Effects of reduced carbonic anhydrase activity on CO₂ assimilation rates in Setaria viridis: a transgenic analysis

Carbonic anhydrase and mesophyll conductance are both limiting factors affecting CO₂ assimilation rates at low pCO₂ as examined in stably transformed lines of the C₄ species, Setaria viridis.

Abstract

In C₄ species, the major β-carbonic anhydrase (β-CA) localized in the mesophyll cytosol catalyses the hydration of CO₂ to HCO₃⁻, which phosphoenolpyruvate carboxylase uses in the first step of C₄ photosynthesis. To address the role of CA in C₄ photosynthesis, we generated transgenic Setaria viridis depleted in β-CA. Independent lines were identified with as little as 13% of wild-type CA. No photosynthetic defect was observed in the transformed lines at ambient CO₂ partial pressure (pCO₂). At low pCO₂, a strong correlation between CO₂ assimilation rates and CA hydration rates was observed. C¹⁸O¹⁶O isotope discrimination was used to estimate the mesophyll conductance to CO₂ diffusion from the intercellular air space to the mesophyll cytosol (g_m) in control plants, which allowed us to calculate CA activities in the mesophyll cytosol (C_m). This revealed a strong relationship between the initial slope of the response of the CO₂ assimilation rate to cytosolic pCO₂ (AC_m) and cytosolic CA activity. However, the relationship between the initial slope of the response of CO₂ assimilation to intercellular pCO₂ (AC_i) and cytosolic CA activity was curvilinear. This indicated that in S. viridis, mesophyll conductance may be a contributing limiting factor alongside CA activity to CO₂ assimilation rates at low pCO₂.

Introduction

C₄ plants have evolved a CO₂-concentrating mechanism (CCM) that enables the elevation of CO₂ around the active sites of Rubisco by a combination of anatomical and biochemical specialization (Hatch, 1987). C₄ photosynthesis has independently evolved >60 times, providing one of the most widespread and effective solutions for remedying the catalytic inefficiency of Rubisco (Sage et al., 2012; Christin and Osborne, 2013). The key carboxylases in C₄ plants are localized to different cellular compartments. Phosphoenolpyruvate carboxylase (PEPC) is localized to the cytosol of mesophyll cells and Rubisco to the chloroplasts of bundle sheath cells. For the CCM to operate effectively, PEPC activity must exceed Rubisco activity to balance leakage of CO₂ out of the bundle sheath compartment. This maintains a high bundle sheath CO₂ level but prevents wasteful overcycling of the mesophyll CO₂ ‘pump’ (von Caemmerer and Furbank, 2003). As PEPC utilizes HCO₃⁻ and not CO₂, the first committed enzyme of the C₄ pathway is carbonic anhydrase (CA) which catalyses the reversible conversion of CO₂ and HCO₃⁻ in the cytosol of mesophyll cells. C₄ acids produced by PEPC then diffuse into the bundle sheath cells where they are decarboxylated, supplying CO₂ for Rubisco.

Within higher plants, there are multiple forms of the α-CA, β-CA, and γ-CA families which share little sequence homology (Moroney et al., 2001). β-CAs are the most prevalent CA family in land plants. CA is an abundant enzyme in C₃ plants, representing up to 2% of the soluble leaf protein (Okabe et al., 1984). In C₃ plants, the role of CA is unclear (Badger and Price, 1994) as it does not appear to limit photosynthesis but does influence stomatal conductance, guard cell movement, and amino acid biosynthesis (Hu et al., 2010; DiMario et al., 2016; Engineer et al., 2016).

It has long been contended that the uncatalysed rate of CO₂ conversion to HCO₃⁻ is insufficient to support C₄ photosynthetic flux (Hatch and Burnell, 1990; Badger and Price, 1994). This hypothesis was supported by experiments in the C₄ dicot Flaveria bidentis, where antisense plants with <10% of wild-type CA activity required high CO₂ for growth and showed reduced CO₂ assimilation rates (von Caemmerer et al., 2004; Cousins et al., 2006). However, in the C₄ monocot Zea mays mutant plants with reduced CA activity (3% of wild type), no limitation to CO₂ assimilation rates at ambient CO₂ was observed (Studer et al., 2014). CA activity has been shown to vary widely between species (Cousins et al., 2008), and it is unclear whether CA activities are limiting at high CO₂ assimilation rates, as has previously been suggested (Hatch and Burnell, 1990; Gillon and Yakir, 2000).

We examined the role of CA in the model C₄ monocot species Setaria viridis (green foxtail millet). Setaria viridis is closely related to agronomically important C₄ crops including Z. mays (maize), Sorghum bicolor (sorghum), and Saccharum officinarum (sugarcane) (Brutnell et al., 2010). It is an ideal model species due to its rapid generation time, small stature, high seed production, diploid status, and small genome that is sequenced and publicly available (Doust et al., 2009; Brutnell et al., 2010; Li and Brutnell, 2011). Here we used a stable transformation approach to examine the role of CA in S. viridis and could show that S. viridis is a useful model species that lends itself to molecular manipulation of the C₄ photosynthetic pathway. Two constructs both targeting the major leaf β-CA (Si003882m.g) were used to generate three independent transformed lines with reduced CA activity. A strong correlation between the CO₂ assimilation rate at low pCO₂ and CA activity was observed. Our combined measurements of mesophyll conductance and CA activity suggest that increasing mesophyll conductance may be an important way to increase the CO₂ assimilation rate at low intercellular pCO₂, as may occur under drought.

Materials and methods

Plant growth conditions

T₁ seeds were incubated in 5% liquid smoke (Wrights) for 24h to promote germination, and germinated in garden soil mix fertilized with Osmocote (Scotts, Australia) in small containers before being transferred to individual 2 litre pots. Plants were grown in controlled environmental chambers, irradiance 500 µmol photons m⁻² s⁻¹, 16h photoperiod, 28 °C day, 24 °C night, 2% CO₂. Pots were watered daily.

Construct generation

Two different constructs were used to generate three lines of reduced CA activity. First, an RNAi was targeted to the primary leaf β-CA Si003882m which generated lines 2.1 and 5.3. A region of Si003882m.g was amplified by PCR using gene-specific primers (Supplementary Table S1 at JXB online) and reverse-transcribed RNA from S. viridis leaves ligated into pENTR/D-TOPO (ThermoFisher), and verified by sequencing. The fragment was inserted via a double Gateway system LR reaction (Invitrogen) into the hairpin RNAi binary vector pSTARGATE (Greenup et al., 2010) to form a stem–loop region under the control of the ubiquitin promoter/intron (UBI) and octopine synthase (OCS) terminator to form the RNAi vector pSG/CAa.

