- Research article
- Open Access
Photoinhibition and photoinhibition-like damage to the photosynthetic apparatus in tobacco leaves induced by pseudomonas syringae pv. Tabaci under light and dark conditions
BMC Plant Biology volume 16, Article number: 29 (2016)
Pseudomonas syringae pv. tabaci (Pst), which is the pathogen responsible for tobacco wildfire disease, has received considerable attention in recent years. The objective of this study was to clarify the responses of photosystem I (PSI) and photosystem II (PSII) to Pst infection in tobacco leaves.
The net photosynthetic rate (Pn) and carboxylation efficiency (CE) were inhibited by Pst infection. The normalized relative variable fluorescence at the K step (W k) and the relative variable fluorescence at the J step (V J) increased while the maximal quantum yield of PSII (F v/F m) and the density of Q A-reducing PSII reaction centers per cross section (RC/CSm) decreased, indicating that the reaction centers, and the donor and acceptor sides of PSII were all severely damaged after Pst infection. The PSI activity decreased as the infection progressed. Furthermore, we observed a considerable overall degradation of PsbO, D1, PsaA proteins and an over-accumulation of reactive oxygen species (ROS).
Photoinhibition and photoinhibition-like damage were observed under light and dark conditions, respectively, after Pst infection of tobacco leaves. The damage was greater in the dark. ROS over-accumulation was not the primary cause of the photoinhibition and photoinhibition-like damage. The PsbO, D1 and PsaA proteins appear to be the targets during Pst infection under light and dark conditions.
Under natural conditions, in addition to abiotic stresses, plants are exposed to various biotic stresses, including infection by pathogens and attack by herbivorous pests [1, 2]. Biotic stresses decrease crop yields worldwide by an average of 15 % . Compared with the number of studies on plant infections caused by fungi and viruses, there are relatively few regarding plants infected by bacteria . The effects of bacterial pathogens infection depends on the severity and timing of infection, but also on the particular type of bacteria and on genotype-associated host resistance [5, 6]. Bacterial infections strongly affect photosynthesis. In fact, it has been reported that the genes encoding photosynthetic functions are down regulated [7–9] and changes to photosystem II (PSII) proteins occur in Pseudomonas syringae-infected plants .
Pseudomonas syringae are opportunistic bacterial pathogens that can attack a wide variety of plants . There are at least 50 P. syringae pathovars based on their host plant specificities and type of disease symptoms [12, 13]. Previous research has revealed that the maximum PSII quantum yield (F v /F m), the quantum yield of open PSII traps (F v’/F m’), and nonphotochemical quenching (NPQ) were decreased in Arabidopsis thaliana leaves infected with P. syringae pv. tomato DC3000 (Pto) [14, 15]. Decreases in the actual photochemical efficiency of PSII (ΦPSII) and NPQ were also observed in Pto-infected Phaseolus vulgaris leaves . Additionally, a decrease in NPQ was observed in P. syringae pv. Phaseolicola (Pph)-infected bean plants, while the F v /F m remained stable . Moreover, decreases in ΦPSII and NPQ were detected in Pph-infected ‘Canadian Wonder’ P. vulgaris leaves . In contrast, a decrease in F v’/F m’ and an increase in NPQ were observed in soybean leaves infiltrated with P. syringae pv. glycinea . As one of the most important pathovars, P. syringae pv. tabaci (Pst) is a hemibiotrophic bacterial pathogen that parasitizes tobacco leaves, causing the formation of brown spots during an infection referred to as wildfire disease [18, 19]. To better understand how to manage P. syringae infections, we focused on the tobacco-Pst model pathosystem. Although considerable research has recently been completed on the tolerance to Pst [20–22] and the photosynthetic performance of plants infected by the other pathovars mentioned above, little information is available on the photosynthetic performance during tobacco-Pst interactions.
The D1 protein is the core protein of the PSII reaction center. The inhibition of photosynthesis electron transport (PET) from the primary quinone electron acceptor of PSII (Q A) to the secondary quinone electron acceptor of PSII (Q B) may consequently be related to the degradation of the D1 protein . Similarly, PsbO, the core component of the oxygen evolving complex (OEC), is critical to the functionality of the OEC . Additionally, photosystem I (PSI) photoinhibition is related to the degradation of PsaA . In several studies, dark conditions were simulated using the PET inhibitors 3-(3,4-dichlorophenyl)-1,1-dimethylurea and 2,5-dibromo-3-methyl-6-isopropylbenzoquinone [26, 27]. However, this study focused on PET as influenced by Pst infection. Therefore, these inhibitors were not used.
Our objectives were to identify the differences in PSI and PSII responses to light and dark conditions following Pst infection of tobacco leaves. We also aimed to determine if photoinhibition occurs during Pst infection. To address these questions, we (1) evaluated the changes to the donor and acceptor sides and the reaction center of PSII as well as the PSI activity after Pst infection, (2) monitored the production of reactive oxygen species (ROS), and (3) performed Western blot analyses of the thylakoid membrane proteins of treated tobacco leaves. We compared the responses of the photosynthetic apparatus to Pst infection under light and dark conditions.
