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Whole-Tree Water Use Efficiency Is Decreased by Ambient Ozone and Not Affected by O3-Induced Stomatal Sluggishness

Whole-Tree Water Use Efficiency Is Decreased by Ambient Ozone and Not Affected by O3-Induced Stomatal Sluggishness

  • Yasutomo Hoshika, 
  • Kenji Omasa, 
  • Elena Paoletti
PLOS
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Abstract

Steady-state and dynamic gas exchange responses to ozone visible injury were investigated in an ozone-sensitive poplar clone under field conditions. The results were translated into whole tree water loss and carbon assimilation by comparing trees exposed to ambient ozone and trees treated with the ozone-protectant ethylenediurea (EDU). Steady-state stomatal conductance and photosynthesis linearly decreased with increasing ozone visible injury. Dynamic responses simulated by severing of a leaf revealed that stomatal sluggishness increased until a threshold of 5% injury and was then fairly constant. Sluggishness resulted from longer time to respond to the closing signal and slower rate of closing. Changes in photosynthesis were driven by the dynamics of stomata. Whole-tree carbon assimilation and water loss were lower in trees exposed to ambient O3 than in trees protected by EDU, both under steady-state and dynamic conditions. Although stomatal sluggishness is expected to increase water loss, lower stomatal conductance and premature leaf shedding of injured leaves aggravated O3 effects on whole tree carbon gain, while compensating for water loss. On average, WUE of trees exposed to ambient ozone was 2–4% lower than that of EDU-protected control trees in September and 6–8% lower in October.

Introduction

Tropospheric ozone (O3) is an important phytotoxic air pollutant and is also recognized as a significant greenhouse gas [1]. Tropospheric O3 level has been continuously increasing since the first direct measurements in 1874 and its atmospheric concentration is now twice or more than in the pre-industrial age in the northern hemisphere [2][4]. Phytotoxic nature of O3 has been well known for decades [5][12]. Ozone concentrations recorded in rural areas are higher than those in the city [13] and thus O3 is now considered as the air pollutant with the highest damage potential to forests [14].

As the penetration of O3 through the cuticle can be considered as negligible [15], uptake through the stomata is a crucial factor for assessing the adverse effect of O3 on plants [16][20]. However, effects of O3 on stomatal responses are not straightforward, as both reductions and sluggish responses have been reported [21], [22]. Reductions of stomatal conductance occur when measurements are carried out under steady-state conditions [23]. Sluggishness has been reported during dynamic stomatal responses to fluctuating photosynthetic photon flux density (PPFD) [22], [24][27], vapor pressure deficit (VPD) [27], and severe water stress imposed by severing a leaf [26], [28][30]. Sluggish stomatal control over transpiration may increase water loss. Plants live in a fluctuating environment. A fast gas exchange response to rapid changes in the environmental stimuli is the key for successful plant adaptation and competition [31]. Because of climate change, forest ability of water control and carbon sequestration under O3 pollution is of rising importance [14].

Scalar and conceptual uncertainties still limit the current understanding of the basic physiological mechanisms that underline responses of forests to O3 [32]. The scalar uncertainties are due to transfer of results from seedlings in controlled environments to mature trees in the field, while the conceptual uncertainties are due to contrasting results about whole-tree water use responses to ambient O3 [32][35]. In contrast, there is a general agreement about O3 exposure as a factor of reduced tree carbon sequestration and biomass [36], although the results usually come from steady-state measurements of photosynthesis.

Ozone visible injury of leaves may be used as a clear and easily quantifiable proxy of O3 foliar damage and is the only method to assess O3 damage in the field [37]. Ozone visible injury has been investigated in many European and North American tree and herbaceous species, and partly validated under controlled conditions [38], [39]. There are few reports of relationship between stomatal conductance and O3 visible injury. After onset of O3 visible injury, significant reductions in steady-state leaf gas exchange were recorded for tree species in chamber experiments [40][42]. Omasa et al. (1981) did not report any correlation between visible injury and stomatal O3 uptake in a leaf [43]. Dynamic stomatal response was slower in injured leaves (20% injury) compared to control leaves (0% injury) for manna ash (Fraxinus ornus L.) [28].

Our main objectives were to improve our knowledge of steady-state and dynamic stomatal response to O3 visible injury in adult trees in the field, and to assess whole-tree water loss and carbon assimilation under ambient O3 impacts. Measurements were carried out in an O3-sensitive poplar clone (Oxford, Populus maximoviczii Henry × berolinensis Dippel) [44]. The amount of leaf injury per tree was experimentally manipulated by applying the O3-protectant ethylenediurea (EDU, N-[2-(2-oxo-1-imidazolidinyl)ethyl]-N’-phenylurea). EDU per se does not affect gas exchange [45] and has been widely used to prevent O3 visible injury and determine O3 effects in many plant species [39], [45][47].