Secondly, an overexpression approach, which resulted in gene silencing, generated the third transformed line, 1.1. The coding sequence of the maize β-CA gene (GRMZM2G348512), ZmCA2 (Studer et al., 2014), was amplified by reverse transcription–PCR (RT–PCR) from total RNA extracted from B73 maize. Total RNA was isolated using hot acid phenol and chloroform, and then treated with RQ1 RNase-free DNase (Promega). The reverse transcription and PCRs were performed as per the manufacturer’s protocols with Superscript II (ThermoFisher) and Phusion High-Fidelity DNA polymerase (NEB), respectively (for primers, see Supplementary Table S1). The sequence encoding an AcV5 epitope tag (Lawrence et al., 2003) was added to the C-terminal end of ZmCA2. The resulting ZmCA2 amplicon was cloned into pENTR/D-TOPO and verified by sequencing. LR Gateway cloning (ThermoFisher) was used to insert the ZmCA2 coding sequence into the overexpression vector, pSC110. pSC110 was created by Gibson Assembly (Gibson et al., 2009) from two modified pMDC164 vectors (Curtis and Grossniklaus, 2003), kindly provided to us by Udo Gowik (Heinrich-Heine University, Dusseldorf, Germany). ZmCA2 expression from pSC110 was driven by the B73 ZmPEPC promoter. pSC110 and pSC110/ZmCA2 were verified by sequencing.

Both constructs were transformed into Agrobacterium tumefaciens strain AGL1 for stable plant transformation.

Callus induction and plant transformation

Stable transformation of S. viridis (accession A10.1) was carried out as described by Brutnell et al. (2010). Seed coats were mechanically removed from mature S. viridis seeds to improve germination. Seeds were sterilized before plating on callus induction medium [CIM; 4.3g l⁻¹ Murashige and Skoog (MS) salts, pH 5.8, 10ml l⁻¹ 100× MS vitamins stock, 40g l⁻¹ maltose, 35mg l⁻¹ ZnSO₄·7H₂O, 0.6mg l⁻¹ CuSO₄·5H₂O, 4g l⁻¹ Gelzan, 0.5mg l⁻¹ kinetin, 2mg l⁻¹ 2,4-D]. After 4 weeks in the dark at 24 °C, any seedling structures or gelatinous calli were removed and remaining calli transferred to fresh CIM. After a further 2 weeks, calli were divided and replated onto fresh CIM. One week later, transformations were performed.

AGL1 containing the construct of interest were grown in the presence of 50 µg l⁻¹ kanamycin and 50 µg l⁻¹ rifampicin at 28 °C to OD₆₀₀=0.5 and then resuspended in CIM without Gelzan and hormones. Acetosyringone (200mM) and synperonic [0.01% (w/v)] were added to the Agrobacterium solution before incubating the calli in the medium for 5min at room temperature. The calli were blotted dry on sterile filter paper and incubated at 22 °C for 3 d in the dark. The calli were then transferred to selective CIM (CIM containing 40mg l⁻¹ hygromycin, 150mg l⁻¹ timentin) and incubated in the dark at 24 °C for 16 d. Calli were then transferred to selective plant regeneration medium (PRM) containing 4.3g l⁻¹ MS salts, pH 5.8, 10ml l⁻¹ 100× MS vitamins, 20g l⁻¹ sucrose, 7g l⁻¹ Phytoblend, 2mg l⁻¹ kinetin, 150mg l⁻¹ timentin, 15mg l⁻¹ hygromycin. Calli were maintained at 24 °C under a 16h light:8h dark photoperiod and a light intensity of 60 µmol photons m⁻² s⁻¹. Developing shoots were transferred to selective rooting medium (RM) containing 2.15g l⁻¹ MS salts, pH 5.7, 10ml l⁻¹ 100× MS vitamins, 30g l⁻¹ sucrose, 7g l⁻¹ Phytoblend, 150mg l⁻¹ timentin, 20mg l⁻¹ hygromycin. Shoots that survived and developed roots were genotyped using primers against the hygromycin phosphotransferase gene (Supplementary Table S1) by PCR, and positive transformants were transplanted to soil.

Selection of plants for analysis

The progeny of three independent T₀ transformation events were analysed for CA hydration rates (Supplementary Fig. S1). One T₁ plant with low CA hydration rates was selected from each transformation event (labelled 5.3, 2.1, and 1.1) and its progeny (T₂) used for all future analysis. Two sets of experiments were performed on the T₂ plants. First, gas exchange and biochemical analysis on lines 5.3, 2.1, and 1.1 (Table 1) and, secondly, gas exchange and oxygen discrimination on lines 5.3 and 1.1 (Table 2). Each T₂ plant was genotyped prior to experiments using primers against the hygromycin phosphotransferase gene (Supplementary Table S1). The progeny of a plant which went through the S. viridis transformation process and tested negative for the hygromycin phosphotransferase gene were used as null controls.

Table 1.

Physiological and biochemical characteristics of CA transformants under ambient CO₂ conditions

Net CO₂ assimilation rate (A), stomatal conductance (g_s), mesophyll pCO₂ (C_m), the rate constant of CA hydration (k_CA), and enzyme activities were measured from the uppermost, fully expanded leaf of 5-week-old plants grown at 2% CO₂. Gas exchange measurements were made at 25 °C leaf temperature, flow rate at 500 µmol m⁻² s⁻¹, and irradiance of 1500 µmol photons m⁻² s⁻¹. Three T₂ plants from three different transformation events were measured.

	A	g s	C m	k CA	Rubisco	PEPC	NADP-ME
µmol m−2 s−1	mol m−2 s−1	µbar	mol m−2 s−1 bar−1	µmol m−2 s−1	µmol m−2 s−1	µmol m−2 s−1
Null	22.5±0.6 a	0.19±0.01 a	132.4±3.3 a	6.1±0.8 a	18.7±1.5 a	229.6±19.3 a	59.8±4.3 a
5.3	21.7±2.6 a	0.2±0.02 a	118.9±13.1 a	3.3±0.2 b	18.8±1.8 a	249.3±24.6 a	54.5±5.8 a
2.1	18.5±1.9 a	0.16±0.01 a	152.9±15.2 a	2.0±0.2 b,c	20.9±2.9 a	181.5±25.4 a	47.3±2.6 a
1.1	19.1±1.2 a	0.19±0.02 a	153.9±4.4 a	0.8±0.1 c	19.7±1.8 a	180.3±18.4 a	43.6±3.9 a

Significant differences are based on one-way ANOVA and Tukey post-hoc analysis (SPSS statistics version 22; P=0.05).

Table 2.