Effects of Pst infection on chlorophyll content in the infiltrated area of tobacco leaves
We observed chlorotic lesions in the infiltrated zone at 3 days post infection (dpi), while necrosis was observed at 3 dpi only in leaves treated in the dark. The infiltrated zone of tobacco leaves exhibited obvious wildfire symptoms regardless of whether the leaves were incubated under light or dark conditions (Fig. 1). The total chlorophyll content in infected leaves at 3 dpi was lower than that of untreated leaves (Fig. 2).
Effects of Pst infection on the donor and acceptor sides and the reaction center of PSII in tobacco leaves
We used the JIP-test to detect PSII changes in Pst-infected tobacco leaves under light and dark conditions. To clarify the effects of Pst on PSII, OJIP curves were normalized to the (F m − F o) level. The shape of the OJIP transient changed over time, with the K and J points increasing markedly and the amplitude increasing along with the inoculation time (Fig. 3). The K step (at 300 μs) of the chlorophyll a fluorescence transient (quantified as W K) has been widely used as a specific indicator of oxygen evolving complex (OEC) injury in the photosynthetic apparatus [28, 29]. We observed that W K increased after Pst infection under light and dark conditions. The increase was more pronounced with increasing time, suggesting that the activity of the donor side of PSII was inhibited and that the OEC was damaged. Compared with that of untreated leaves, W k increased by 12.9 and 25.6 % at 3 dpi under light and dark conditions, respectively (Fig. 4a, b). The relative variable fluorescence at the J-step (V J) represents the subsequent kinetic bottleneck of the electron transport chain, resulting in the momentary maximum accumulation of Q A − [30, 31]. V J is an indicator of the level of closure of PSII reaction centers or the redox state of Q A . In this study, compared with untreated leaves, V J increased by 13.9 and 103 % in the infiltrated zone at 3 dpi under light and dark conditions, respectively (Fig. 4c, d). Thus, electron transport from Q A to Q B was severely blocked after Pst infection in tobacco leaves. Moreover, inhibition of the K and J steps was more pronounced in the dark, as indicated by the greater increase of the W k and V J values in the dark during Pst inoculation (Fig. 4a-d). The maximum quantum yield of PSII (F v/F m) and the density of Q A − reducing PSII reaction centers per cross section (RC/CSm) values decreased to 94.7 nd 85.4 % of the values of untreated leaves (under light conditions) at 3 dpi, respectively (Fig. 4e, g). The F v/F m and RC/CSm values of treated leaves decreased to 91.9 and 66.8 % of the values of untreated leaves (under dark conditions) at 3 dpi, respectively (Fig. 4f, h).
Effects of Pst infection on PSI complex activity in tobacco leaves
We observed considerable differences in PSI activity among treated leaves. The PSI complex activities of treated leaves were 80.0 and 70.8 % of the activity of untreated leaves at 3 dpi under light and dark conditions, respectively (Fig. 5). This indicates that P700 photo-oxidation was rapidly and effectively impaired by Pst infection in tobacco leaves under light and dark conditions. Further, the extent of the decrease in PSI activity was greater in the dark (Fig. 5).
Effects of Pst infection on carbon assimilation in tobacco leaves
The net photosynthetic rate (Pn), stomatal conductance (Gs), and carboxylation efficiency (CE) values of treated leaves were 69.3, 17.5, and 21.1 % lower than those of mock controls at 3 dpi, respectively. In contrast, the intercellular CO2 concentration (Ci) value of treated leaves was 23.6 % higher than that of mock controls at 3 dpi (Table. 1).
Relative ROS level changes after Pst infection in tobacco leaves
We evaluated H2O2 production in the Pst-infiltrated zone of tobacco leaves at 3 dpi under light and dark conditions because H2O2 is the most stable ROS that can be readily measured . The production of H2O2 was evaluated in the Pst-infiltrated zone of tobacco leaves at 3 dpi under light and dark conditions. The H2O2 content of treated leaves were 269 and 112 % higher than that of untreated controls at 3 dpi under light and dark conditions, respectively (Fig. 6). This implies that an over-accumulation of ROS was induced by Pst infection in tobacco leaves under light and, to a lesser extent, dark conditions.
Pst-induced degradation of PsbO, D1, and PsaA proteins in tobacco leaves
The D1 protein pool sizes is representative of the abundance of fully assembled PSII centers as there is one D1 subunit per reaction center. The mature protein is thought to accumulate only when it is integrated into PSII reaction centers. The content of PsbO, D1, and PsaA proteins decreased to 67.0, 65.1 and 70.0 % of the values of water-treated leaves at 3 dpi under light conditions, respectively. The core proteins decreased to 44.1, 51.0 and 50.2 % of the values of water-treated leaves at 3 dpi under dark conditions, respectively (Fig. 7).