Materials and Methods

Experimental Site and Plant Material

The study was carried out in an experimental field site located in central Italy (Antella: 43°44' N, 11°16' E, 50 m a.s.l., 14.7°C as mean annual temperature and 1233 mm as total annual precipitation in 2010). Forty root cuttings of the O3-sensitive Oxford clone were planted in two lines in 2007. Every week over the growing seasons 2008–2010, each tree was irrigated with 1 to 2 L of water (WAT, control line) or 450 ppm EDU solution (EDU, treated line), according to the successful application of EDU as soil drench to adult trees [48]. In 2010, the mean tree height was 2.9 m, and the mean stem diameter at breast height was 19 mm. Soil moisture was measured in the root layer (30 cm depth) by EC5 sensors equipped with an EM5b data logger (Decagon Devices, Pullman WA, USA). On average, soil moisture was 21.1±0.2% during the gas exchange measurements (September-October) and 24.5±0.1% during the growing season (April to October). The values were between field capacity (25.5%) and wilting point (17.5%) for this type of soil, i.e. sandy clay loam. Air temperature, relative humidity and precipitation were recorded by a 110-WS-16 modular weather station (NovaLynx corp., Auburn CA, USA). Average vapor pressure deficit during daylight hours and total precipitation were 1.02 kPa and 197 mm in September to October and 1.42 kPa and 625 mm from April to October, respectively. Ozone concentrations were continuously recorded at canopy height (2.0 m) by an O3 monitor (Mod. 202, 2B Technologies, Boulder CO, USA). The AOT40 value (accumulated exposure above a threshold concentration of 40 ppb during daylight hours) during the growing season (April to October) was 25.8 ppm⋅h and the maximum hourly O3 concentration reached 118 ppb.

Assessment of Ozone Visible Injury

Ozone visible injury occurred as dark stippling on the upper leaf surface since early September 2010. The injury was identified as O3-like because it was missing in shaded leaves and more severe in older than in younger leaves [38]. The symptoms were similar to those caused by ambient O3 in Populus nigra [42]. In September (22th to 28th) and October (23th to 28th), all 9502 leaves from five trees per treatment (WAT and EDU) were counted and assigned to 5%-step injury classes by the same two observers. Photoguides quantifying visible injury (0∼100%) by image analysis processing were used [38], [39]. Pest, pathogen and mechanical injury occurred in both EDU and WAT trees and was assessed to be <5% of total leaves. Leaves for measurements of gas exchange showed O3 visible injury only and were evaluated on a 1%-step basis.

Measurement of Steady-state and Dynamic Gas Exchange

Fully expanded sun leaves (medium size) with visible injury from 0% to 50% at set positions from the terminal shoot (5th to 16th) of WAT trees were measured in clear sky days of September and October 2010 between 10∶00 and 15∶00 CET. Preliminary measurements did not show significant differences in gas exchange of healthy leaves, i.e. without visible ozone injury, at those set positions. Gas exchange was measured with a portable infra-red gas analyzer (CIRAS-2 PPSystems, Herts, UK), equipped with a 2.5 cm2 leaf cuvette which controlled leaf temperature (24°C), leaf-to-air vapour pressure deficit (1.0 kPa), saturating light (1800 µmol m−2 s−1) and CO2 concentration (375 ppm). Steady-state light-saturated photosynthesis (Amax), stomatal conductance to water vapor (gs) and transpiration were measured in 41 leaves from WAT trees.

Dynamic measurements were carried out for 21 leaves from WAT trees. When both gs and Amax reached equilibrium under constant light at 1800 µmol m−2 s−1, the leaf petiole was severed with a sharp scalpel, similar to the methodology in Paoletti (2005) [26]. The data were logged at 1 min intervals for 30 min after severing. As the absolute value of gs and Amax varied among individual leaves, relative gs and Amax were expressed as a percentage of the average of the last 5 points at equilibrium, i.e., just before leaf severing. The following parameters were estimated based on fittings of two linear lines to minimize the root mean square error between measured and predicted values for gs or A (Figure 1A): range of relative gs decrease at 30 min after severing, Δgs; time to start gs decrease, Tresp (gs); rate of gs decrease at 30 min from severing, Slope(gs)  =  Δgs/(30– Tresp (gs)); range of relative Amax decrease at 30 min after severing, ΔA; time to start Amax decrease, Tresp (A); rate of Amax decrease at 30 min from severing, Slope(A)  =  ΔA/(30– Tresp (A)).

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Figure 1. Examples of dynamic response of gs and Amax after detachment of the leaf (A: calculation of the dynamic parameters in a leaf with 0% visible injury, B: time courses of absolute values in gs, C: time courses of absolute values in A).