Physiological characteristics of CA transformants at ambient CO₂ measured using LI-6400XT coupled to a tunable diode laser

Net CO₂ assimilation rate (A), stomatal conductance (g_s), mesophyll pCO₂ (C_m), the ratio of intercellular to ambient pCO₂ (C_i/C_a), the rate constant of CA hydration (k_CA), online Δ¹⁸O discrimination, and the length of mesophyll cells exposed to intercellular airspace (S_m) were measured on the uppermost, fully expanded leaf of 5-week-old plants grown at 2% CO₂. Gas exchange measurements were made at 2% O₂, 25 °C leaf temperature, flow rate at 500 µmol m⁻² s⁻¹, and irradiance of 1500 µmol photons m⁻² s⁻¹. Three T₂ plants from two different transformation events were measured.

	A	g s	C m	C i/Ca	k CA	Δ18O	S m
µmol m−2 s−1	mol m−2 s−1	µbar	µbar	mol m−2 s−1 bar−1	‰	m2 m−2
Null	30.0±1.4 a	0.30±0.03 a	144.6±5.9 a	0.39±0.03 a	8.4±0.7 a	18.0±1.4 a	10.2±0.4 a
5.3	29.2±0.9 a	0.29±0.02 a	157.9±10.5 a	0.34±0.01 a	2.5±0.3 b	13.6±0.7 a,b	–
1.1	24.5±1.6 a	0.26±0.03 a	178.1±13.5 a	0.43±0.02 a	0.8±0.2 b	10.9±0.6 b	10.2±0.9 a

Significant differences are based on one-way ANOVA and Tukey post-hoc analysis (SPSS statistics version 22; P=0.05).

Insertion number estimation

DNA was isolated from a fully expanded leaf using a CTAB (cetyltrimethylammonium bromide) extraction buffer [2% CTAB (v/v), 20mM Tris–HCl pH 8, 1.4M NaCl, 20mM EDTA, 1% polyvinylpyrrolidone (PVP)-40 (w/v), 0.2% (v/v) β-mercaptoethanol] followed by extraction with phenol/chloroform/isoamylalcohol (25:24:1) and ethanol clean-up. DNA quality and quantity was determined using a NanoDrop spectrophotometer (Thermo Scientific).

IDNA genetics (UK) performed quantitative real-time PCR (qPCR) analysis to estimate the numbers of transgene copies in the CA transformed lines following the procedure described in Bartlett et al. (2008) with some modifications. The hygromycin phosphotransferase gene (with a FAM reporter) and the internal positive control (IPC, with a VIC reporter) were amplified together in a multiplex reaction (15min denaturation, then 40 cycles of 15s at 95 °C and 60s at 60 °C) in an ABI1900 real-time PCR machine. Fluorescence from the FAM and VIC fluorochromes was measured during each 60 °C step and the Ct values obtained. The difference between the Ct values for the hygromycin phosphotransferase gene and the IPC (the Delta Ct) was used to allocate the assayed samples into groups with the same gene copy number.

RNA extraction and reverse transcription–quantitative PCR (RT–qPCR)

Leaf discs (0.78cm²) frozen and stored at −80 °C were lysed using the Qiagen TissueLyser II. RNA was extracted using the Trizol extraction method and in the presence of RNase inhibitor (Ambion). DNA was removed using the TURBO DNA free kit (Ambion), and RNA quantity and quality were determined using a NanoDrop (Thermo Scientific).

RNA (200ng) was reverse transcribed into cDNA using Qiagen’s RT² HT First Strand cDNA synthesis kit. RT–qPCR and melt curve analysis were performed on a Viia7 Real-time PCR system using the Power SYBR green PCR Master Mix (Thermo Fisher) according to the manufacturer’s instructions. Primers (Supplementary Table S1) were designed using Primer3 in Geneious R7.1.6, ensuring products spanned an intron. Primer amplification efficiencies were determined by the Ct slope method; efficiencies for all primer pairs were comparable (~95%) and no amplification was detected in the no template control. Relative fold change was calculated by the ΔΔCt method, using the average of three nulls as reference, as described by Livak and Schmittgen (2001). The geometric mean of the Ct values for three reference genes was used for normalization (Vandesompele et al., 2002). Statistics were performed with SigmaPlot (version 11.0).

Determination of enzyme activities

For CA activity, leaf discs (0.78cm²) were collected from the uppermost fully expanded leaf of 5-week-old S. viridis plants and frozen in liquid nitrogen. Soluble protein was extracted by grinding one frozen leaf disc in ice-cold glass homogenizers (Tenbroek) in 500 µl of extraction buffer [50mM HEPES, pH 7.8, 1% (w/v) PVP, 1mM EDTA, 10mM dithiothreitol, 0.1% (v/v) Triton X-100, 2% (v/v) protease inhibitor cocktail (Sigma)]. Crude extracts were centrifuged at 4 °C for 1min at 13 000 g and the supernatant collected for the soluble CA assay. Activity was measured on a membrane inlet mass spectrometer to measure the rates of ¹⁸O exchange from labelled ¹³C¹⁸O₂ to H₂¹⁶O at 25 °C (Badger and Price, 1989; von Caemmerer et al., 2004). The hydration rates were calculated as described by Jenkins et al. (1989).

For Rubisco, PEPC, and NADP-malic enzyme (ME) activities, soluble protein was extracted from fresh leaf discs collected from leaves used for gas exchange analysis. Spectrophotometric assays were then performed as described previously (Pengelly et al., 2010, 2012; Sharwood et al., 2016).

Gas exchange measurements

Net photosynthesis (A) was measured over a range of intercellular pCO₂ (C_i) on the uppermost, fully expanded leaf of 5-week-old S. viridis plants using a portable gas exchange system LI-COR 6400XT (LI-COR Biosciences). Measurements were made after leaves had equilibrated at 380 µbar, flow rate 500 µmol s⁻¹, leaf temperature 25 °C, and irradiance 1500 µmol photons m⁻² s⁻¹. CO₂ response curves were measured in a stepwise increase (3min intervals) in CO₂ partial pressure 380, 0, 23.75, 47.5, 71.25, 95, 142.5, 190, 285, 380, 570, 760, and 950 µbar whilst maintaining leaf temperature and irradiance conditions.