We observed lesions consisting of a necrotic center surrounded by chlorotic tissue at 3 dpi in the dark (Fig. 1). Plant pathogens can generally be categorized in three classes (necrotrophs, biotrophs, and hemibiotrophs) on the basis of mechanisms of infection. Biotrophics need living tissue for growth and reproduction. Necrotrophics kill the host tissue during the initial stages of infection and feed on the dead tissue. Hemi-biotrophics exist as biotrophs before switching to a necrotrophic stage .
Our study revealed that chlorophyll content decreased considerably during Pst inoculation under light and dark conditions (Fig. 2). Chlorophyll degradation has been observed in several plant − pathogen interactions [35, 36]. Kudoh and Sonoike reported that in the early recovery stage after PSI damage, chlorophyll degradation occurred to prevent the absorption of excessive light energy which can otherwise lead to secondary injury of the photosystems . Moreover, Thomas reported that tabtoxinine-β-lactam, a toxin originally described as being from Pst, is a dipeptide whose hydrolysis product irreversibly inhibits glutamine synthetase and induces chlorophyll degradation in tobacco leaves . Therefore, the putative tabtoxin activity of Pst and the need for photoprotection of the tobacco leaves after PSI damage may have been responsible for the observed chlorophyll degradation.
The reduction of Pn in leaves may have been due to limited CO2 diffusion to carboxylation sites as a consequence of decreased stomatal conductance or because of perturbation of enzymatic processes in the Calvin cycle . The decreased Gs and the increased Ci in the Pst infiltrated leaves (Table 1) indicated that the decrease in Pn may be the result of a non-stomatal limitation. The decrease in CE (Table 1) indicates that the ribulose 1, 5-bisphosphate carboxylase/oxygenase activity may be inhibited by Pst infection, leading to the inhibition of CO2 assimilation. Photosynthetic electron transport and carboxylation were both inhibited by Pst infection. However, it is unclear whether the effects on PET are the result of inhibition of downstream carboxylation.
The phosphoenolpyruvate carboxylase (EC 220.127.116.11, PEPc) catalyses the irreversible β-carboxylation of phosphoenolpyruvate using HCO3 − as a substrate in a reaction that yields oxaloacetic acid and inorganic phosphate . Several papers have shown that PEPc activity increased in salt treated Sorghum bicolor (a C4 plant), Hordeum vulgare (a C3 plant) and Aleuropus litoralis (a C3-C4 intermediate plant) [41–43]. The activity of PEPc increased after Potato virus Y or Potato virus A infection in tobacco leaves [44, 45]. This stimulation of PEPc activity under biotic and abiotic stresses would allow replenishment of the tricarboxylic acid cycle to maintain the activated internal nitrogen metabolism in spite of the reduced photosynthesis rate .
The decreases in F v/F m and RC/CSm are conventional indicators of photoinhibition under light conditions . The F v/F m and RC/CSm values decreased considerably as the Pst infection progressed (Fig. 4), suggesting that Pst infection causes photoinhibition of PSII under light conditions.
Photosystem II is considered to be more vulnerable than PSI when plants encounter stresses because few species have been found in which PSI is more easily photoinhibited than PSII [48, 49]. Photoinhibition of PSI was first reported by Terashima et al. in cucumber plants exposed to low temperature . The PSI activity decreased after Pst infection (Fig. 5), indicating that PSI photoinhibition occurred during Pst inoculation under light conditions. However, we observed damages to the photosynthetic apparatus during Pst inoculation under dark conditions that were similar to the damage caused by photoinhibition induced by light. Therefore, this damage was referred to as “photoinhibition-like damage” which was further indicated by the degradation of PsbO, D1, and PsaA proteins (Fig. 7).
Chloroplasts are the major source of ROS in plant cells. The direct reduction of O2 to superoxide by reduced donors associated with PSI occurs during the Mehler reaction . The impairment of photosystems inevitably leads to the generation of ROS by the Mehler reaction during Pst inoculation (Fig. 6). There are two roles for H2O2 in plants. At low concentrations, it acts as a messenger molecule involved in signaling related to acclimation and the triggering of defense mechanisms against various stresses . At high concentrations, H2O2 promotes programmed cell death and oxidative damage . Additionally, H2O2 can suppress de novo D1 protein synthesis by inhibiting elongation factor G [54, 55]. Several reports have suggested that ROS over-production is involved in photoinhibition during various stresses [56, 57]. However, the observed damage to the photosystems was greater and the increase in H2O2 was much smaller in the dark than in the light (Fig. 6). These results suggest that ROS over-accumulation was not the main reason for the photoinhibition and photoinhibition-like damage induced by Pst in tobacco leaves. Additionally, PSI is likely to be attacked by ROS during exposure to stresses, but this attack occurs only if the reduced state of iron-sulfur centers can be maintained, which requires visible light . However, the damage to PSI was greater in the dark, further supporting the viewpoint mentioned above. In accordance with this, Fan et al. indicated that the photoinhibition-like damage of daylily, willow, euonymus japonicus and maize was not caused by the over-accumulation of ROS under dark conditions .
