoalexins [54]. Some plants constitutively produce phytoanticipins, secondary metabolites with antimicrobial activity [55], some of which can function as photosensitizers. For instance, psoralenes and a polycyclic quinone hypericin are phototoxins of the Apiaceae family and of the genus Hypericum, respectively [5]. In animal cells, ¹O₂ can be generated in neutrophils during the myeloperoxidase reaction in the course of phagocytosis [56]; thus far, it is not known whether similar reactions play a role in plants’ defense against pathogens. At any rate, in Arabidopsis thaliana, chlorophyll catabolites can be used as photosensitizers during the hypersensitivity response against the pathogen Pseudomonas syringae [57].

¹O₂ can be produced also in underground plant organs in the absence of light [58,59]. In roots of Arabidopsis thaliana, osmotic stress induced by polyethylene glycol (PEG) elicited ¹O₂ production in the rhizodermis of the root tip, and later in the root apical meristems. This was accompanied by the death of root meristem cells and an increase in lateral root formation. In roots subjected to osmotic stress, the source of ¹O₂ could be hydroperoxides of fatty acids produced by lipoxygenase from linoleic acid; these hydroperoxides can form tetrahydroperoxides which decompose with generation of ¹O₂ according to Russell’s mechanism [47,60,61]. Apart from lipoxygenase reaction, hydroperoxides of linoleic acid in roots could be formed in reactions with hydroxyperoxyl radicals or hydroxyl radicals [4,59].

In tobacco Bright Yellow 2 (BY-2) suspension culture cells, ¹O₂ was produced in the dark in the apoplast in response to hyperosmotic stress induced by salt or sorbitol, supposedly during peroxidase reactions in cell walls [62,63,64]. The rapid production of ¹O₂ induced Ca²⁺ entry in tobacco cells and activated the SOS (Salt Overly Sensitive) signaling cascade necessary to protect cells from accumulation of excess Na⁺ and development of programmed cell death (PCD; [65]).

5. Damaging Effects of ¹O₂

Although ¹O₂ is metastable and its lifetime in the cells is short, a portion of ¹O₂ can diffuse over considerable distances both in polar and non-polar environments [15,17]. The lifetime of ¹O₂ can differ by several orders in various organic solvents [66]. In cell culture, ¹O₂ lifetime is about 10⁻⁶ s, and it can diffuse to a distance of ca. 155 nm [67] and permeate through membranes. In tissues, ¹O₂ rapidly attacks neighboring biomolecules such as DNA, pigments, lipids and proteins, causing oxidative damage [11,68].

In cells, ¹O₂ rapidly oxidizes molecules containing C-C double bonds, forming hydroperoxides or endoperoxides [27]. The main targets of ¹O₂ are double bonds of aromatic amino acid residues in proteins, polyunsaturated fatty acids, guanine bases in nucleic acids and thiols groups (Figure 2). These hydroperoxides can initiate free radical chain reactions, e.g., upon interaction with light or with hydroxyl radicals, which multiplies the damaging effects of ¹O₂.

The most common targets of ¹O₂ are proteins [45]. Generally, proteins are the main targets of oxidative damage in cells due to their large amounts and high reactivity with radicals and excited molecules including ¹O₂. Reactions of tyrosine, tryptophan and histidine, both free and as part of proteins, with ¹O₂ result in high levels of hydroperoxide formation [69]. In proteins, ¹O₂ rapidly oxidizes these amino acids residues and also methionine, cysteine and phenylalanine. As noted above, during photoinhibition, ¹O₂ leads to a degradation of the D1 protein which plays a vital role in primary charge separation and stabilization of PS II [31,38], and also inhibits protein translation in chloroplasts, thus inhibiting D1 repair [36].

Interaction of ¹O₂ with lipids induces their rapid peroxidation [27]. ¹O₂-mediated lipid peroxidation can directly precede cell death [70]. The main target of ¹O₂ is linolenic acid, which leads to the generation of lipid hydroperoxides LOOH, such as 10- and 12-hydroperoxy-octadecadienic acids (HPODE) which represent reactive electrophile species [25]. In the presence of photosensitizers, lipid hydroperoxides can initiate free-radical reactions; therefore, they are detoxified by peroxidases forming other electrophile species such as 13-keto-octadecadienic and -trienic acids. These compounds can serve as signals: for instance, in the green alga Chlamydomonas rheinhardtii, many ¹O₂-activated genes contain «electrophile response elements» in their promoters and are induced by electrophilic lipids [71].