Δgs and ΔA show the range of gs and Amax variation, respectively, over 30 min from the leaf severing. Tresp (gs) and Tresp(A) show the time to start decrease of gs and Amax, respectively. Slope(gs) and Slope(A) show the rate of decrease for gs and Amax, respectively, over 30 min.

http://dx.doi.org/10.1371/journal.pone.0039270.g001

After measurements, the leaf area was measured by means of a leaf area meter (AM300, ADC, Herts, UK) for assessing a relationship between leaf size and the variation of gs in single leaves. We hypothesized that the water content of a leaf may depend on leaf size and affect gs response.

Tree Level Modeling

To assess effects of O3 visible injury on leaf gas exchange at tree level, we constructed a simple model to scale up from single–leaf steady-state and dynamic gas exchange. The model was applied to the five trees per treatment (WAT and EDU) whose leaves were counted and assigned to a 5%-step visible injury class. Steady-state leaf water loss and photosynthesis at tree level, i.e. Wloss: mol H2O tree−1 s−1, and Atree: µmol CO2 tree−1 s−1, were estimated as follows:(1)(2)where Tr_inj and Amax_inj are transpiration rate (mmol m−2 s−1) and photosynthesis (µmol m−2 s−1), respectively, at 1800 µmol m−2 s−1 constant light for leaves showing O3 visible injury. Ninj is the number of leaves in each 5%-step injury class. LA is the average leaf area per leaf (0.003 m2 leaf−1), calculated from subsamples of 30 randomly collected leaves per tree.

Whole-tree leaf water loss and carbon assimilation under the severe water stress simulated by severing a leaf (Wloss_st: mol H2O tree−1 s−1, and Atree_st: µmol CO2 tree−1 s−1) were estimated by the following equations:(3)(4)where is the average transpiration rate (mmol m−2 s−1) and is the average photosynthesis (µmol m−2 s−1) at 1800 µmol m−2 s−1 constant light during the 30 min after severing a leaf with O3 visible injury.

Statistical Analysis

Effects of O3 visible injury on steady-state leaf gas exchange and dynamic responses after severing a leaf were tested with a regression analysis. Correlation between variables of dynamic stomatal response was tested. Two-way analysis of variance (ANOVA) was used to assess the effects of measuring month and EDU treatments on number of leaves, ozone visible injury and gas exchange parameters at whole tree level. Differences among means were tested by Tukey HSD test. Percents were arcsine square root transformed prior to analysis. Data were checked for normal distribution (Kolmogorov-Smirnov D test) and homogeneity of variance (Levene’s test). Results were considered significant at p<0.05. All statistical analyses were performed with STATISTICA software (6.0, StatSoft Inc., Tulsa, OK, USA).

Results

Number of Leaves and Ozone Visible Injury

In September, EDU trees had 83% more leaves per tree than WAT trees (Figure 2A). In October, leaf abscission had progressed faster in WAT trees (−36% of leaves relative to September) than in EDU trees (−15%), resulting in EDU trees showing significantly more leaves (+144%) than WAT trees. The percentage of injured leaves (>5% of visible injury) was significantly higher in WAT trees than in EDU trees in both September and October (Figure 2B). In October, the percentage of injured leaves was 3.13 and 7 times higher than in September in WAT and EDU trees, respectively.

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Figure 2. Total number of leaves (A) and percentage of ozone injured leaves (more than 5% of injured surface) (B) per tree (+SE) (WAT: water treated plants; EDU: EDU treated plants).

* and *** denote significance at the 5% and 0.1% level, respectively; n.s. indicates no significance. Different letters above the bars indicate significant differences among bars (Tukey HSD test, P<0.05, n = 5 trees).

http://dx.doi.org/10.1371/journal.pone.0039270.g002

Steady-state gs and Amax

Steady-state leaf gas exchange for both gs and Amax decreased with increasing O3 visible injury (Figure 1, 3). In healthy leaves (0% injury), gs was 400 to 800 mmol m−2 s−1 whereas it was less than 100 mmol m−2 s−1 in leaves with 50% injury (Figure 3A). Leaves with higher injury (>50% injury) were tested but did not show a measurable gs. In control leaves, Amax was 5 to 15 µmol m−2 s−1, and dropped to around 0 µmol m−2 s−1 in leaves with more than 35% injury (Figure 3B).

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Figure 3. Relationships between steady-state leaf gas exchange (A: stomatal conductance (gs), B: light-saturated photosynthesis (Amax)) and visible ozone foliar injury.

http://dx.doi.org/10.1371/journal.pone.0039270.g003

Variation of gs and Amax after Detachment of a Leaf

After detachment of a leaf, two phases of gas exchange response were observed (Figure 1A): no response until Tresp and then a linear decrease. The magnitude of change in gs at 30 min after severing a leaf (Δgs) did not depend on leaf size (data not shown: R2 = 0.02, p = 0.537) and thus on the total water content of a leaf.