Counteracting to the negative effects of ROS on the photosynthetic apparatus during photoinhibition, the greater abundance of H2O2 under light conditions may have led to increased hydroxyl free radical production by the Fenton reaction. The hydroxyl radical may inhibit the pathogen under light conditions . This may be a positive effect of H2O2 that helped to alleviate photoinhibition and photoinhibition-like damage.
The production of ATP and NADPH during photosynthesis decreases in the dark . The replacement of damaged PSII proteins (primarily the D1 protein) with newly synthesized proteins is an ATP-dependent process . Additionally, the synthesis of the D1 protein of the PSII heterodimer, which is the most rapidly synthesized chloroplast protein, is stimulated by bright light . Therefore, the limited recovery of PSII under dark conditions may be one of the reasons for the greater overall damage observed in the dark during Pst inoculation. If a partially repaired PSII in the light minimized the overall damage to the photosystem, it is unclear why the damage to PSI was less extensive in the light than in the dark. The repair of PSI is a very slow process that requires several days or longer. Therefore, the results can not be related to PSI repair. Further studies are needed to clarify this point.
We evaluated the response of PSI and PSII to Pst infection in tobacco leaves under light and dark conditions. The reaction centers and the donor and acceptor sides of the photosystems were all severely damaged, indicating that photoinhibition and photoinhibition-like damage had occurred. We also observed a considerable (net) degradation of PsbO, D1, and PsaA proteins and an over-accumulation of ROS. The accumulated ROS, however, was not the main reason for the photoinhibition and photoinhibition-like damage induced by Pst in tobacco leaves. The PsbO, D1, and PsaA proteins appear to be the targets of Pst infection under light and dark conditions. Further investigations of photosystem responses may help to identify the main sites of Pst-induced damaged in tobacco leaves. This will lead to a better understanding of the mechanisms of plant-pathogen interactions and assist in the breeding of Pst-tolerant species.
Plant materials and infiltration with Pst
Seeds of tobacco (Nicotiana tabacum cv. Longjiang 911, a susceptible cultivar, was kindly supplied by Dr. Jian-Ping Sun, Tobacco Research Institute of Mudanjiang, Mudanjiang, China) were germinated on vermiculite. Forty-five days after germination, the seedlings were transplanted to pots containing a compost-soil substrate to grow in a greenhouse under a natural photoperiod. The two upper fully expanded attached leaves of six to eight weeks old plants were used for experiments.
Pseudomonas syringae pv. tabaci were grown on solid King’s B agar plates overnight , diluted with distilled water to a concentration 106 colony forming units per milliliter. Distilled water (mock) or bacterial suspensions were hand-infiltrated into mesophyll with a needleless syringe on the abaxial side of the leaves. Infiltrating area was about 1 cm−2 and measurements were made at a distance of about 0.5 cm from the infiltration area. Following inoculation, the leaves were kept under 14 h light (200 μmol m−2 s−1) /10 h dark cycles or continuous darkness at 25 °C.
Measurements of total chlorophyll content in tobacco leaves after Pst infection
Leaf total chlorophyll was extracted with 80 % acetone in the dark for 72 h at 4 °C. The extracts were analyzed using a UV-visible spectrophotometer UV-1601 (Shimadzu, Japan) according to the method of Porra (2002) .
Measurement of gas exchange in tobacco leaves after Pst infection
The Pn, Gs, and Ci were measured by a CIRAS-3 portable photosynthetic system (PP Systems, USA), which controls the photosynthetic photon flux density at 800 μmol m−2 s−1, temperature at 25 °C and CO2 concentration at 390 μmol mol−1 in the leaf chamber. CO2 concentration was changed every 3 min in a sequence of 1 600, 1 200, 800, 600, 400, 300, 200, 150, 100 and 0 μmol mol−1. Irradiance and CO2 concentration were controlled by the automatic control function of the system. CE was calculated according the initial slop of Pn-Ci response curve .
Measurements of the chlorophyll a fluorescence transient (OJIP) and PSI activity in tobacco leaves after Pst infection
Induction kinetics of prompt fluorescence and the modulated reflected signal of 820 nm (MR820 nm) were simultaneously recorded using a Multifunctional Plant Efficiency Analyzer, M-PEA (Hansatech Instrument Ltd., UK) as has been described . All leaves were dark adapted before measurements. Chlorophyll a fluorescence transients were analyzed with the JIP-test: F v/F m = 1− (F o / F m); V J = (F2 ms − Fo) / (Fm − Fo); W k = (F 0.3 ms − F o) / (F 2 ms − F o); RC/CSm = φPo · (V J / M o) • (ABS / CSm), and Mo = 4 (F 0.3 ms − F o) / (F m − F o); φPo = F v/F m. The MR820 nm signal measured at 820 nm provides information about oxidation state of PSI, including plastocyanin and P700. The induction curve of MR820 nm of the leaves obtained by saturating red light showed a fast oxidation phase and a subsequent reduction phase. The initial slope of the oxidation phase of MR820 nm at the beginning of the saturated red light indicates the capability of P700 to get oxidized, which is used to reflect the activity of PSI [68, 69].