¹O₂ can interact also with DNA by inducing breaks in DNA strands and causing chromosome defects [72]. It reacts preferentially with guanine bases, forming 8-oxo-7,8-dihydroguanine and spiro-iminodihydantoin [73]. These products cause point mutations [25]. However, although ROS can cause severe damage in living cells, increasing amounts of data suggest that ROS-related cell death occurs mostly via activation of signaling pathways leading to PCD while cell death due to oxidative injuries is a relatively rare phenomenon [74].

6. Plant Defense Against ¹O₂

Quenching of ¹O₂ can occur by means of energy dissipation as heat without modifications of the quencher (physical quenching), leading to the formation of a ground state of ³O₂ molecule, or by means of chemical quenching, leading to the formation of oxidized molecules [5]. In plant cells, carotenoids, tocopherols, plastoquinols and ascorbic acid are the main antioxidants protecting the cells from ¹O₂ [25].

As discussed above, ³Chl^* and ¹O₂ produced in LHC can be quenched very efficiently by carotenoids via the physical mechanism [5,18]. Although in PS II reaction centers, β-carotene cannot quench ¹O₂ via production of triplet states, it still protects PS II from ¹O₂ very efficiently by means of chemical quenching [75]. The products of this reaction are specific aldehydes and endoperoxides of β-carotene: β-cyclocitral, dihydroactinidiolide, and b-ionone [75]. These substances initiate signaling pathways, and their generation greatly increases in high light [5,25,76].

Tocopherols can also quench ¹O₂, but their rate of quenching is two orders of magnitude lower than that of β-carotene. α-Tocopherol can be oxidized by ¹O₂ to 8-hydroperoxytocopherol and further to α-tocopherolquinone, at this point, the pathway of α-tocopherol regeneration is unknown. Tocopherols also inhibit ¹O₂-initiated lipid peroxidation in thylakoids by reacting with lipid radicals, thus breaking free-radical reaction chains [77]. Data obtained for C. rheinhardtii showed that plastoquinol in thylakoids can be more effective in ¹O₂ quenching than tocopherols [78]. Moreover, chloroplasts contain high amounts of ascorbic acid [74] which also quenches ¹O₂ [79].

Tryptophan can quench ¹O₂ by a physical mechanism, similar to carotenoids, due to its chemical structure. More often, however, interaction of ¹O₂ with tryptophan leads to the production of peroxides via chemical quenching. These peroxides further can form stable compounds, such as N-formylkynurenine which can be used for identifications of the sites of ROS production [69]. Histidine, cysteine, methionine, tyrosine, and phenylalanine can also quench ¹O₂. The D1 protein is probably oxidized by ¹O₂ at the highest rate of all cellular proteins, and has a high rate of re-synthesis; therefore, it can be considered as a specific chemical quencher of ¹O₂ [18].

As reactions of ¹O₂ with cell components leads to the production of peroxides, reactive electrophilic species and other highly reactive molecules, diverse protective antioxidant systems are required for defense against ¹O₂: They can detoxify the reactive products and break free-radical chain reactions [9,74].

7. Roles of ¹O₂ in Plant Stress Response

While all ROS cause similar cytotoxic effects, the signaling pathways they activate are highly specific. Studies on the effects of ¹O₂ on plants are challenged by the fact that in the light, several types of ROS are produced simultaneously [80]. A very valuable tool for these studies are mutants that specifically produce high amounts of ¹O₂. One of them is the flu (fluorescent in blue light) mutant of Arabidopsis thaliana [81]. The nuclear-encoded chloroplast protein FLU regulates chlorophyll biosynthesis by preventing excess accumulation of the intermediates of Mg-protoporphyrin branch of tetrapyrrole synthesis. FLU forms a complex with proteins catalyzing final steps of chlorophyll synthesis, Mg²⁺-protoporphyrin IX monomethyl ester cyclase and NADPH:protochlorophyllide oxidoreductases B and C [82]. This complex localizes to grana margins [28]. Upon binding free protochlorophyllide, the complex inhibits glutamyl-tRNA-synthetase by blocking protochlorophyllide synthesis. The absence of FLU prevents formation of the glutamyl-tRNA-inhibiting complex, which causes accumulation of free protochlorophyllide in the dark [82].