Figure 4 shows the relationships between O3 visible injury and dynamic response of gs and Amax. Δgs showed a non-linear response to O3 visible injury (Figure 4A). It sharply decreased from 45–60% in healthy leaves (0% injury) to 15–30% in leaves with >5% visible injury. Slope(gs) sharply decreased from 2.5–3.2% min–1 in healthy leaves (0% injury) to 0.8–1.8% min–1 in leaves with >5% visible injury, and did not vary in leaves with 5–50% of injury (Figure 4B). The response time to start stomatal closing (Tresp (gs)) was linearly correlated to O3 visible injury (Figure 4C). Tresp (gs) increased from about 10 min in healthy leaves to >13 min in leaves with >20% injury. The magnitude of decrease in photosynthetic rate (ΔA) sharply decreased from about 55% in healthy leaves to about 25% in leaves with >5% visible injury (Figure 4D). Slope(A) sharply decreased from about 3.3% min–1 in healthy leaves to about 1.6% min–1 in leaves with >5% visible injury (Figure 4E). There was a linear relationship between the response time to start decrease of photosynthesis (Tresp (A)) and O3 visible injury (Figure 4F). Tresp (A) increased from 5–13 min in healthy leaves to 25 min in a leaf with 50% injury. Table 1 shows correlation between the Amax and gs variables obtained from dynamic response after severing of a leaf. The magnitude of change in Amax (ΔA) increased with increasing Δgs. The rate of reduction in Amax, i.e. Slope(A), was positively correlated with Slope(gs). The response times to start decrease of Amax and gs, i.e., Tresp, were not significantly correlated, although they showed a statistical tendency to a positive correlation (p<0.1).

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Figure 4. Relationships between visible ozone foliar injury and dynamic response of stomatal conductance (gs) and photosynthesis (Amax) over 30 min after leaf severing (A: Δgs at 30 min; B: Slope(gs); C: Tresp (gs); D: ΔA; E: Slope(A); F: Tresp (A)).

http://dx.doi.org/10.1371/journal.pone.0039270.g004

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Table 1. Correlation between Amax vs. gs variables obtained during the dynamic response to severing of a leaf (Δ: magnitude of change in Amax and gs over 30 min from the leaf severing; Tresp: time to start decrease in Amax and gs after severing a leaf; Slope: rate of Amax and gs decrease).

http://dx.doi.org/10.1371/journal.pone.0039270.t001

Carbon Assimilation and Water Loss at Tree Level

In September, Atree and Wloss were significantly lower in WAT trees, being half of the values in EDU trees (Figure 5A–B). In October, the difference between WAT and EDU trees became even larger. Whole-tree water use efficiency (Atree/Wloss) at steady-state was significantly higher in EDU trees than in WAT trees both in September and October (Figure 5C). WUE decreased over time, but the decrease was larger in WAT (−6%) than in EDU trees (−2%), resulting in a significant Time x EDU interaction. Both in September and October, both Atree_st and Wloss_st, i.e. whole-tree carbon assimilation and water loss under the simulated severe water stress, were significantly lower in WAT trees (Figure 6A–B), similarly to the results from steady-state measurements (Figure 5A–B). Whole-tree instantaneous water use efficiency, expressed as Atree_st/Wloss_st, was significantly higher in EDU trees than in WAT trees both in September and October (Figure 6C). Again, the decrease of WUE_st over time was larger in WAT (−8%) than in EDU trees (−3%).

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Figure 5. Estimated steady-state carbon assimilation (A: Atree), water loss (B: Wloss) and instantaneous water use efficiency expressed as Atree/Wloss (C: WUE) at tree level (+SE) (WAT: water treated plants; EDU: EDU treated plants).

* and *** denote significance at the 5% and 0.1% level, respectively; n.s. indicates no significance. Different letters above the bars indicate significant differences among bars (Tukey HSD test, P<0.05, n = 5 trees).

http://dx.doi.org/10.1371/journal.pone.0039270.g005

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Figure 6. Estimated carbon assimilation (A: Atree_st), water loss (B: Wloss_st) and instantaneous water use efficiency expressed as Atree_st/Wloss_st (C: WUE_st) at tree level under severe water stress imposed by severing a leaf (+SE) (WAT: water treated plants; EDU: EDU treated plants).