Detection of H2O2 generation in tobacco leaves after Pst infection
H2O2 was extracted and determined according to the method of Patterson . Leaf segments (0.5 g) were ground in liquid nitrogen, extracted with 5 ml of 5 % (w / v) trichloroacetic acid and then centrifuged at 16 000 × g for 10 min. The supernatant was used for the H2O2 assay.
Detection of Psb O, D1, and PsaA proteins in tobacco leaves after Pst infection
Thylakoid membranes proteins were detected by Western blot with equal amounts of chlorophyll. Leaves were homogenized in an ice cold isolation buffer [100 mM sucrose, 50 mM Hepes (pH 7.8), 20 mM NaCl, 2 mM EDTA and 2 mM MgCl2], then filtered through three layers of pledget. The filtrate was centrifuged at 3000 × g for 10 min. The sediments were washed with isolation buffer, re-centrifuged, and then finally suspended in an isolation buffer. The thylakoid membrane proteins were then denatured and separated using 12 % polyacrylamide gradient gel. The denatured proteins in the gel were then electro-blotted to PVDF membranes, probed with antibodies supplied by Fan et al.  and then visualized by a chemiluminescence method. Quantitative image analysis of protein levels was performed with Gel-Pro Analyzer 4.0 software.
Chemicals used in the study
All the compounds used in this study were manufactured by Sigma.
The results presented were the means of at least three independent measurements. Means were compared by analysis of variance and LSD range test at 5 % level of significance.
Availability of data and materials
All the supporting data are included as additional files.
Intercellular CO2 concentration
Days post infection
- F o :
F m, Initial and maximum fluorescence
- F v /F m :
Maximal quantum yield of PSII
- F v’/F m’:
The quantum yield of open PSII traps
K, Intermediate steps of chlorophyll a fluorescence rise between F o and F m
- MR820 nm :
Modulated reflected signal of 820 nm
The modified red-edge ratio
Oxygen evolving complex
Photosynthesis electron transport
Net photosynthetic rate
- Pph :
Pseudomonas pv. Phaseolicola
- Pst :
Pseudomonas syringae pv. tabaci
- Pto :
Pseodomonas syringae pv. tomatao DC300
- Q A :
The primary quinone electron acceptor of PSII
- Q B :
The secondary quinone electron acceptor of PSII
Density of Q A − reducing PSII reaction centre
Reactive oxygen species
- V J :
The relative variable fluorescence at the J step
- V t :
The relative variable fluorescence at the any time
- W K :
Normalized relative variable fluorescence at the K step
- ΦPSII :
The actual photochemical efficiency of PSII
Atkinson NJ, Urwin PE. The interaction of plant biotic and abiotic stresses: from genes to the field. J Exp Bot. 2012;63(10):3523–43.
Berger S, Sinha AK, Roitsch T. Plant physiology meets phytopathology: plant primary metabolism and plant–pathogen interactions. J Exp Bot. 2007;58(15–16):4019–26.
Oerke EC, Dehne HW. Safeguarding production losses in major crops and the role of crop protection. Crop Prot. 2004;23(4):275–85.
Barón M, Flexas J, DeLucia E H. Photosynthesis responses to biotic stress. En: Terrestrial photosynthesis in a changing environment. A molecular, physiological and ecological approach. Ed. J. Flexas, F. Loreto and H. Medrano. Cambridge:Cambridge Press; 2012. p. 331–350.
McElrone AJ, Forseth IN. Photosynthetic responses of a temperate liana to Xylella fastidiosa infection and water stress. J Phytopathol. 2004;152(1):9–20.
Berova N, Di Bari L, Pescitelli G. Application of electronic circular dichroism in configurational and conformational analysis of organic compounds. Chem Soc Rev. 2007;36(6):914–31.
Tao Y, Xie Z. ChenW, Glazebrook J, Chang HS, Han B, et al. Quantitative nature of Arabidopsis responses during compatible and incompatible interactions with the bacterial pathogen Pseudomonas syringae. Plant Cell. 2003;15:317–30.
Zou J, Rodriguez-Zas S, Aldea M, Li M, Zhu J, Gonzalez DO, et al. Expression profiling soybean response to Pseudomonas syringae reveals new defense-related genes and rapid HR-specific downregulation of photosynthesis. MPMI. 2005;18:1161–74.
Truman W, Torres de Zabala M, Grant M. Type III effectors orchestrate a complex interplay between transcriptional networks to modify basal defence responses during pathogenesis and resistance. Plant J. 2006;46:14–33.
Jones AME, Thomas V, Bennett MH, Mansfield JW, Grant M. Modifications to the Arabidopsis defense proteome occur prior to significant transcriptional change in response to inoculation with Pseudomonas syringae. Plant Physiol. 2006;142:1603–20.
Ichinose Y, Taguchi F, Mukaihara T. Pathogenicity and virulence factors of Pseudomonas syringae. J Gen Plant Pathol. 2013;79:285–96.