The flu mutant remains viable when grown under continuous light: It shows growth pattern and seed production similar to those of wild type [83]. However, in the dark flu plants accumulate free protochlorophyllide. After transfer of flu plants from the darkness to light, protochlorophyllide acts as a strong photosensitizer leading to ¹O₂ generation [70,83]. Thus, the flu mutant represents a unique tool for “quantification” of ¹O₂ effects on plants, because the amounts of generated ¹O₂ are proportional to the amounts of accumulated protochlorophyllide, and the latter depends on the length of the dark period. By varying the time of incubation in darkness before transfer of flu plants in the light, dose effects of ¹O₂ on plants can be studied [84].

¹O₂ formation leads to death of flu etiolated seedlings, and to growth arrest in flu green plants [18,70,83]. Notably, neither death nor growth arrest in flu result from oxidative damage exerted by ¹O₂ but occur due to the activation of genetic programs of stress response [18]. ¹O₂-activated genes of early stress response differ from the genes activated by O₂^•- and H₂O₂ [83]. Of special interest are genes that are specifically activated by ¹O₂ and function in PCD. In flu plants, two nuclear-encoded chloroplast proteins, EXECUTER1 (EX1) and EX2, trigger ¹O₂-dependent PCD [80]. In sharp contrast to flu, double mutants flu/ex1 survive dark-to-light transfer even though their levels of accumulated protochlorophyllide and ¹O₂ production are similar to flu [18,85]. However, under severe light stress, even ex1/ex2 plants die due to oxidative damage [86]. EX1 and EX2 proteins localize to grana margins [28]. An increase in ¹O₂ production leads to oxidation of these proteins triggering their proteolysis by the FtsH protease [28]. This proteolysis is related to the oxidation of the Trp643 residue in the DUF3506 domain of EX1; the DUF3506 is highly prone to oxidation by ¹O₂ and was designated SOS (singlet oxygen sensor) domain [87]. It is assumed that EX1 proteins can only be oxidized by ¹O₂ produced at grana margins; therefore, EX1/EX2-mediated signaling represents a ¹O₂-specific retrograde signaling pathway related to synthesis and/or repair of PS II [28].

The Arabidopsis EX1 protein per se mediates ¹O₂-dependent retrograde and/or plastidic signaling. It is degraded by FtsH, and presumably, products of its proteolysis function as signal. Notably, only levels of ¹O₂ sufficient to induce EX1 proteolysis can trigger PCD [28]. In the course of ¹O₂- and EX1/EX2-mediated PCD, levels of salicylic acid (SA) increase and ENHANCED DISEASE SUSCEPTIBILITY1 (EDS1) protein is activated; this protein is a key component of cell death during hypersensitive response elicited by biotrophic pathogens [88]. Accordingly, ¹O₂-dependent PCD is inhibited in flu/eds1 double mutants [88]. The levels of jasmonates (JA) also increase in response to ¹O₂ production in the flu mutant [85,88]. In Arabidopsis, development of ¹O₂-dependent PCD also requires the presence of blue light receptor CRYPTOCHROME 1 (CRY1; [89]). Interestingly, development of PCD due to overaccumulation of protochlorophyllide was observed also in barley mutant tigrina-d.1 orthologous to Arabidopsis flu mutant [90].

Recently, a novel chloroplast protein, SAFEGUARD1 (SAFE1), was shown to localize to the stroma and suppress EX1-dependent PCD in Arabidopsis [91]. SAFE1 protects grana margins from ¹O₂ and is degraded via chloroplast-originating vesicles when ¹O₂ levels rise. Interestingly, SAFE1 was also proposed to function in a novel retrograde signaling pathway leading to PCD induction independently of EX1 [91].

The Arabidopsis ch1 mutant represents another useful model to study ¹O₂ effects on plants. The ch1 plants lack chlorophyll b due to a mutation in the unique gene encoding chlorophyllide-a-oxygenase. In ch1 plants, the LHC antenna of PS II is strongly reduced which disturbs the functions of PS II and the processes of lateral diffusion in thylakoid membranes [80,92,93]. As a result, production of ¹O₂ in PS II reaction centers is strongly increased in ch1, without effects on the levels of other ROS [80]. However, in contrast to flu, ¹O₂ production at PS II in ch1 occurs in chloroplasts in stacked membranes of grana cores [80], and not in grana margins or in etioplasts as in flu [28].