* and *** denote significance at the 5% and 0.1% level, respectively; n.s. indicates no significance. Different letters above the bars indicate significant differences among bars (Tukey HSD test, P<0.05, n = 5 trees).

http://dx.doi.org/10.1371/journal.pone.0039270.g006

Discussion

According to previous reports in different species [28], [40][42], the steady-state measurements indicated that gs and Amax linearly decreased with increasing leaf visible injury in the O3-sensitive Oxford clone (Figure 3). Amax dropped to around 0 µmol m−2 s−1 in leaves with more than 35% injury and gs was not measurable in leaves with more than 50% injury. In a previous field study, leaves of manna ash with 20% visible injury showed a 33% reduction in gs and Amax relative to healthy leaves (measurement in September) [28]. The result of the present study showed a larger reduction in gs (about 39%) and Amax (about 54%) of 20% injured leaves, suggesting effects of O3 visible injury on gas exchange are species-specific. Paoletti et al. (2009a) suggested that the modifications of stomatal conductance in O3 injured leaves were driven by the structural alterations found in the mesophyll rather than by structural changes in stomata or other epidermal cells [28]. Omasa et al. (1981) suggested that stomatal opening in leaves with O3 visible injury varied with changes in the pressure balance between guard cells and epidermal cells caused by the water-soaking of epidermal cells [43]. The most likely changes, however, are due to photosynthetic impairment [21], [49].

When analyzing dynamic gs response to severing of a leaf, stomata of injured leaves were shown to be slower than those of healthy leaves in responding to the closing signal (Tresp (gs)) and in the rate of closing (Slope(gs)) (Figure 4B–C). These combined effects translated in a lower ability of injured leaves to close stomata, i.e. in a lower Δgs than healthy leaves, resulting in a sluggish stomatal control over water loss. In a previous study, Paoletti et al. (2009a) also reported a slower response of stomata to severing in leaves of manna ash with O3 visible injury [28], even though only leaves with 0% and 20% injury were compared. Here, we compared leaves with a range of O3 visible injury, i.e. from no injury (control) until a measurable gs was recorded (∼50% injury) and showed that Δgs decreased sharply above 5% injury and did not change any more (Figure 4A).

Literature results highlight several mechanisms by which O3 may induce sluggishness. Omasa (1990) reported a slight increase in permeability of epidermal cell membranes and alteration of the osmotic pressure after O3 exposure, that may modulate a balance in turgor between guard and subsidiary cells [50]. Vahisalu et al. (2010) found that Ca2+-dependent signaling and O3-induced stomatal movements were independent, and highlighted a temporary desensitization of the guard cells due to blocking of the K+ channels [51]. Another cause of sluggishness may be O3-induced lower rates of transpiration in which leaves take longer to perceive the same change in water status following petiole excision [26], [28][30] or light variation [22], [26]. All the above mechanisms, however, cannot explain the non-linear response of Δgs to visible injury observed in the present study. Ozone may also delay stomatal responses by stimulating ethylene production and reducing stomatal sensitivity to ABA [52]. Ethylene production is known to increase with increasing O3 visible injury [53], [54]. In tomato plants, concentration of ACC (1-aminocyclopropane-1-carboxylic acid), a precursor of ethylene, increased when visible injury reached 5% and remained constant until the maximum injury recorded in the experiment, i.e. 35% [55]. A sharp rise of ethylene emission as soon as visible injury reaches 5% and a constant emission over this threshold would explain why Δgs decreased sharply above 5% injury and did not change any more when injury was >5% (Figure 4A). Tuomainen et al. (1997) also showed that ethylene emission from detached leaves was enhanced fourfold in ozone-treated plants, while no changes were observed in control leaves that were similarly cut at the petiole [55].

Sluggish Amax responses with increasing O3 visible injury were also found in the measurements of dynamic leaf gas exchange (Figure 4D–F). The response of Amax was similar to that of gs after severing a leaf (Figure 1), i.e. no response until Tresp and then a linear decrease during stomatal closure. Although the response time to start reduction of Amax was not significantly correlated with the response time to closing stomata, the magnitude and rate of reduction in Amax were linearly correlated to those of stomatal closure (Table 1). Heber et al. (1986) showed that photosynthetic rate decreased following stomatal closure after severing of a leaf [56]. Slightly shorter Tresp(gs) than Tresp(A) confirmed that the reduction of Amax was mediated by the response of gs. The slower reduction of Amax in injured leaves than in healthy leaves would increase carbon assimilation under water stress conditions and may be interpreted as a feedback mechanism to maximize photosynthesis under stress. However, severe O3 visible injury (>35%) shifted carbon sink to source because Amax was <0 µmol m−2 s−1 (Figure 3B).