Young JM, Takikawa Y, Gardan L, Stead DE. Changing concepts in the taxonomy of plant pathogenic bacteria. Annu Rev Phytopathol. 1992;30:67–105.
Mansfield J, Genin S, Magori S, Citovsky V, Sriariyanum M, Ronald P, et al. Top 10 plant pathogenic bacteria in molecular plant pathology. Mol Plant Pathol. 2012;13:614–29.
Bonfig KB, Schreiber U, Gabler A, Roitsch T, Berger S. Infection with virulent and avirulent P. syringae strains differentially affects photosynthesis and sink metabolism in Arabidopsis leaves. Planta. 2006;225(1):1–12.
Berger S, Benediktyová Z, Matouš K, Bonfig K, Mueller MJ, Nedbal L, et al. Visualization of dynamics of plant–pathogen interaction by novel combination of chlorophyll fluorescence imaging and statistical analysis: differential effects of virulent and avirulent strains of P. syringae and of oxylipins on A. thaliana. J Exp Bot. 2007;58(4):797–806.
Pérez‐Bueno ML, Pineda M, Díaz‐Casado E, Barón M. Spatial and temporal dynamics of primary and secondary metabolism in Phaseolus vulgaris challenged by Pseudomonas syringae. Physiol Plantarum. 2015;153(1):161–74.
Rodríguez-Moreno L, Pineda M, Soukupová J, Macho AP, Beuzón CR, Barón M. Early detection of bean infection by Pseudomonas syringae in asymptomatic leaf areas using chlorophyll fluorescence imaging. Photosynth Res. 2008;96(1):27–35.
Uchytil TF, Durbin RD. Hydrolysis of tabtoxins by plant and bacterial enzymes. Experientia. 1980;36:301–2.
Ramegowda V, Senthil-Kumar M, Ishiga Y, Kaundal A, Udayakumar M, Mysore KS. Drought stress acclimation imparts tolerance to Sclerotinia sclerotiorum and Pseudomonas syringae in Nicotiana benthamiana. Int J Mol Sci. 2013;14(5):9497–513.
Lee S, Yang DS, Uppalapati SR, Sumner LW, Mysore KS. Suppression of plant defense responses by extracellular metabolites from Pseudomonas syringae pv tabaci in Nicotiana benthamiana. BMC Plant Biol. 2013;13:65.
Hann DR, Rathjen JP. Early events in the pathogenicity of Pseudomonas syringae on Nicotiana benthamiana. Plant J. 2007;49:607–18.
Taguchi F, Ichinose Y. Role of type IV Pili in virulence of Pseudomonas syringae pv. tabaci 6605: correlation of motility, multidrug resistance, and HR-inducing activity on a nonhost plant. MPMI. 2011;24(9):1001–11.
Aro EM, Virgin I, Andersson B. Photoinhibition of photosystem II. Inactivation, protein damage and turnover. Biochim Biophys Acta. 1993;1143:113–34.
Nelson N, Ben-Shem A. The complex architecture of oxygenic photosynthesis. Nat Rev Mol Cell Bio. 2004;5:1–12.
Rochaix JD. Assembly of photosynthetic complexes. Plant Physiol. 2011;155:1493–500.
Clavier CGJ, Boucher G. The use of photosynthesis inhibitor (DCMU) for in situ metabolic and primary production studies on soft bottom benthos. Hydrobiologia. 1992;246(2):141–5.
Takano S, Tomita J, Sonoike K, et al. The initiation of nocturnal dormancy in Synechococcus as an active process. BMC Biol. 2015;13(1):36.
Strasser BJ. Donor side capacity of photosystem II probed by chlorophyll a fluorescence transients. Photosynth Res. 1997;52:147–55.
Tóth SZ, Schansker G, Kissimon J, Kovács L, Garab G, Strasser RJ. Biophysical studies of photosystem II-related recovery processes after a heat pulse in barley seedlings (Hordeum vulgare L.). J Plant Physiol. 2005;162:181–94.
Strasser BJ, Strasser RJ. Measuring fast fluorescence transients to address environmental questions: the JIP-test [M]. In: Photosynthesis: From Light to Biosphere. Ed, P Mathis. Dordrecht:Kluwer Academic Publishers; 1995. p. 977–980.
Li PM, Cheng LL, Gao HY, Jiang CD, Peng T. Heterogeneous behavior of PSII in soybean (Glycine max) leaves with identical PSII photochemistry efficiency under different high temperature treatments. J Plant Physiol. 2009;166:1607–15.
Haldimann P, Strasser RJ. Effects of anaerobiosis as probed by the polyphasic chlorophyll a fluorescence rise kinetic in pea (Pisum sativum L.). Photosynth Res. 1999;62:67–83.
Fleury C, Mignotte B, Vayssière JL. Mitochondrial reactive oxygen species in cell death signaling. Biochimie. 2002;84:131–41.