Gene expression profiles in leaves of ch1 and flu after light stress showed high similarity: of more than 2600 genes with changed expression profiles in ch1, 80% showed a similar response in flu [80]. However, in contrast to flu, in ch1 EX1 does not participate in the onset of PCD [80]. In ch1, ¹O₂-dependent PCD involves a serine-threonine kinase OXIDATIVE SIGNAL INDUCIBLE1 (OXI1), which was previously shown to regulate H₂O₂-mediated processes including those related to the response to pathogens [94,95]. In a ch1/oxi1 double mutant, high light leads to ¹O₂ generation but not to PCD [94]. OXI1 signaling involves phytohormones: expression of genes encoding enzymes involved in JA and SA biosynthesis is strongly increased in plants overexpressing OXI1 (OE-OXI1) even in the absence of light stress, while in an oxi1 knockout mutant the levels of SA, but not JA, were decreased [95]. Only a small number of genes is activated both during OXI-mediated and during EX1-mediated cell death [96]. Other genes induced in the ch1 mutant by high light are regulated by accumulation of hydroxyl-octadecatrienic acids due to ¹O₂-triggered lipid peroxidation [80].

Thus, ¹O₂ produced in stacked membranes of grana cores induces a specific type of cell death, namely OXI1-dependent PCD, while ¹O₂ produced at grana margins triggers EX1-dependent PCD. Both types of PCD depend on an increase in JA biosynthesis, which in turn activates the biosynthesis of SA triggering PCD. Importantly, these pathways differ from those activated during plant defense: Upon attack of necrotrophic pathogens, JA suppresses cell death induced by the release of O₂^•− and H₂O₂. However, JA induces ¹O₂-dependent PCD during light stress. Although these data were obtained for flu and ch1 mutants, the corresponding signaling pathways were shown to function also in Arabidopsis wild-type plants. In extreme stress, for instance, when very high illumination is combined with cold temperature, wild-type plants show PCD mediated by OXI1 kinase and not by EX proteins [94].

Notably, exposure of ch1 plants to moderate light intensities before their transfer to high light prevents induction of OXI and the development of PCD [80,94]. Thus, ch1 plants can become acclimated to high light stepwise. The key component of the acclimation was shown to be an endoperoxide of β-carotene, β-cyclocitral, which is produced in PS II during an increase in ¹O₂ levels. This process might include also other ¹O₂-specific products of the oxidation of β-carotene, for instance, dihydroactinidiolide [75,76]. The acclimation includes the activation of genes encoding regulators of biosynthesis of plastoquinone and ubiquinone, anthocyanin and flavonoids, pyridoxine and methionine, and of other compounds which show a high reactivity with ¹O₂ [80]. Acclimation also leads to a decrease in expression levels of the genes encoding proteins related to mechanical damage as well as some transcription factors and proteins related to photosynthesis [80].

Of special interest is the inhibition of the expression of genes encoding enzymes involved in JA synthesis during the acclimation of ch1 to high light, as it contrasts sharply with the high expression levels of these genes in leaves of ch1 in high light. Acclimation was shown to involve the transcriptional regulators METHYLENE BLUE SENSITIVITY 1 (MBS1) [76] and SCARECROW LIKE14 (SCL14) [97], which are responsible for the inhibition of transcription of genes of JA synthesis and the induction of genes regulating detoxification processes, respectively. Both MBS1 and SCL14 are induced by β-cyclocitral, which is a sensor of light excess and of the increase in charge recombination in PS II. Interestingly, β-cyclocitral induces biosynthesis of SA during acclimation, but this does not lead to PCD [98].