Measurements of C¹⁸O¹⁶O discrimination (Δ¹⁸O)

Simultaneous measurements of exchange of CO₂, H₂O, C¹⁸O¹⁶O, and H₂¹⁸O were made by coupling two LI-6400XT gas exchange systems to a tunable diode laser (TDL: TGA200A, Campbell Scientific Inc., Logan, UT, USA) to measure C¹⁸O¹⁶O and a Cavity Ring-Down Spectrometer (L2130-i, Picarro Inc., Sunnyvale, CA, USA) to measure the oxygen isotope composition of water vapour. The system is essentially that described by Tazoe et al. (2011) except that the TGA100 was replaced by a TGA200A and the additional laser for water vapour measurements has been added together with a 16 port distribution manifold. To generate gas flows to the gas exchange systems, N₂ and O₂ were mixed by mass flow controllers (Omega Engineering Inc., Stamford, CT, USA) to generate CO₂-free air with 2% O₂. The humidity of incoming air was adjusted by varying the temperature of water circulating around a Nafion tube (Permapure, MH-110-12P-4) but was kept constant in this set of experiments to supply water vapour of a constant ¹⁸O composition. To supply flow to the TDL and the L2130-i from the sample and reference gas streams, two T junctions were inserted into the match valve tubing and in the reference line of the LI-6400XT, respectively. This allowed leaves of two plants to be measured in sequence, with each LI-6400XT sampled by the TDL at 4min intervals for 20s at the sample and reference line. The Picarro Cavity Ring Down spectrometer sampled for 3min, so that leaves were sampled at 6min intervals.

Supplementary Fig. 5 shows the CO₂ dependence of the standard error of δ¹⁸O of CO₂ in the reference gas of repeated measurements on the TGA200A. The ¹⁸O isotopic composition of the CO₂ calibration gas was 22.17±0.04‰ for Vienna mean oceanic water (VSMOW) and was checked against standards on an Isoprime mass spectrometer. We monitored the ¹⁸O composition of water vapour of the reference air streams daily, and the values were −6.07±0.08‰ and −6.34±0.08‰ (VSMOW) for LI-6400XT L1 and L2 references, respectively. We attribute the small difference between the reference lines to differences in the Nafion tubing. At the end of the experiment, the calibration of the Picarro L2130-i was confirmed by collecting water vapour samples from the gas stream of the LI-6400XT reference lines going to the Picarro as described by Cousins et al. (2006) and assaying these water samples against standards on a Picarro 1102i, which was set up to measure the ¹⁸O isotopic composition of water samples.

Gas exchange was measured on the uppermost fully expanded leaf of 5-week-old S. viridis plants at 25 °C, and leaves were equilibrated at ambient CO₂ (380 µbar), irradiance 1500 µmol photons m⁻² s⁻¹, and 2% O₂. The flow rate was 200 µmol s⁻¹. CO₂ concentration was adjusted from 380 to 760, 570, 380, and 190 µbar at 1h intervals. Immediately following gas exchange measurements, leaf discs were collected and stored at −80 °C until measurements of CA activity were made.

Calculations of C¹⁸O¹⁶O (Δ¹⁸O) discrimination and mesophyll conductance (g_m)

Discrimination against ¹⁸O in CO₂ during photosynthesis, Δ¹⁸O, was calculated from the isotopic composition of the CO₂ entering δ_in and exiting δ_out the leaf chamber and the CO₂ concentration entering C_in and exiting C_out (all measured with the TDL) (Evans et al., 1986; Barbour et al., 2016;):

$${\Delta }^{18}\text{O}=\frac{\xi \left({\delta }_{out}-{\delta }_{in}\right)}{1+{\delta }_{out}-\xi \left({\delta }_{out}-{\delta }_{in}\right)}$$ (1)

where ξ=C_in/C_in–C_out. Sample streams were passed through a Nafion drying tube before entering the TDL, and CO₂ values presented are all at zero water vapour concentration.

Following the derivation by Barbour et al. (2016) and Farquhar and Cernusak (2012) photosynthetic Δ¹⁸O discrimination was used to calculate pCO₂ in the mesophyll cytosol, C_m, with the assumption that C_m is equal to the pCO₂ at the site of CO₂–H₂O exchange and assuming that cytosolic CO₂ is in full isotopic equilibrium with local cytosolic water. This allowed g_m to be calculated from

$$g_{\text{m}}=A/\left(C_{\text{i}}-C_{\text{m}}\right)$$ (2)

$$C_m=C_i\left(\frac{{\delta }_i-a_w-{\delta }_A\left(1+a_w\right)}{{\delta }_c-a_w-{\delta }_A\left(1+a_w\right)}\right)$$ (3)

Equation 3 is the same as equation 21 of Barbour et al. (2016), and is a rearrangement of equation 18 of Farquhar and Cernusak (2012) using their notation. The oxygen isotope ratios are expressed relative to the standard, (VSMOW) $({\delta }_{\text{x}}=\frac{{\left({}_{ }{}^{18}O/{}_{ }{}^{16}O\right)}_{\text{x}}}{{\left({}_{ }{}^{18}O/{}_{ }{}^{16}O\right)}_{\text{std}}}-1)$. Intercellular pCO₂ is denoted by C_i, and a_w is the discrimination against C¹⁶O¹⁸O during liquid phase diffusion and dissolution (0.8‰).

The isotopic composition of CO₂ being assimilated, δ_A, is given by

$${\delta }_A=\frac{{\delta }_a-{\Delta }^{18}O}{1+{\Delta }^{18}O},$$ (4)

where δ_a is the isotopic composition of ambient air (in our case δ_a=δ_out).

The oxygen isotope composition of CO₂ in the intercellular airspaces, δ_i, including ternary corrections proposed by Farquhar and Cernusak (2012), is given by

$${\delta }_i=\frac{{\delta }_{io}+t\left[{\delta }_A\left(\frac{C_a}{C_i}+1\right)-{\delta }_a\frac{C_a}{C_i}\right]}{1+t}$$ (5)

where C_a is the pCO₂ in the ambient air. The ternary correction factor, t, is given by

$$t=\frac{\left(1+\frac{a_{18bs}}{1000}\right)E}{2g_{ac}}$$ (6)

where g_ac is the total conductance to CO₂, E the transpiration rate, and a_18bs is the weighted discrimination of C¹⁶O¹⁸O diffusion across the boundary layer and stomata in series given by:

$$a_{18bs}=\frac{\left(C_a-C_s\right)a_{18b}-\left(C_s-C_i\right)a_{18s}}{\left(C_a-C_i\right)}$$ (7)

where C_s is the pCO₂ at the leaf surface and a_18s and a_18b are the discriminations against C¹⁶O¹⁸O through stomata and the boundary layer (8‰ and 5.8‰, respectively).