Meinhardt LW, Costa GGL, Thomazella DPT, Thomazella DP, Teixeira PJP, Carazzolle MF, et al. Genome and secretome analysis of the hemibiotrophic fungal pathogen, Moniliophthora roreri, which causes frosty pod rot disease of cacao: mechanisms of the biotrophic and necrotrophic phases. BMC Genomics. 2014;15(1):164.
Balachandran S, Osmond CB, Daley PF. Diagnosis of the earliest strain-specific interactions between tobacco mosaic virus and chloroplasts of tobacco leaves in vivo by means of chlorophyll fluorescence imaging. Plant Physiol. 1994;104(3):1059–65.
Balachandran S, Osmond CB, Makino A. Effects of two strains of tobacco mosaic virus on photosynthetic characteristics and nitrogen partitioning in leaves of Nicotiana tabacum cv Xanthi during photoacclimation under two nitrogen nutrition regimes. Plant Physiol. 1994;104(3):1043–50.
Kudoh H, Sonoike K. Irreversible damage to photosystem I by chilling in the light: Cause of the degradation of chlorophyll after returning to normal growth temperature. Planta. 2002;215:541–8.
Thomas MD, Langston-Unkefer PJ, Uchytil TF, Durbin RD. Inhibition of glutamine synthetase from pea by tabtoxinine-β-lactam. Plant Physiol. 1983;71:912–5.
Sharkey TD, Bernacchi CJ, Farquhar GD, Singsaas EL. Fitting photosynthetic carbon dioxide response curves for C3 leaves. Plant Cell Environ. 2007;30:1035–40.
Lepiniec L, Vidal J, Chollet R, Gadal P, Crétin C. Phosphoenolpyruvate carboxylase: structure, regulation and evolution. Plant Sci. 1994;99:111–24.
Sankhla N, Huber W. Regulation of balance between C3 and C4 pathway: role of abscisic acid. Z Pflanzenphysiol. 1974;74:267–71.
Amzallag GN, Lerner HR, Poljakoff-Mayber A. Exogenous ABA as a modulator of the response of sorghum to high salinity. J Exp Bot. 1990;41:1529–34.
Popova LP, Stoinova ZG, Maslenkova LT. Involvement of abscisic acid in photosynthetic process in Hordeum vulgare L. during salinity stress. J Plant Growth Regul. 1995;14:211–8.
Muller K, Doubnerova V, Synkova H, Cerovska N, Ryslava H. Regulation of phosphoenolpyruvate carboxylase in PVYNTN-infected tobacco plants. Biol Chem. 2009;390:245–51.
Ryslava H, Muller K, Semoradova S, Synkova H, Cerovska N. Photosynthesis and activity of phosphoenolpyruvate carboxylase in Nicotiana tabacum L. leaves infected by Potato virus A and Potato virus Y. Photosynthetica. 2003;41:357–63.
Tietz S, Wild A. Investigations on the phosphoenolpyruvate carboxylase activity of spruce needles relative to the occurrence of novel forest decline. Plant Physiol. 1991;137:327–31.
Goh CH, Ko SM, Koh S, Kim YJ, Bae HJ. Photosynthesis and environments: photoinhibition and repair mechanisms in plants. J Plant Biol. 2012;55:93–101.
Barth C, Krause GH, Winter K. Responses of photosystem I compared with photosystem II to high-light stress in tropical shade and sun leaves. Plant Cell Environ. 2001;24:163–76.
Öquist G, Huner NPA. Photosynthesis of overwintering plants. Annu Rev Plant Biol. 2003;54:329–55.
Terashima I, Funayama S, Sonoike K. The site of photoinhibition in leaves of Cucumis sativus L. at low temperatures is photosystem I, not photosystem II. Planta. 1994;193:300–6.
Asada K. The water-water cycle in chloroplasts: scavenging of active oxygens and dissipation of excess photons. Annu Rev Plant Biol. 1999;50(1):601–39.
Galvez Valdivieso G, Mullineaux PM. The role of reactive oxygen species in signalling from chloroplasts to the nucleus. Physiol Plantarum. 2010;138(4):430–9.
Apel K, Hirt H. Reactive oxygen species: metabolism, oxidative stress, and signal transduction. Annu Rev Plant Biol. 2004;55:373–99.
Allakhverdiev SI, Murata N. Environmental stress inhibits the synthesis de novo of proteins involved in the photodamage–repair cycle of Photosystem II in Synechocystis sp. PCC 6803. Biochim Biophys Acta. 2004;1657:23–32.
Parrado J, Absi EH, Machado A, Ayala A. “In vitro” effect of cumene hydroperoxide on hepatic elongation factor-2 and its protection by melatonin. Biochim Biophys Acta. 2003;1624:139–44.
Murata N, Takahashi S, Nishiyama Y, Allakhverdiev SI. Photoinhibition of photosystem II under environmental stress. BBA-Bioenergetics. 2007;1767(6):414–21.
Takahashi S, Murata N. How do environmental stresses accelerate photoinhibition? Trends Plant Sci. 2008;13:178–82.