Altogether, signaling pathways initiated by ¹O₂ and mediated by EX1/EX2 differ from those mediated by OXI1 or β-cyclocitral, respectively (Figure 5). These differences are probably based on the short lifetime and high reactivity of ¹O₂. It is assumed that ¹O₂ cannot diffuse over a distance longer than a half of grana length (approx. 250 nm; Figure 6). Thus, ¹O₂ production at grana margins probably does not influence the oxidation of β-carotene in PSII reaction centers located in grana cores, while ¹O₂ produced at grana cores does not reach grana margins to induce EX1 degradation. Recently, a novel ¹O₂-activated signaling pathway has been revealed which recognizes damaged chloroplasts and leads to their ubiquitinylation and rapid degradation [99]. A cytoplasmic E3-ubiquitin-ligase PUB4 (plant U-box 4) “marks” chloroplasts with enhanced levels of ¹O₂ production, ensuring maintenance of the population of physiologically active chloroplasts in the mesophyll [100,101] (Figure 5). These data were obtained using Arabidopsis fc2 mutants with defects in plastidial ferrochelatase 2. These plants accumulated high levels of protoporphyrin IX leading to the generation of ¹O₂ in the light [99]. Interestingly, there was no activation of EX1-dependent signaling, although it can be assumed that the accumulation of protoporphyrin IX, and therefore the generation of ¹O₂, in fc2 plants occurs close to the complex containing Mg²⁺-protoporphyrin IX monomethyl-ester-cyclase, i.e., at grana margins. Notably, PUB4-mediated degradation of chloroplasts occurs much faster than chlorophagy [101].

Importantly, the local production of ¹O₂ in one of the leaves, or in a part of a leaf, of mature Arabidopsis plants induces the systemic acclimation to stress in the whole plant [102]. Thus, the influence of ¹O₂ on plants extends far beyond the chloroplasts where it is generated.

8. Role of ¹O₂ in Development of PCD in Plants

As already discussed above, ¹O₂ fulfils at least two signaling roles in plants: in the acclimation to excess light conditions, and in the induction of PCD [103]. While the first role is specific to leaves, the second role has been detected also in roots of Arabidopsis thaliana [59]. Here, ¹O₂-induced PCD of apical meristems might cause an increase in lateral root formation, which is a common response to many abiotic stresses experienced by roots [59]. It can be speculated that in leaves, ¹O₂-triggered OXI1-dependent PCD might represent the outcome of an unsuccessful adaptive response, while ¹O₂-triggered EX1-dependent PCD might provide an emergency pathway for elimination (often leading to the formation of microlesions on leaves) of leaf cells accumulating highly dangerous chlorophyll precursors/metabolites in an uncontrolled fashion [103,104]. An important but probably underestimated, and clearly not sufficiently studied, function of ¹O₂-induced PCD might be the participation in the hypersensitive response during pathogen attack [103,105]. ¹O₂-triggered PCD has been described also in photosynthesizing suspension cell cultures of Arabidopsis [106]. Altogether, more research is necessary to understand the physiological roles of ¹O₂-induced PCD in plants.

Neither the exact source of ¹O₂ nor the components of the signal transduction pathway involved in ¹O₂-triggered PCD induction are known for roots. The best characterized ¹O₂ signaling pathways in leaves are mediated by OXI1 and EX1, respectively; recently, a novel route involving the SAFE1 protein was suggested [91]. Notably, while EX1 and SAFE1 are chloroplastic proteins, OXI1 kinase is expressed not only in leaves but also in roots and plays a role in root hair growth and in the oxidative burst [107]. Transduction of ¹O₂ signals leading to the induction of PCD involves JA and SA: synthesis of both groups of phytohormones increases in the course or OXI1- or EX1-mediated PCD, respectively. JA plays a key role in the ¹O₂-signaling cascades leading to PCD in both flu and ch1 mutants, and the choice between PCD and acclimation to ¹O₂ also depends on this phytohormone [108]. Interestingly, 12-oxophytodienoic acid (OPDA), the precursor of JA, has an antagonistic effect on PCD initiated by JA in Arabidopsis suspension cell cultures [106]. ¹O₂-induced PCD requires the synthesis of SA in both flu and ch1 mutants [88,109]. However, addition of the photosensitizer Rose Bengal to photosynthesizing Arabidopsis suspension cell cultures during moderate light stress elicited JA- and ethylene-dependent PCD while the EDS1 protein was not involved, suggesting that SA signaling was not required [106]. Ethylene signaling was also suggested to take part in the ¹O₂-mediated PCD in leaves [106,108].

