<figure><img src="image_1.png" /></figure>

Corrigendum to

“Effects of leaf length and development stage on the triple oxygen isotope signature of grass leaf water and phytoliths: insights for a proxy of continental atmospheric humidity” published in *Biogeosciences*, 16, 4613–4625, 2019

Anne Alexandre<fnref n="1" />, Elizabeth Webb<fnref n="2" />, Amaelle Landais<fnref n="3" />, Clément Piel<fnref n="4" />, Sébastien Devidal<fnref n="4" />, Corinne Sonzogni<fnref n="1" />, Martine Couapel<fnref n="1" />, Jean-Charles Mazur<fnref n="1" />, Monique Pierre<fnref n="3" />, Frédéric Prié<fnref n="3" />, Christine Vallet-Coulomb<fnref n="1" />, Clément Outrequin<fnref n="1" />, and Jacques Roy<fnref n="4" />

**Correspondence:** Anne Alexandre (alexandre@cerege.fr)

Published: 11 December 2019

Two authors were attributed a wrong affiliation. The authors' affiliations are now correct in the author list above. The authors apologize for any inconvenience that this may have caused.

<footnote n="1">¹Aix Marseille Univ, CNRS, IRD, INRA, Coll France, CEREGE, Aix-en-Provence, France</footnote>

<footnote n="2">²Department of Earth Sciences, The University of Western Ontario, London, Ontario, Canada</footnote>

<footnote n="3">³Laboratoire des Sciences du Climat et de l'Environnement (LSCE/IPSL/CEA/CNRS/UVSQ), Gif-sur-Yvette, France</footnote>

<footnote n="4">⁴Ecotron Européen de Montpellier, Univ Montpellier, UPS 3248 CNRS, Campus Baillarguet, Montferrier-sur-Lez, France</footnote>
# Effects of leaf length and development stage on the triple oxygen isotope signature of grass leaf water and phytoliths: insights for a proxy of continental atmospheric humidity

Anne Alexandre, Elizabeth Webb, Amaelle Landais, Clément Piel, Sebastien Devidal, Corinne Sonzogni, Martine Couapel, Jean-Charles Mazur, Monique Pierre, Frederic Prie, et al.

► To cite this version:

Anne Alexandre, Elizabeth Webb, Amaelle Landais, Clément Piel, Sebastien Devidal, et al. Effects of leaf length and development stage on the triple oxygen isotope signature of grass leaf water and phytoliths: insights for a proxy of continental atmospheric humidity. Biogeosciences, 2019, 16 (23), pp.4613-4625. 10.5194/bg-16-4613-2019. hal-02464804

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https://hal.science/hal-02464804

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# Effects of leaf length and development stage on the triple oxygen isotope signature of grass leaf water and phytoliths: insights for a proxy of continental atmospheric humidity

Anne Alexandre<fnref n="1" />, Elizabeth Webb<fnref n="2" />, Amaelle Landais<fnref n="3" />, Clément Piel<fnref n="4" />, Sébastien Devidal<fnref n="4" />, Corinne Sonzogni<fnref n="1" />, Martine Couapel<fnref n="1" />, Jean-Charles Mazur<fnref n="1" />, Monique Pierre<fnref n="2" />, Frédéric Prié<fnref n="2" />, Christine Vallet-Coulomb<fnref n="1" />, Clément Outrequin<fnref n="1" />, and Jacques Roy<fnref n="4" />

**Correspondence:** Anne Alexandre (alexandre@cerege.fr)

Received: 1 March 2019 – Discussion started: 27 March 2019

Revised: 4 October 2019 – Accepted: 5 November 2019 – Published: 5 December 2019

**Abstract.** Continental relative humidity (RH) is a key climate parameter, but there is a lack of quantitative RH proxies suitable for climate model-data comparisons. Recently, a combination of climate chamber and natural transect calibrations have laid the groundwork for examining the robustness of the triple oxygen isotope composition ($\delta^{18}$O and $^{17}$O-excess) of phytoliths, that can preserve in sediments, as a new proxy for past changes in RH. However, it was recommended that besides RH, additional factors that may impact $\delta^{18}$O and $^{17}$O-excess of plant water and phytoliths be examined. Here, the effects of grass leaf length, leaf development stage and day-night alternations are addressed from growth chamber experiments. The triple oxygen isotope compositions of leaf water and phytoliths of the grass species *F. arundinacea* are analysed. Evolution of the leaf water $\delta^{18}$O and $^{17}$O-excess along the leaf length can be modelled using a string-of-lakes approach to which an unevaporated-evaporated mixing equation must be added. We show that for phytoliths to record this evolution, a kinetic fractionation between leaf water and silica, increasing from the base to the apex, must be assumed. Despite the isotope heterogeneity of leaf water along the leaf length, the bulk leaf phytolith $\delta^{18}$O and $^{17}$O-excess values can be estimated from the Craig and Gordon model and a mean leaf water-phytolith fractionation exponent ($\lambda_{Phyto-LW}$) of 0.521. In addition to not being leaf length dependent, $\delta^{18}$O and $^{17}$O-excess of grass phytoliths are expected to be impacted only very slightly by the stem vs.