Sonoike K, Kamo M, Hihara Y, Hiyama T, Enami I. The mechanism of the degradation of psaB gene product, one of the photosynthetic reaction center subunits of photosystem I upon photoinhibition. Photosynth Res. 1997;53:55–63.
Fan X, Zhang Z, Gao H, Yang C, Liu M, Li Y, et al. Photoinhibition-like damage to the photosynthetic apparatus in plant leaves induced by submergence treatment in the dark. PLoS One. 2014;9:e89067.
de Torres Zabala M, Littlejohn G, Jayaraman S, Studholme D, Bailey T, Lawson T, et al. Chloroplasts play a central role in plant defence and are targeted by pathogen effectors. Nature Plants. 2015;1(6):1–10.
Yamori W, Noguchi KO, Hikosaka K, Terashima I. Phenotypic plasticity in photosynthetic temperature acclimation among crop species with different cold tolerances. Plant Physiol. 2010;152:388–99.
Nishiyama Y, Allakhverdiev SI, Murata N. Protein synthesis is the primary target of reactive oxygen species in the photoinhibition of photosystem II. Physiol Plant. 2011;142:35–46.
Balachandran S, Osmond CB. Susceptibility of tobacco leaves to photoinhibition following infection with two strains of tobacco mosaic virus under different light and nitrogen nutrition regimes. Plant Physiol. 1994;104(3):1051–7.
King EO, Wood MK, Raney DE. Two simple media for the demonstration of pyocyanin and fluorescin. J Lab Clin Med. 1954;44(2):301–7.
Porra RJ. The chequered history of the development and use of simultaneous equations for the accurate determination of chlorophylls a and b. Photosynth Res. 2002;73:149–56.
Bingham M J, Long S P. Equipment for field and laboratory studies of whole plant and crop photosynthesis and productivity research. Techniques in Bioproductivity and Photosynthesis: Pergamon International Library of Science, Technology, Engineering and Social Studies, 2014. p. 229.
Strasser RJ, Tsimilli-Michael M, Qiang S, Goltsev V. Simultaneous in vivo recording of prompt and delayed fluorescence and 820-nm reflection changes during drying and after rehydration of the resurrection plant Haberlea rhodopensis. BBA-Bioenergetics. 2010;1797(6):1313–26.
Gao J, Li P, Ma F, Goltsev V. Photosynthetic performance during leaf expansion in Malus micromalus probed by chlorophyll a fluorescence and modulated 820 nm reflection. J Photoch Photobio B. 2013;137:144–50.
Oukarroum A, Goltsev V, Strasser RJ. Temperature effects on pea plants probed by simultaneous measurements of the kinetics of prompt fluorescence, delayed fluorescence and modulated 820 nm reflection. PLoS One. 2013;8:e59433.
Patterson BD, Macrae EA, Ferguson IB. Estimation of hydrogen peroxide in plant extracts using titanium (IV). Anal Biochem. 1984;139:487–92.
This work was supported by the Fundamental Research Funds for the Central Universities (No. 2572014AA18), China National Nature Science Foundation (No. 31070307) and Outstanding Academic Leaders for Innovation Talents of Science and Technology of Harbin City in Heilongjiang Province (No. 2013RFXXJ063).
The authors declare that they have no competing interests.
DDC, ZSZ, GYS and XBS designed the study. DDC and ZSZ carried out most of the experiments and data analysis. DDC, WSC and MZ conceived of the study, and helped to draft and revise the manuscript. All authors read and approved the final manuscript.
PsbO protein level was evaluated at 3 days post infection in tobacco leaves. Lanes from left to right in the picture represent leaves infiltrated with distilled water in the light, leaves infiltrated with P. syringae pv. tabaci (Pst) in the light, leaves infiltrated with distilled water in the dark, and leaves infiltrated with Pst in the dark, respectively (PNG 9 kb)
D1 protein level was evaluated at 3 days post infection in tobacco leaves. Lanes from left to right in the picture represent leaves infiltrated with distilled water in the light, leaves infiltrated with P. syringae pv. tabaci (Pst) in the light, leaves infiltrated with distilled water in the dark, and leaves infiltrated with Pst in the dark, respectively (PNG 7 kb)
PsaA protein level was evaluated at 3 days post infection in tobacco leaves. Lanes from left to right in the picture represent leaves infiltrated with distilled water in the light, leaves infiltrated with P. syringae pv. tabaci (Pst) in the light, leaves infiltrated with distilled water in the dark, and leaves infiltrated with Pst in the dark, respectively (PNG 10 kb)
About this article
Cite this article
Cheng, DD., Zhang, ZS., Sun, XB. et al. Photoinhibition and photoinhibition-like damage to the photosynthetic apparatus in tobacco leaves induced by pseudomonas syringae pv. Tabaci under light and dark conditions. BMC Plant Biol 16, 29 (2016). https://doi.org/10.1186/s12870-016-0723-6
- Biotic stress
- Pseudomonas syringae pv. tabaci
- Photosystem I
- Photosystem II
- Nicotiana tabacum