It should be noted that there is evidence for cross-talk between ¹O₂-signaling and signaling networks related to other ROS: for instance, reduced ROS antagonize ¹O₂-mediated signaling which eventually can lead to the delay of PCD [110]. Sabater and Martin [111] hypothesized that the ratios between different ROS might be translated into changes in the JA/H₂O₂ ratio, and thus could influence the choice between the activation of the defense response vs. PCD response.

Cytological characteristics of ¹O₂-mediated PCD were investigated using plants with modified levels of protochlorophyllide oxidoreductase C, namely porC-2 (mutant lacking PORC and overaccumulating Pchlide) and PORCx (plants overexpressing porC-2) [112]. This study allowed minimization of the production of ROS other than ¹O₂ by using low levels of light. Treatment with 5-aminolevulinic acid caused blebbing of the plasma membrane and DNA breaks (revealed by TUNEL-positive nuclei), both hallmarks of apoptosis, in protoplasts of wild-type and porC-2 plants [112]. While the low amounts of ¹O₂ produced in PORCx protoplasts under experimental conditions were not sufficient to initiate PCD, after prolonged exposure to light, PCD occurred also in PORCx protoplasts [112].

Interestingly, an increase in ¹O₂ production did not lead to cell death in the Arabidopsis npq1lut2 double mutant lacking the LHC carotenoids zeaxanthin and lutein [113]. At the same time, the ABA deficient mutant aba1 lacking zeaxanthin deepoxidase and deficient in two other LHC carotenoids, violaxanthin and neoxanthin, was shown to produce ¹O₂ leading to cell death under high light [110]. During ¹O₂-mediated cell death in aba1 plants, chloroplasts aggregated at the center of the cells; such aggregation is regarded as a step preceding their autophagic degradation [110]. Disruption of chloroplasts was also detected [110].

Thus, light and chloroplasts are of high significance for ¹O₂-mediated PCD in leaves: First, ¹O₂ is mainly produced in chloroplasts in the light; second, such key regulators of ¹O₂-signaling pathways as EX1 and SAFE1 are located in chloroplasts; third, the phytohormones JA and SA regulating ¹O₂-mediated PCD are synthesized in chlotoplasts. Nevertheless, PCD is a whole-cell process involving other cell compartments. For instance, it was shown that during pathogen treatment, the red-chlorophyll-catabolite can move from chloroplasts to mitochondria and induce ¹O₂-dependent PCD in mutants lacking the ACCELERATED CELL DEATH2 protein [105]. A recent study using the ceh1 mutant impaired in isoprenoid synthesis revealed another important player of ¹O₂-mediated PCD, the endoplasmic reticulum (ER)-mediated unfolded protein response (UPR) [109]. The UPR is a stress reaction activated in response to the accumulation of aggregates of unfolded and misfolded proteins inside the ER lumen (ER stress) which aims at the restoration of normal ER functions but can elicit PCD if the adaptation was unsuccessful. The role of the URP in ¹O₂-mediated PCD was further confirmed using ch1 mutants [109]. In ch1, expression of UPR genes was found to be constitutively enhanced compared to the situation in wild type plants, and increased further under high light conditions, eventually leading to cell death. Thus, a moderate UPR served as part of the acclimatory response of ch1 plants to ¹O₂, and a strong activation of the whole UPR was associated with cell death [109]. Notably, some of UPR-related genes induced in ch1 were also induced in the flu mutant [109]. It has been shown that URP in plants is regulated by SA [114]. The exact mechanisms of interaction of chloroplasts and ER during ¹O₂-mediated PCD remain unknown, but it is proposed that the involvement of the ER in ¹O₂ signaling might be mediated via direct contacts between ER and chloroplasts. Chloroplasts are known to form fine protrusions of stroma, called stromules, into the cytoplasm, especially under high levels of ROS production [115]. The ER also has specific membrane extensions, which might connect to stromules [109].

A recent study showed that ¹O₂ produced in the vacuole or at the plasma membrane can be involved in vacuole-mediated PCD [116]. In leaves of Arabidopsis, ¹O₂ generation was induced either by Rose Bengal or by Acridine Orange, which localized to the plasma membrane or to the vacuole, respectively. Photoactivation of both photosensitizers led to induction of PCD of the vacuolar type, but the patterns were different. Disruption of the tonoplast was observed only when ¹O₂ was generated by vacuolar Acridine Orange. This process was accompanied by a release of RESPONSIVE TO DESSICATION-21 (RD21) protease into the cytoplasm, its binding to the protective protein AtSerpin and strong acceleration of PCD [116]. Although these data were obtained with artificial photosensitizers, the same study showed that a similar mechanism can operate in leaf cells during acute water stress [116].