leaf biomass ratio. Our experiment additionally shows that because a lot of silica polymerises in grasses when the leaf reaches senescence (58 % of leaf phytoliths in mass), RH prevailing during the start of senescence should be considered in addition to RH prevailing during leaf growth when interpreting the $^{17}$O-excess of grass bulk phytoliths. Although under the study conditions $^{17}$O-excess$_{Phyto}$ do not vary significantly from constant day to day-night conditions, additional monitoring at low RH conditions should be done before drawing any generalisable conclusions. Overall, this study strengthens the reliability of the $^{17}$O-excess of phytoliths to be used as a proxy of RH. If future studies show that the mean value of 0.521 used for the grass leaf water-phytolith fractionation exponent $\lambda_{Phyto-LW}$ is not climate dependent, then grassland leaf water $^{17}$O-excess obtained from grassland phytolith $^{17}$O-excess would inform on isotope signals of several soil-plant-atmosphere processes.

## 1 Introduction

Recently, a combination of growth chamber and natural transect calibrations laid the groundwork for examining the robustness of the triple oxygen isotope composition (expressed by $^{17}$O-excess = $\delta^{17}$O – 0.528 $\cdot \delta^{18}$O) of phytoliths as a new proxy for past changes in continental atmospheric relative

<footnote n="1">¹Aix Marseille Univ, CNRS, IRD, INRA, Coll France, CEREGE, Aix-en-Provence, France</footnote>

<footnote n="2">²Department of Earth Sciences, The University of Western Ontario, London, Ontario, Canada</footnote>

<footnote n="3">³Laboratoire des Sciences du Climat et de l'Environnement (LSCE/IPSL/CEA/CNRS/UVSQ), Gif-sur-Yvette, France</footnote>

<footnote n="4">⁴Ecotron Européen de Montpellier, Univ Montpellier, UPS 3248 CNRS, Campus Baillarguet, Montferrier-sur-Lez, France</footnote>
humidity (RH) (Alexandre et al., 2018). Continental RH is a key climate parameter. When combined with atmospheric temperature, it can be used to estimate the concentration of atmospheric water vapour, one of the main components of the global water cycle. However, global climate models have difficulties to properly capture continental RH (Sherwood et al., 2010; Risi et al., 2012; Fischer and Knutti, 2013), and there is a lack of RH proxies suitable for model-data comparisons.

Phytoliths are micrometric particles of hydrous amorphous silica (SiO₂(H₂O)ₙ) that form in and between living plant cells. Silica polymerises from the sap that contains dissolved silicon (among other nutrients) absorbed by the plant roots from the soil. Phytoliths can take the shape of the cells they form in, which gives them morphological taxonomic properties. Hence, phytolith morphological assemblages extracted from buried soils, loess and sediments are commonly used for palaeoenvironmental reconstructions (Miyabuchi and Sugiyama, 2015; Nogué et al., 2017; Woodburn et al., 2017). In grasses, silica, that represents several percent of the dry weight (d.w.), polymerises mainly in the leaf epidermis from where the plant water evaporates during transpiration (Alexandre et al., 2011; Kumar et al., 2016), and to a much lesser extent in the stem (Webb and Longstaffe, 2000). This polymerisation is assumed to occur in isotope equilibrium with the plant water (Alexandre et al., 2018; Shahack-Gross et al., 1996; Webb and Longstaffe, 2000).

Variations in the ¹⁷O-excess of plant water can exceed most of the variations identified so far in seawater, surface water, rainfall and ice (Landais et al., 2006; Li et al., 2017; Sharp et al., 2018; Alexandre et al., 2018). They are mainly driven by evaporative fractionation of the transpired water in the leaves. The extent of this fractionation partly depends on atmospheric RH (Cernusak et al., 2016; Craig and Gordon, 1965), which changes daily, seasonally and at longer timescales of climate change. In rainfall the ¹⁷O-excess varies slightly as it is weakly affected by temperature (Barkan and Luz, 2005; Uemura et al., 2010) or phase changes during air mass transport, in contrast to the deuterium-excess (d-excess = δ²H – 8.0 × δ¹⁸O). In surface waters, the ¹⁷O-excess is a powerful tool for tracing very evaporative conditions (Gázquez et al., 2018; Surma et al., 2015, 2018). The ¹⁷O-excess of waters imprints the ¹⁷O-excess of minerals formed in isotope equilibrium with these waters (Gázquez et al., 2017; Herwartz et al., 2017; Passey et al., 2014; Sharp et al., 2016, 2018).