At whole-tree level, the total carbon assimilation (Atree) and water loss (Wloss) assessed under steady-state conditions were significantly lower in WAT trees exposed to ambient ozone than in EDU-protected trees in both September and October (Figure 5A–B). Such O3-induced reduction of photosynthesis and water loss was in agreement with meta-analysis results [36]. Dynamic and steady-state whole-tree WUEs showed a similar seasonal trend. WUE was significantly higher in EDU trees than in WAT trees, both in September and October and both when assessed under steady-state and dynamic conditions (Figure 5C and 6C). On average, WUE of trees exposed to ambient ozone was 2–4% lower than that of EDU-protected control trees in September and 6–8% lower in October. The decrease of tree-level WUE over time, in fact, was larger in WAT than in EDU trees, confirming the frequently reported decrease in leaf-level WUE in O3-exposed plants [33] and O3-injured leaves [41]. Also whole-tree dynamic carbon assimilation (Atree_st) and water loss (Wloss_st) were significantly lower in WAT trees than in EDU-protected trees (Figure 6A–B). In contrast, ozone-induced stomatal sluggishness would be expected to increase whole-tree water loss. This response, however, was balanced by lower gas exchange (Figure 3) and premature shedding of injured leaves. After the onset of O3 visible injury in early September, ozone visible injury increased quickly (Figure 2B). In parallel, leaf abscission also progressed (Figure 2A), so that both whole-tree water loss and carbon assimilation were reduced. However, McLaughlin et al. (2007) reported that ambient O3 spikes significantly increased water loss of trees, as assessed from sap-flow measurements, suggesting that ozone-induced aberrations in the stomatal dynamics may differ depending on the species and the environmental conditions [32].

Conclusions

One of the topical subjects in the assessment of O3 risk to forests is scaling up from leaf level to the stand and landscape level [4]. Further improvement of our understanding about stomatal responses to ambient O3 can be regarded as an essential factor in modelling and predicting forest responses to both O3 and climate [21]. Occurrence of O3 visible injury resulted in loss of stomatal control for water loss, but was compensated by lower stomatal conductance and premature leaf shedding. The resulting decline in whole tree ability of transpiring and sequestering atmospheric carbon is a significant effect of ambient ozone pollution.

Stomata play a crucial role in regulating plant gas exchange with the atmosphere, including O3 uptake [16][20]. Surface O3 concentrations are continuously increasing [4]. The climate change brings about the risk of drought and flooding [1]. The results of this study contribute new knowledge about water control and carbon sequestration of trees under ambient O3 exposure and suggest that the effects of O3–induced stomatal sluggishness on the whole-tree carbon and water balance are negligible.

Acknowledgments

Prof. William J. Manning and Dr. Marcus Schaub are greatly acknowledged for providing EDU and poplar cuttings, respectively.

Author Contributions

Conceived and designed the experiments: EP KO. Performed the experiments: YH EP. Analyzed the data: YH EP. Contributed reagents/materials/analysis tools: EP. Wrote the paper: YH EP.