Hence, the initiation of PCD by ¹O₂ evolved from chloroplasts, as well as from other cellular compartments, both in leaves and in non-photosynthetic plant organs is a highly intricate and not yet understood process. A picture is emerging that there are several signaling pathways transducing the ¹O₂-triggered PCD signal into the nucleus, which can interact and compete. Our current understanding of molecular and cytological mechanisms of ¹O₂-mediated PCD remains incomplete.

9. Detection of ¹O₂ in Plants

¹O₂ was discovered by Hans Kautsky [117] who noticed that chlorophyll fluorescence in living cells was lower than in chlorophyll extracts and was rapidly quenched. The reason was in vivo quenching of chlorophyll fluorescence by oxygen accompanied by energy transfer and formation of ¹O₂ [118]. As the lifetime of ¹O₂ and its diffusion distance are very short, the specific tracers and quenchers used for ¹O₂ detection should be able to access the sites of ¹O₂ generation within the cells as closely as possible [77].

The sites and the levels of ¹O₂ production in plant cells can be revealed on the basis of specific ¹O₂ reaction products (for instance, lipid peroxidation products) or using specific quenchers like sodium azide or histidine. However, these methods are indirect and the results are equivocal [46]. Direct detection of ¹O₂ as well as the estimation of its concentration and time dynamics in a biological environment is a complicated task [119]. Without reactions, ¹O₂ returns to its ground state by emission of light of about 1270 nm. Unfortunately, the 1268 nm peak is positioned on the declining spectral component of chlorophyll phosphorescence which makes any quantification impossible [31].

The most selective method of ¹O₂ detection is electron paramagnetic resonance (EPR) spectroscopy. EPR spectroscopy detects free radicals; therefore, identification of ¹O₂ is based on spectral characteristics of special “trapping” molecules forming radicals after interaction with ¹O₂. In 1976, TEMP (2,2,6,6-tetramethylpiperidine) was proposed as a trap for ¹O₂ detection [120]. As a strong electrophile species, ¹O₂ can oxidize TEMP to its stable N-oxyl radical TEMPO (2,2,6,6-tetramethylpiperidine-1-oxyl) which can be detected with EPR spectroscopy [31,38]. Unfortunately, this technique cannot be used for ¹O₂ detection in plants in vivo due to the high sensitivity of nitroxide-radicals to reductants, especially those produced in illuminated thylakoids. Moreover, the relatively high water contents in leaves also interfere with EPR-based methods [33].

To date, a very convenient way to detect sites and levels of ¹O₂ generation in plants is provided by specific fluorescent probes which change their properties after reaction with ¹O₂ [121,122]. In leaves, ¹O₂ generation in chloroplasts in the light can be traced using a fluorescing spin probe DanePy which exhibits bright fluorescence in the absence of ¹O₂ but becomes progressively quenched by ¹O₂ in a quantitative manner. Experiments with DanePy using photoinhibited isolated thylakoid membranes showed that the light-induced quenching of DanePy fluorescence is specific to ¹O₂ [33]. Another commercially available probe is Singlet Oxygen Sensor Green (SOSG) which is highly selective for ¹O₂ and does not change fluorescence upon interaction with O₂^•− or OH^• [123]. In the absence of ¹O₂ SOSG displays a weak blue fluorescence with excitation peaks at 372 nm and 393 nm, and emission peaks at 395 nm and 416 nm. In the presence of ¹O₂ SOSG shows bright green fluorescence with excitation and emission peaks at 504 nm and 525 nm, respectively [27]. Reaction of SOSG with ¹O₂ leads to formation of SOSG endoperoxide. Intramolecular transfer of electrons quenches the fluorescence of the SOSG chromophore before reaction with ¹O₂ while formation of the endoperoxide prevents electron transfer, and SOSG fluorescence can be observed [123].