The isotopic composition of intercellular CO₂ ignoring ternary corrections is given by

$${\delta }_{io}={\delta }_A\left(1-\frac{C_a}{C_i}\right)\left(1+a_{18bs}\right)-\frac{C_a}{C_i}\left({\delta }_a-a_{18bs}\right)+a_{18bs}$$ (8)

To calculate C_m, we assume that the isotopic composition of CO₂ in the cytosol, δ_c, is the isotopic composition of CO₂ equilibrated with cytosolic water, δ_cw, and

$${\delta }_{\text{cw}}={\delta }_{\text{w}}+{\epsilon }_{\text{w}}$$ (9)

where δ_w is the stable oxygen isotope composition of water in the cytosol at the site of evaporation and ε_w is the isotopic equilibrium between CO₂ and water (dependent on temperature T_K in K (Barbour et al., 2016, and references therein).

$${\epsilon }_w(‰)=\frac{17604}{T_K}-17.93$$ (10)

Calculation of the isotopic composition of water at the site of evaporation from the isotopic composition of transpired water

The isotopic composition of water at the site of evaporation, δ_w, can be estimated from the Craig and Gordon model of evaporative enrichment (Craig and Gordon, 1965; Farquhar and Lloyd, 1993)

$${\delta }_w={\delta }_t+{\epsilon }^{*}+{\epsilon }_k+\frac{e_a}{e_i}\left({\delta }_{wa}-{\epsilon }_k-{\delta }_t\right)$$ (11)

where ε* is the equilibrium fractionation during evaporation, ε_k is the kinetic fractionation during vapour diffusion in air, δ_t is the oxygen isotopic composition of transpired water, e_a/e_i is the ratio of ambient to intercellular vapour pressure, and δ_a is the isotopic composition of ambient air. ε* is dependent on temperature:

$${\epsilon }^{*}=2.644-3.206\left(\frac{{10}^3}{T_K}\right)+1.534\left(\frac{{10}^6}{T_K^2}\right)$$ (12)

ε_k is dependent on stomatal and boundary layer conductances and associated fractionation factors (Barbour et al., 2016, and references therein):

$${\epsilon }_k=\frac{28g_s^{-1}+19g_b^{-1}}{g_s^{-1}+g_b^{-1}}$$ (13)

The isotopic composition of transpired water δ_t can be calculated from mass balance knowing the isotopic composition of the water entering δ_win and exiting δ_wout the leaf chamber (measured with the Picarro) and the water vapour concentration entering w_in and exiting w_out (measured with the LI-6400XT):

$${\delta }_t=\left({\delta }_{wout}\left(1-w_{in}\right)-{\delta }_{win}\frac{w_{in}}{w_{out}}\left(1-w_{out}\right)\right)\frac{w_{out}}{w_{out}-w_{in}}$$ (14)

Calculation of the proportion of mesophyll cytosolic CO₂ in equilibration with leaf water, θ

If C_m is known, it is possible to calculate the isotopic composition of cytosolic CO₂ from measurements of Δ¹⁸O using equation 18 from Farquhar and Cernusak (2012):

$${\delta }_c={\delta }_A\left(1-\frac{C_i}{C_m}\right)\left(1+a_w\right)+\frac{C_i}{C_m}\left({\delta }_i-a_w\right)+a_w.$$ (15)

This can then be compared with δ_cw (Equation 9), the isotopic composition of CO₂ in equilibrium with water at the site of evaporation. We calculated mesophyll conductance, g_m, in the S. viridis null plants assuming that δ_c=δ_cw and then used this g_m to estimate C_m in the S. viridis transgenics to calculate the proportion of cytosolic CO₂ in equilibration with leaf water, θ using equations developed by Cernusak et al. (2004)

$$\theta =\frac{{\delta }_c-{\delta }_a+a_{18}\left(1+\frac{C_c}{C_a}\right)}{{\delta }_{cw}-{\delta }_a+a_{18}\left(1+\frac{C_c}{C_a}\right)}$$ (16)

where a₁₈ is the weighted discrimination of C¹⁶O¹⁸O diffusion across the boundary layer, stomata, and the liquid phase in series given by:

$$a_{18}=\frac{a_b\left(C_a-C_s\right)+a_s\left(C_s-C_i\right)+a_w\left(C_i-C_m\right)}{\left(C_a-C_m\right)}.$$ (17)

Leaf anatomical measurements and estimation of g_m from anatomical measurements

Fully expanded leaves from 5-week-old T₂ plants, null and line 1.1, were collected and cut into ~0.5×2mm pieces. Leaf slices were fixed in 2.5% (v/v) glutaraldehyde, 2% (v/v) paraformaldehyde, 0.1M phosphate buffer, and 0.01% (v/v) Tween-20 under vacuum for 20min, then replaced with buffer containing no Tween-20 and fixed overnight at 4 °C. Leaf pieces were washed in phosphate buffer and post-fixed in 1% (w/v) osmium tetroxide for 2h. Fixed leaf pieces were then dehydrated in an ethanol series (10, 30, 50, 70, 80, 95, 100%) followed by infiltration with LR white. Leaf sections were finally placed in moulds filled with resin and baked at 60 °C for 24h. Sections of 0.5 µm thickness were cut using glass knives on a Reichert ultramicrotome, stained with toluidine blue, and heat fixed to glass slides. Slides were viewed using a Zeiss Axioskop light microscope at ×400 magnification. Three images were taken from each slide for analysis, each containing a leaf cross-section in the same orientation and showing at least two vascular bundles. Fiji quantification software (Schindelin et al., 2012) was used to select regions of interest. Mesophyll surface area exposed to intercellular airspace to leaf area ratio (S_m) was calculated using Equation 18 where CCF is the curvature correction factor of 1.43 (Evans et al., 1994).

$$S_{\text{m}}=\frac{\text{Length of mesophyll cells exposed to intercellular airspace}}{\text{Interveinal distance}}\times \text{CCF}$$ (18)

The values of S_m together with measurements of cell wall thickness and cytosol thickness were used to derive an estimate of g_m from anatomical parameters. The cell wall thickness (0.113±0.005 μm) was kindly estimated from transmission electron micrographs of S. viridis grown under similar conditions by Florence Danila (Danila et al., 2016). Calculations followed equations 1–5 of von Caemmerer and Evans (2015) using the membrane permeability of Gutknecht for a lipid bilayer of 3.5×10^–3 m s⁻¹ since only the plasma membrane needs to be transversed for diffusion of CO₂ from he intercellular airspace to mesophyll cytosol (Gutknecht et al., 1977) and a cytosol thickness of 0.3 μm (von Caemmerer and Evans, 2015). These calculations give a g_m of 0.68mol m⁻² s⁻¹ bar⁻¹.

Statistical analysis

One-way ANOVAs with post-hoc Tukey test analyses were performed for all measurements of gas exchange and enzyme activities with P=0.05 using the IBM SPSS Statistics 22 package.

Results

Generation of transgenic S. viridis with reduced β-CA

In S. viridis we identified four β-CA genes: Si002140m.g (with one other isoform Si002148m), Si002669m.g, Si030616m.g (with two other isoforms Si030928m and Si030803m), and Si003882m.g. There is very low sequence identity between these β-CA genes, ~37% (Supplementary Fig. S2). Si003882m.g has been shown to be the major leaf β-CA (Christin et al., 2013; John et al., 2014).