References

  1. 1. Bytnerowicz A, Omasa K, Paoletti E (2007) Integrated effects of air pollution and climate change on forests: A northern hemisphere perspective. Environ Pollut 147: 438–445.
  2. 2. Volz A, Kley D (1988) Evaluation of the Montsouris series of ozone measurements made in the nineteenth century. Nature 332: 240–242.
  3. 3. Akimoto H (2003) Global Air Quality and Pollution. Science 302: 1716–1719.
  4. 4. Paoletti E (2007) Ozone impacts on forests. CAB Reviews: Perspectives in Agriculture, Veterinary Science, Nutrition and Natural Resources 2 (No. 68), 13p.
  5. 5. NIES (National Institute for Environmental Studies) (1980) Studies on effects of air pollutants on plants and mechanisms of phytotoxicity. Res Rep Natl Inst Environ Stud Jap, Japan. 265 p.
  6. 6. NIES (1984) Studies on effects of air pollutant mixtures on plants. Part 1 & 2. Res Rep Natl Inst Environ Stud Jap, Japan. 163p & 155p.
  7. 7. Koziol MJ, Whatley FR (1984) Gaseous air pollutants and plant metabolism. Butterworths, London. 466 p.
  8. 8. Schulte-Hostede S, Darrall NM, Blank LW, Wellburn AR (1987) Air pollution and plant metabolism. London: Elsevier. 381p p.
  9. 9. Yunus M, Iqbal M (1996) Plant response to air pollution. Chichester: Wiley. 545p p.
  10. 10. Sandermann H, Wellburn AR, Heath RL (1997) Forest decline and ozone: a comparison of controlled chamber and field experiments. Berlin: Springer-Verlag. 400p p.
  11. 11. De Kok LJ, Stulen I (1998) Responses of plant metabolism to air pollution and global change. Leiden: Backhuys. 519p p.
  12. 12. Omasa K, Saji H, Youssefian S, Kondo K (2002) Air Pollution and Plant Biotechnology. Tokyo: Springer-Verlag. 455p p.
  13. 13. Gregg JW, Jones CG, Dawson TE, et al. (2003) Urbanization effects on tree growth in the vicinity of New York City. Nature 424: 183–187.
  14. 14. Serengil Y, Augustaitis A, Bytnerowicz A, Grulke N, Kozovitz AR (2011) Adaptation of forest ecosystems to air pollution and climate change: a global assessment on research priorities. iForest 4: 44–48.
  15. 15. Kerstiens G, Lendzian KJ (1989) Interactions between ozone and plant cuticles. 1. Ozone deposition and permeability. New Phytol 112: 13–19.
  16. 16. Omasa K, Abo F, Natori T, Totsuka T (1979) Studies of air pollutant sorption by plants. (II) Sorption under fumigation with NO2, O3 or NO2+O3. J Agric Meteorol 35: 77–83. (in Japanese with English summary).
  17. 17. UNECE (2004) Mapping critical levels for vegetation. Chapter 3 Manual on Methodologies and Criteria for Modelling and Mapping Critical Loads and Levels and Air Pollution Effects, Risks and Trends. Berlin: Umweltbundesamt. 52p p.
  18. 18. Grulke NE, Paoletti E, Heath RL (2007a) Comparison of calculated and measured foliar O3 flux in crop and forest species. Environ Pollut 146: 640–647.
  19. 19. Paoletti E, Manning WJ (2007) Toward a biologically significant and usable standard for ozone that will also protect plants. Environ Pollut 150: 85–95.
  20. 20. Cieslik S, Omasa K, Paoletti E (2009) Why and how terrestrial plants exchange gases with air. Plant Biol 11: 24–34.
  21. 21. Paoletti E, Grulke NE (2005) Does living in elevated CO2 ameliorate tree response to ozone? A review on stomatal responses. Environ Pollut 137: 483–493.
  22. 22. Paoletti E, Grulke NE (2010) Ozone exposure and stomatal sluggishness in different plant physiognomic classes. Environ Pollut 158: 2664–2671.
  23. 23. Wittig VE, Ainsworth EA, Long SP (2007) To what extent do current and projected increases in surface ozone affect photosynthesis and stomatal conductance of trees? A meta-analytic review of the last 3 decades of experiments. Plant Cell Environ 30: 1150–1162.
  24. 24. Reich PB, Lassoie JP (1984) Effects of low level O3 exposure on leaf diffusive conductance and water-use efficiency in hybrid poplar. Plant Cell Environ 7: 661–668.
  25. 25. Reiling K, Davison AW (1995) Effects of ozone on stomatal conductance and photosynthesis in populations of Plantago major L. New Phytol 129: 587–594.
  26. 26. Paoletti E (2005) Ozone slows stomatal response to light and leaf wounding in a Mediterranean evergreen broadlieaf, Arbutus unedo. Environ Pollut 134: 439–445.
  27. 27. Grulke NE, Neufeld HS, Davison AW, Chappelka A (2007b) Stomatal behavior of O3-sensitive and -tolerant cutleaf coneflower (Rudbeckia laciniata var. digitata) Great Smoky Mountain National Park. New Phytol 173: 100–109.
  28. 28. Paoletti E, Contran N, Bernasconi P, Gunthardt-Goerg MS, Vollenweider P (2009a) Structural and physiological responses to ozone in Manna ash (Fraxinus ornus L.) leaves of seedlings and mature trees under controlled and ambient conditions. Sci Tot Environ 407: 1631–1643.
  29. 29. Mills G, Hayes F, Wilkinson S, Davies WJ (2009) Chronic exposure to increasing background ozone impairs stomatal functioning in grassland species. Glob Chan Biol 15: 1522–1533.
  30. 30. Hoshika Y, Omasa K, Paoletti E (2012) Both ozone exposure and soil water stress are able to induce stomatal sluggishness. Environ Exp Bot. doi:10.1016/j.envexpbot.2011.12.004.
  31. 31. Tinoco-Ojanguren C, Pearcy RW (1993) Stomatal dynamics and its importance to carbon gain in two rain forest Piper species. II. Stomatal vesus biochemical limitations during photosynthetic induction. Oecol 94: 395–402.