A drawback of SOSG is its ability to function as photosensitizer after illumination with UV light or after prolonged exposure to high light, thus promoting ¹O₂ formation [124]. However, even under these conditions the levels of SOSG fluorescence caused by photosensitization effects are much lower than the levels of ¹O₂ production in plants in vivo [94]. This, as well as the high specificity for ¹O₂ [123], sensitivity and convenient detection methods (in contrast to DanePy whose fluorescence is quenched by ¹O₂, SOSG fluorescence increases proportional to ¹O₂ levels) explain the increasing use of SOSG.

Usually, a buffered SOSG solution with a final concentration of 5–100 µM is introduced into leaves or seedlings by means of vacuum-infiltration [94,125]. SOSG was described as not being able to penetrate cell membranes [126]; however, other authors reported that in high concentrations, SOSG can enter cells and accumulate in the nucleus [121,122]. Nevertheless, infiltration of low concentrations of SOSG in leaves, i.e., into the leaf intercellular space where it comes in contact with the apoplastic water phase, seems to represent a convenient method to study ¹O₂ generation in chloroplasts. It should be taken into account that in mesophyll cells, chloroplasts are situated very close to plasma membrane and cell walls: the diffusion distance for ¹O₂ from chloroplasts to SOSG in the apoplast is about 200 nm (Figure 6). The lifetime of ROS in the apoplast is much longer than inside cells due to the absence of most antioxidant systems [74]. Accumulation of fluorescent SOSG in infiltrated leaves in the light allows estimation of the levels of ¹O₂ production and performance of quantitative and semi-quantitative evaluations (see, for instance, [50,76,124]).

Another tool used for studies of ¹O₂ production in plants are non-fluorescent quenchers like DABCO (1,4-diazabicyclo[2.2.2]octane, or triethylenediamine TEDA) [127,128] and 2,2,5,7,8-pentamethyl-6-chromanol (PMC) [129]. DABCO is a nucleophilic aliphatic quaternary amine often used in mounting kits for fluorescent microscopy as an antifading agent. PMC is a lipophilic analog of α-tocopherol able to quench ¹O₂ and lipid peroxyl radicals [130,131]. Both DABCO and PMC are highly effective ¹O₂ quenchers [132]. A disadvantage of DABCO is that its cross-reactivity with other ROS is not fully understood, while PMC is not very specific to ¹O₂ and reacts also with superoxide radical [133], ozone [134] and NO [135]. Nevertheless, DABCO and PMC were used in studies of the role of ¹O₂ during salt stress-induced PCD in tobacco suspension cells and in the halophyte Cakile maritima [127,128].

A very convenient and sensitive method of ¹O₂ detection is based on in vivo imaging of whole plants for the detection of autoluminescence. Autoluminescence arises due to spontaneous photon emission (SPE) during decomposition of lipid hydroperoxides and endoperoxides produced via lipid oxidation by ¹O₂ or triplet carbonyls [136,137,138,139]. SPE occurs at an intensity several orders lower than that of bioluminescence and has a long relaxation period of up to several hours. The equipment for detection of autoluminescence includes a high-sensitivity cooled CCD camera, a 50-mm focal lens and a set of color filters for the analysis of the spectral characteristics of the autoluminescence [139]. Autoluminescence imaging allows non-invasive quantitation of early symptoms of oxidative stress in plants which can be detected much earlier than visual signs such as chlorophyll bleaching or turgor loss (e.g., [75,76,94,95]).

10. Conclusions

Photochemistry and photophysics of ¹O₂ constantly and significantly influence plants’ lives. Along with other ROS, ¹O₂ is a central component of plant response to stress, and its levels and sites of production can determine the type of response: acclimation vs. programmed cell death. Studies of mechanisms, sites and regulation of ¹O₂ formation in plants, as well as understanding of signaling pathways activated by ¹O₂, is of high importance for basic and applied research; for instance, results of such studies allowed the development of effective herbicides [10]. Now, it is important to extend the knowledge obtained using Arabidopsis to other plant species including crops. The levels of ¹O₂ generation affect plants’ adaptation to environmental factors, most prominently to two of them, light and biotic stress induced by pathogens. Studies of interactions between signaling pathways regulated by ¹O₂ and by photoreceptors, respectively, as was shown for CRY1 in Arabidopsis, might reveal new aspects of the role of ¹O₂ in plant acclimation to light conditions, and allow optimization of light conditions in greenhouses.