Three independent transformation events resistant to hygromycin and with reduced CA activity were generated using two different approaches. First, one line (1.1) was generated through gene suppression upon transformation with the overexpression construct pSC110/ZmCA2. The coding sequences of ZmCA2 and Si003882m.g show 87% identity (Supplementary Fig. S3). Most probably, expression of ZmCA2 therefore caused suppression of the primary S. viridis β-CA gene, resulting in reduced CA activity in line 1.1. The second approach was to target Si003882m.g using the RNAi construct pSG/CAa which generated stably transformed lines from two different events (2.1 and 5.3). Plants were grown at high pCO₂ for all experiments.

To determine the specificity of the RNAi construct and check which β-CA was suppressed in line 1.1, RT–qPCR was performed against the β-CAs in S. viridis. Expression of the primary leaf β-CA Si003882m.g was significantly down-regulated, between 83% and 96%, in lines from all three transformation events (Fig. 1A). Transcript levels of Si030616m.g and Si002140m.g were unchanged relative to expression in the null plants (Fig. 1B, C) while Si002669m.g transcript was undetectable in all samples (data not shown). Therefore, expression of only the target β-CA gene was affected in the three transformed lines.

Fig. 1.

Expression level of β-CA transcripts. (A) Si003882m.g, (B) Si002140m.g, and (C) Si030616m.g in null control and CA transformed lines 1.1, 2.1, and 5.3 as measured by RT–qPCR and analysed by ΔΔCt. Fold change relative to the null transformant is shown; bars represent mean fold change, and circles show the data range of T₂ plants (n=5–7 plants) from each transformation event measured in triplicate. The dotted line indicates average null fold change. Expression level of the major leaf β-CA transcript Si003882m.g (A) is significantly lower compared with the null control in all three transformed lines, calculated using one-way ANOVA.

qPCR was used to estimate the number of insertions in the transgenic plants, based on the number of copies of the hygromycin phosphotransferase gene. Three T₂ plants of the three lines were analysed and there were two, four, and more than four transgene insertions detected for plants of line 5.3, 2.1, and 1.1, respectively. The high copy number in the overexpressing line of 1.1 is the likely cause of the suppression of transcript accumulation.

CA and photosynthetic enzyme activity and leaf anatomy

T₁ progeny of the three independent transformation events showed a range of CA hydration rates as measured on the soluble leaf fraction on a membrane inlet mass spectrometer. Compared with the null control, lines 1.1, 2.1, and 5.3 had on average (n=7 T₂ plants) an 87, 70, and 50% reduction of CA activity, respectively (Fig. 2). The CA hydration rate in the null plants was 934±92 µmol m⁻² s⁻¹ as calculated at a mesophyll pCO₂ (C_m) of 140 µbar (Equation 2).

Fig. 2.

Range of CA hydration rates at mesophyll pCO₂ (C_m) measured using a membrane inlet mass spectrometer in the null control and T₂ plants from lines 5.3, 2.1, and 1.1.

The activities of the photosynthetic enzymes Rubisco, PEPC, and NADP-ME were unchanged in lines 5.3, 2.1, and 1.1 compared with the nulls (Table 1) and showed no correlation with CA hydration rates (one-way ANOVA and Tukey post-hoc analysis (SPSS statistics version 22; P=0.05).

No significant differences were observed for the surface area of mesophyll cells exposed to intercellular airspace per unit leaf area (S_m) in embedded leaf sections of nulls (10.22±0.35 m² m⁻²) and plants from line 1.1 (10.18±0.95 m² m⁻²). These anatomical measurements were used to estimate an anatomical g_m of 0.68mol m⁻² s⁻¹ bar⁻¹ (see the Materials and methods).

CA activity and CO₂ assimilation rates

The response of CO₂ assimilation rate (A) to increasing intercellular pCO₂ (C_i) was investigated to examine the effect of reduced CA activity on CO₂ assimilation rates (Fig. 3). There were no statistical differences in the maximum rate of CO₂ assimilation under ambient or high CO₂ conditions between null control and progeny of transformant lines. At low pCO₂, CO₂ assimilation rates were reduced to varying degrees in the progeny of the transformed lines compared with the null control. Individuals of line 1.1 with the lowest CA hydration rate had the lowest initial slopes of the AC_i curves. The initial slopes of the AC_i and AC_m curve were plotted against the CA hydration rate constant (k_CA; Fig. 4). Mesophyll cytosolic pCO₂, C_m, was calculated from Equation 2, using the average null g_m (0.9mol m⁻² s⁻¹ bar⁻¹) since there was no difference in S_m. A strong correlation between the initial slope from the AC_m curve and k_CA was observed, with the initial slope increasing as CA hydration rates increase (R²=0.845; Fig. 4). There was a curvilinear response between the initial slope of the ACi curves indicating other limitations. No difference in stomatal conductance (g_s) was observed across a range of intercellular pCO₂ between null controls and any of the transformed lines during the rapid measurements of CO₂ responses (Fig. 5).

Fig. 3.

CO₂ assimilation rate of transformed lines over a range of intercellular pCO₂ (C_i). Average of three T₂ plants from each line. Plants were grown at 2% CO₂, and the uppermost, fully expanded leaves of 5-week-old plants were measured using a LI-6400XT at 25 °C leaf temperature at an irradiance of 1500 µmol photons m⁻² s⁻¹. Arrows mark ambient pCO₂ for each line; note that the dotted arrow is line 1.1.

Fig. 4.

Relationship between the initial slope of the AC_m (triangles) or AC_i (circles) curves and the rate constant of CA hydration rates (k_CA), AC_mR²=0.846. Each point represents a measurement made on an individual leaf of a T₂ plant.

Fig. 5.

Stomatal conductance (g_s) over a range of intercellular pCO₂ (C_i). Measurements were made concurrently with those in Fig. 4.

Oxygen isotope discrimination measurements

Oxygen (∆¹⁸O) isotope discrimination and CO₂ assimilation rates were measured in response to changes in pCO₂ using a LI-6400XT coupled to a TDL trace gas analyser to measure C¹⁸O¹⁶O and a Cavity Ring-Down Spectrometer to measure the oxygen isotope composition of water vapour. Transformed plants with reduced CA hydration rates had lower ∆¹⁸O compared with the nulls, but only line 1.1 was significantly lower (Table 2).