  32. 32. McLaughlin SB, Nosal M, Wullschleger SD, Sun G (2007) Interactive effects of ozone and climate on tree growth and water use in a southern Appalachian forest in the USA. New Phytol 174: 109–124.
  33. 33. Mansfield TA (1998) Stomata and plant water relations: does air pollution create problems? Environ Pollut 101: 1–11.
  34. 34. Robinson MF, Heath J, Mansfield TA (1998) Disturbances in stomatal behaviour caused by air pollutants. J Exp Bot 49: 461–470.
  35. 35. Wieser G, Matyssek R, Then C, Cieslik S, Paoletti E (2008) Upscaling ozone flux in forests from leaf to landscape. Ital J Agron 1: 35–41.
  36. 36. Wittig VE, Ainsworth EA, Naidu SL, Karnosky DF, Long SP (2009) Quantifying the impact of current and future tropospheric ozone on tree biomass, growth, physiology and biochemistry: a quantitative meta-analysis. Glob Chan Biol 15: 396–424.
  37. 37. Heath RL (2008) Modification of the biochemical pathways of plants induced by ozone: What are the varied routes to change? Environ Pollut 155: 453–463.
  38. 38. Innes JL, Skelly JM, Schaub M (2001) Ozone and broadleaved species. A guide to the identification of ozone-induced foliar injury. Bern: Paul Haupt Verlag. 136p p.
  39. 39. Paoletti E, Ferrara AM, Calatayud V, Cervero J, Giannetti F, et al. (2009b) Deciduous shrubs for ozone bioindication: Hibiscus syriacus as an example. Environ Pollut 157: 865–870.
  40. 40. Zhang J, Ferdinand JA, VanderHeyden DJ, Skelly JM, Innes JL (2000) Variation in gas exchange within native plant species of Switzerland and relationships with ozone injury: an open-top experiment. Environ Pollut 113: 117–185.
  41. 41. Paoletti E, Nali C, Lorenzini G (2004) Gas exchange and ozone visible injury in Mediterranean evergreen broadleaved seedlings. In: Kinnunen H, Huttunen S, editors. pp. 85–101. Proceedings of the Meeting Forest Under Changing Climate, Enhanced UV and Air Pollution. Oulu: Dept Biology, Thule Institute, Univ. Oulu.
  42. 42. Novak K, Schaub M, Fuhrer J, Skelly JM, Hug C, et al. (2005) Seasonal trends in reduced leaf gas exchange and ozone-induced foliar injury in three ozone sensitive woody plant species. Environ Pollut 136: 33–45.
  43. 43. Omasa K, Hashimoto Y, Aiga I (1981) A quantitative analysis of the relationships between O3 absorption and its acute effects on plant leaves using image instrumentation. Environ Control Biol 19: 85–92.
  44. 44. Marzuoli R, Gerosa G, Desotgiu R, Bussotti F, Ballarin-Denti A (2009) Ozone fluxes and foliar injury development in the ozone-sensitive poplar clone Oxford (Populus maximowiczii × Populus berolinensis): a dose–response analysis. Tree Physiol 29: 67–76.
  45. 45. Paoletti E, Contran N, Manning WJ, Ferrara AM (2009c) Use of the antiozonant ethylenediurea (EDU) in Italy: verification of the effects of ambient ozone on crop plants and trees and investigation of EDU’s mode of action. Environ Pollut 157: 1453–1460.
  46. 46. Paoletti E, Manning WJ, Spaziani F, Tagliaferro F (2007) Gravitational infusion of ethylenediurea (EDU) into trunks protected adult European ash trees (Fraxinus excelsior L.) from foliar ozone injury. Environ Pollut 145: 869–873.
  47. 47. Manning WJ, Paoletti E, Sandermann H Jr, Ernst D (2011) Ethylenediurea (EDU): A research tool for assessment and verification of the effects of ground level ozone on plants under natural conditions. Environ Pollut 159: 3283–3293.
  48. 48. Paoletti E, Manning WJ, Ferrara AM, Tagliaferro F (2011) Soil drench of ethylenediurea (EDU) protects sensitive trees from ozone injury. iForest 4: 66–68.
  49. 49. Pell EJ, Eckardt N, Enyedi AJ (1992) Timing of ozone stress and resulting status of ribulose bisphosphate carboxylase/oxygenase and associated net photosynthesis. New Phytol 120: 397–405.
  50. 50. Omasa K (1990) Study on changes in stomata and their surroundings cells using a nondestructive light microscope system: responses to air pollutants. J Agric Meteorol 45: 251–257. (in Japanese with English summary).
  51. 51. Vahisalu T, Puzorjova I, Brosché M, Valk E, Lepiku M, et al. (2010) Ozone-triggered rapid stomatal response involves the production of reactive oxygen species, and is controlled by SLAC1 and OST1. Plant J 62: 442–453.
  52. 52. Wilkinson S, Davies W (2010) Drought, ozone, ABA and ethylene: new insights from cell to plant community. Plant Cell Environ 33: 510–525.
  53. 53. Tingey DT, Standley C, Field RW (1976) Stress ethylene evolution: a measure of ozone effects on plants. Atmos Environ 10: 969–974.
  54. 54. Samuel MA, Walia A, Mansfield SD, Ellis BE (2005) Overexpression of SIPK in tobacco enhances ozone-induced ethylene formation and blocks ozone-induced SA accumulation. J Exp Bot 56: 2195–2201.
  55. 55. Tuomainen J, Betz C, Kangasjärvi J, Ernst D, Yin Z, et al. (1997) Ozone induction of ethylene emission in tomato plants: regulation by differential accumulation of transcripts for the biosynthetic enzymes. Plant J 12: 1151–1162.
  56. 56. Heber U, Neimanis S, Lange OL (1986) Stomatal aperture, photosynthesis and water fluxes in mesophyll cells as affected by the abscission of leaves. Simultaneous measurements of gas exchange, light scattering and chlorophyll fluorescence. Planta 167: 554–562.