In the null controls, measurements of ∆¹⁸O were used to estimate conductance of CO₂ from the intercellular airspace to the sites of CO₂ and H₂O exchange in the cytosol (g_m) with the assumption that CO₂ was in full isotopic equilibrium with leaf water in the cytosol (Equation 2; Fig. 6). Although g_m appeared to increase with decreasing C_i, there were no significant differences between g_m estimated at the different C_i, and the average value was 0.94±0.06mol m⁻² s⁻¹ bar⁻¹ (Fig. 6B). C_i–C_m indicates the drawdown of CO₂ from the intercellular airspace to the site of fixation, and for the null controls there is an increasing gradient of pCO₂ as C_i increases (Fig. 6C).

Fig. 6.

(A) CO₂ assimilation rate, (B) mesophyll conductance (g_m; Equation 2), and (C) C_i–C_m over a range of intercellular pCO₂ in null controls measured using a LI-6400XT coupled to a tunable diode laser. Plants were grown at 2% CO₂ and the uppermost, fully expanded leaves of 5-week-old plants were measured at 25 °C leaf temperature, flow rate 200 µmol m⁻² s⁻¹, 2% O₂ at an irradiance of 1500 µmol photons m⁻² s⁻¹.

∆¹⁸O at ambient pCO₂ showed statistically significant differences between line 1.1 (with the lowest CA activity) and null plants (Table 2). When plotted against C_m/C_a, ∆¹⁸O measurements closely correspond to theoretical curves representing θ (Equation 16) under different scenarios either where cytosolic CO₂ is at full isotopic equilibrium with the cytosolic water (null lines) or where there is only partial equilibrium (such as line 1.1; Fig. 7). Calculated values for line 5.3 which showed a 50% reduction in CA activity relative to the null controls fell in between these two theoretical lines. This is illustrated again with theta (θ) of lines 1.1 and 5.3 over a range of C_m (Fig. 8). When CO₂ is at full isotopic equilibrium with the cytosolic water, θ would be 1, whereas in lines 1.1 and 5.3 (with reduced CA hydration rates relative to the null control) θ is <1. There was no CO₂ dependence of θ over the range of pCO₂ measured.

Fig. 7.

Oxygen isotope discrimination (Δ¹⁸O) as a function of the ratio of mesophyll pCO₂ to ambient pCO₂ (C_m/C_a) in null and lines 5.3 and 1.1. Each point represents a measurement made on an individual leaf of a T₂ plant. Triangular symbols represent measurements made at low pCO₂. Theoretical curves represent the scenario where cytosolic CO₂ is at full isotopic equilibrium with cytosolic water (θ=1, black) or under partial equilibrium (θ=0.5, grey) of ¹⁸O in the leaf. The equations for the curves are given by $\Delta {}_{ }{}^{18}O=a_{18}+\frac{C_{\mathrm{m}}}{C_{\mathrm{a}}-C_{\mathrm{m}}}\left({\delta }_{\mathrm{c}}-{\delta }_{\mathrm{a}}\right)$ and a₁₈=5.85‰ and δ_c–δ_a=33‰ at full equilibration or a₁₈=5.1‰ and δ_c–δ_a=15‰ (Farquhar and Lloyd, 1993).

Fig. 8.

Average isotopic equilibrium (theta, θ) over a range of mesophyll pCO₂ in two reduced CA lines 5.3 (grey) and 1.1 (white). Measured values of θ were determined from Δ¹⁸O using Equation 16. Each point represents the average measurement of three T₂ plants.

Discussion

Setaria viridis as a model species to study photosynthetic physiology in a C₄ monocot

Flaveria bidentis, a readily transformable model C₄ dicot, has been successfully used to study the regulation of C₄ photosynthesis using antisense and RNAi technology (Furbank et al., 1997; Matsuoka et al., 2001; von Caemmerer et al., 2004; Pengelly et al., 2012). This work has been crucial in quantifying the rate-limiting steps in the C₄ pathway by ‘titrating’ out levels of target enzymes by gene suppression and observing the effects on physiological characteristics of the resultant transgenics (Furbank et al., 1997). There are, however, important differences between C₄ dicots and the C₄ monocots which make up the majority of agriculturally important C₄ species. Setaria viridis has emerged as a new model grass to study C₄ photosynthesis in crops and related bioenergy species. Setaria viridis is an appropriate biochemical model species for Z. mays and S. bicolor as all three use NADP-ME as the primary decarboxylation enzyme. We generated transgenic S. viridis plants with reduced CA activity to compare the effect with previous results obtained with F. bidentis and Z. mays (von Caemmerer et al., 2004; Studer et al., 2014) and to explore the effect that a reduction in CA activity has on the initial slope of the AC_i and AC_m curves. In these lines, only the major leaf isoform of β-CA was reduced (Fig. 1). The transgenic plants had a range of different CA activities (Fig. 2), but showed no changes in PEPC and Rubisco activity (Table 1) or anatomical parameters (Table 2), making these plants ideal for exploring the role of CA activity in S. viridis.

Initial slope of AC_i curves in C₄ plants

Models of C₄ photosynthesis suggest that the initial slope of the AC_i curve is determined by three possible limitations: (i) the mesophyll conductance to CO₂ diffusion from the intercellular airspace to the mesophyll cytosol (g_m); (ii) the rate of CO₂ hydration by CA; and (iii) the rate of PEP carboxylation (von Caemmerer, 2000). However, it is not readily known which is the major limitation in C₄ species. Studies with PEPC mutants from the C₄ dicot Amaranthus edulis indicate that PEPC activity may not be the major limitation as a 60% reduction in PEPC leads to only a 20% reduction in the CO₂ assimilation rate at ambient pCO₂ accompanied by a small reduction in initial slope for the AC_i curves (Dever et al., 1992; Dever, 1997; Cousins et al., 2007). This study with S. viridis confirms that substantial reductions in CA activity are possible before a reduction in steady-state CO₂ assimilation rate and initial slope of the AC_i curve are observed. This is in accordance with previous observations in F. bidentis and Z. mays (von Caemmerer et al., 2004; Studer et al., 2014).

The Michaelis–Menten constant for CO₂ for CA is >2mM (~5% CO₂) which makes it appropriate to quantify CA activity by its first-order rate constant (Jenkins et al., 1989; Hatch and Burnell, 1990) and simplifies species comparisons. In S. viridis, the lowest rate constant recorded was 0.8mol m⁻² s⁻¹ bar⁻¹ compared with values of 0.1 for the ca1ca2 double mutant in Z. mays and 0.47 for transgenic F. bidentis (von Caemmerer et al., 2004; Studer et al., 2014). With this low rate constant, F. bidentis had very low CO₂ assimilation rates and the CO₂ response curves did not saturate at high CO₂. In contrast, for both S. viridis transgenics and Z. mays mutants, CO₂ assimilation rates were only slightly less than in the controls, suggesting that S. viridis is more similar to Z. mays in its CA requirements. This suggests that these two monocot species can make better use of leaf CA activity or that in vivo CA activity is greater than that estimated in vitro.

Mesophyll conductance and the initial slope of AC_m curves

Next, we used recently established techniques that utilize ¹⁸O discrimination measurements to quantify g_m in our null controls (Fig. 6B; Barbour et al., 2016). This estimates the diffusion of CO₂ from the intercellular airspace through the cell wall, plasma membrane, and cytosol to the sites of CA activity. At ambient pCO₂, the g_m observed for the null plants were similar to those reported by Barbour et al. (2016). A key assumption for the calculation of g_m is that CA activity is not limiting and that CO₂ is in isotopic equilibrium with HCO₃⁻; consequently g_m was not measured in the transgenic lines with reduced CA activity. In C₃ species, g_m (in this instance from the intercellular airspace to the chloroplast stroma) has been shown to be proportional to the chloroplast surface area appressing the intercellular airspace per unit leaf area (Evans et al., 1994). Evans and von Caemmerer (1996) hypothesized that in C₄ species g_m may correlate with the mesophyll surface area exposed to intercellular airspace per unit leaf area (S_m). Since S_m was similar between the nulls and line 1.1 plants, we assumed that g_m may also be similar between the plants. In C₃ species, g_m has been shown to, in some instances, increase with decreasing pCO₂ (Flexas et al., 2007; Tazoe et al., 2011; Alonso-Cantabrana and von Caemmerer, 2016). These changes to g_m which may be important in regulating and maintaining photosynthesis were also observed here in the S. viridis null plants, with g_m increasing slightly at low pCO₂. However, because the differences in g_m at different pCO₂ were not significant, we used the average g_m estimated for the null plants to calculate mesophyll cytosolic pCO₂ (C_m) in the transgenics.

As shown in Fig. 4, a strong almost linear relationship was found between AC_m and k_CA, whereas a saturating relationship was observed with AC_i. This indicates that the CO₂ assimilation rate is limited by cytosolic CA activity, with the relationship becoming clearer after accounting for g_m. It is tempting to speculate that the differences between the two monocot species and F. bidentis relate to differences in limitations imposed by g_m which affects cytosolic pCO₂ and hence in vivo CA activity, but this is not borne out by comparative measurements of g_m made by Barbour et al. (2016). CA activity increases with increasing pH, so variation in cytosolic pH can also contribute to variations in in vivo CA activity; however, these effects are not large (Jenkins et al., 1989). The interaction of β-CA and a CO₂-permeable aquaporin in Arabidopsis thaliana has indicated that CA can be localized near the plasma membrane rather than dispersed throughout the mesophyll cytosol (Wang et al., 2016). This may also impact on CA activity and result in another difference between the C₄ species. Other possibilities pertain to differences in anatomical characteristics of leaves. Both CA and PEPC are cytosolic enzymes, and differences in S_m may affect the efficiency with which CA is used. Our results suggest that increasing g_m may be an important way to increase the CO₂ assimilation rate at low intercellular pCO₂, a scenario that may, for example, occur under drought.

Oxygen isotope discrimination and the CO₂ dependence of isotopic equilibrium

As had previously been observed, Δ¹⁸O decreased with reductions in CA activity as CA facilitates the exchange of O₂ between cytosolic water and CO₂ (Fig. 7; Williams et al., 1996; Cousins et al., 2006). Previous reports, which have estimated the proportion of cytosolic CO₂ in equilibrium with leaf water (θ) in C₄ species, have generally assumed a relatively large g_m value and this then led to lower estimates of θ (Cousins et al., 2006, 2008). Here we assumed that in the S. viridis null plants there is sufficient CA for isotopic equilibrium to be reached, as discussed by Barbour et al. (2016). For comparison, we also estimated g_m from anatomical estimates of S_m, and cell wall and cytosolic thickness following calculations outlined by von Caemmerer and Evans (2015). This gives a g_m value of 0.68mol m⁻² s⁻¹ bar⁻¹ which is less than the value of 0.9mol m⁻² s⁻¹ bar⁻¹ calculated from Δ¹⁸O measurements and highlights the anatomical constraints for CO₂ diffusion dictated by the photosynthetic pathway in leaves of C₄ plants (von Caemmerer et al., 2007).

Reduction in CA activity led to significant reductions in θ but it is interesting to note that θ did not vary significantly with pCO₂. This is explained by the fact that CA activity increases linearly with pCO₂ so that although there is more CO₂ that needs to equilibrate with leaf water, there is also proportionally more CA activity. The fact that neither transgenic line showed a CO₂ dependence suggests that the decrease in the ratio of CA hydrations to PEP carboxylations is not affecting the isotopic equilibration of CO₂ with leaf water. These results have important implications for the interpretation of the ¹⁸O signature of atmosopheric CO₂ (Yakir and Sternberg, 2000; Gillon and Yakir, 2001; Wingate et al., 2009).

Reduction of CA in S. viridis does not alter the stomatal reponse to CO₂

The CO₂ regulation of stomatal conductance remains an open question (Engineer et al., 2016). It has been previously shown that in the ca1/ca4 double mutant of A. thaliana, the degree of stomatal closure in response to increasing pCO₂ was reduced (Hu et al., 2010; Wang et al., 2016). It is clear that CA is part of a complex signal transduction network. However, nothing is currently known about the role of CA in stomatal CO₂ responses in C₄ species. In our study, where only one β-CA isoform was reduced, we found no change in the response of stomatal conductance to CO₂. The S. viridis β-CA reduced here (Si003882m.g) has low sequence identity (<50%) to all of the Arabidopsis β-CAs, but we would predict that multiple reductions in β-CA isoforms would be required to observe a similar stomatal phenotype in S. viridis.

Conclusion

Under current atmospheric conditions, CA activity was not rate limiting for C₄ photosynthesis in S. viridis. At lower C_i, which may, for example, occur under conditions of drought, our results suggest that g_m may pose a greater limitation than CA activity. However, it is important to investigate the role of CA on C₄ photosynthesis under a range of environmental conditions such as high temperatures which have recently been suggested to deactivate CA activity in S. viridis (Boyd et al., 2015). Here we have shown that S. viridis is a useful model monocot C₄ species that lends itself to molecular manipulation of the C₄ photosynthetic pathway.

Supplementary Data

Supplementary data are available at JXB online.

Table S1. Primers used in this study

Figure S1. CA hydration rates at mesophyll pCO₂ in the T₁ plants.

Figure S2. Very low sequence identity (~37%) between the four main S. viridis β-CAs.

Figure S3. High sequence identity (87%) of Si003882m.g to the ZmCA2 (GRMZM2G348512).

Figure S4. CO₂ assimilation rate of the TDL experiment.

Figure S5. Standard error of δ¹⁸O in the reference gas of repeated measurements with the TGA200A.