In Alexandre et al. (2018), the ¹⁷O-excess of phytoliths from a grass species (*Festuca arundinacea*) grown in a climate chamber was examined. A linear relationship with RH was demonstrated. This relationship was close to the one obtained for soil phytoliths collected in West Africa along a vegetation and RH transect. This relationship allowed for the prediction of RH with a standard error of 5.6 %. However, it was recommended that, besides RH, additional factors that may impact the ¹⁷O-excess of bulk phytolith samples should

be examined before using this relationship as a proxy of past RH.

In particular, in nature, the biomass of grass stem, sheath and blade, as well as the leaf length is highly species dependent. Previous studies showed that for grasses the water δ¹⁸O increases from stem to leaf and from the bottom to the tip of the leaf blade (e.g. Gan et al., 2002; Helliker and Ehleringer, 2000; Farquhar and Gan, 2003; Webb and Longstaffe, 2003; Cernusak et al., 2016). The ¹⁷O-excess of grass water also shows variation along the leaf (Landais et al., 2006). This raises the question whether diversity in grass physiognomy impacts the relationship between the ¹⁷O-excess of phytoliths and RH.

Silica precipitate throughout the grass's life, mainly, but not exclusively, in the epidermis. The process can be either metabolically controlled or passive, i.e. depending mainly on silica saturation during cell dehydration when the leaf water evaporates (Kumar et al., 2017, 2019 and references therein). The contribution of evaporated water to the bulk leaf water may vary with transpiration (Cernusak et al., 2016), which changes from day to night (Caird et al., 2007) and decreases drastically when the start of senescence occurs (Norton et al., 2014). This raises the question whether RH changes from day to night and from leaf growth to leaf senescence should be considered when interpreting the ¹⁷O-excess of phytoliths as a RH proxy.

In order to address these issues, a growth chamber experiment was set up to explore the influence of light–dark and day–night alternations on the ¹⁷O-excess and δ¹⁸O of leaf water and phytoliths of *F. arundinacea*. Another experiment allowed us to examine the evolution of water and phytolith ¹⁷O-excess and δ¹⁸O values along the leaf, and from young to adult and senescent leaves of *F. arundinacea*. Leaf water and phytoliths were extracted and analysed for δ¹⁸O and δ¹⁷O. Silica concentrations were measured. Phytolith morphological assemblages that give information on the type of tissue and cells that are silicified were identified. The observed ¹⁷O-excess and δ¹⁸O values of leaf water and phytolith-forming water are compared with Craig and Gordon (1965)-derived evaporation model estimates. This comparison allows us to assess the processes driving the ¹⁷O-excess and δ¹⁸O values of grass leaf water and phytoliths. Implications for the calibration of the RH proxy are discussed.

## 2 Notations in the triple oxygen isotope system

In the triple oxygen isotope system (δ¹⁸O, δ¹⁷O) the fractionation factors (¹⁷α and ¹⁸α) are related by the exponent θ, where ¹⁷α=¹⁸αθ or θ = ln¹⁷α/ln¹⁸α. For the silica-water couple, and according to the Sharp et al. (2016) empirical Eq. (10), θsilica-water equals 0.524 for the 5–35 °C temperature range. For the water liquid-water vapour couple at equilibrium, θequil equals 0.529 for the 11–41 °C range (Barkan
and Luz, 2005). When evaporation occurs, a fractionation due to the vapour diffusion in air is added to the equilibrium fractionation, as conceptualised by the Craig and Gordon model (Craig and Gordon, 1965; Gat, 1996). $\theta_{\text{diff}}$ associated with this diffusion fractionation equals 0.518 (Barkan and Luz, 2007). When RH decreases, amplitude of the fractionation governed by $\theta_{\text{diff}}$ increases. While $\theta$ applies to a particular well-constrained physical process, the term $\lambda$ is used when several fractionation processes occur at the same time. The overall fractionation in the triple oxygen isotope system can be formulated as following: $\lambda = \Delta'^{17}\text{O}_{\text{A-B}}/\Delta'^{18}\text{O}_{\text{A-B}}$, with $\Delta'^{17}\text{O}_{\text{A-B}} = \delta'^{17}\text{O}_{\text{A}} - \delta'^{17}\text{O}_{\text{B}}$, $\Delta'^{18}\text{O}_{\text{A-B}} = \delta'^{18}\text{O}_{\text{A}} - \delta'^{18}\text{O}_{\text{B}}$, $\delta'^{17}\text{O} = \ln(\delta'^{17}\text{O} + 1)$ and $\delta'^{18}\text{O} = \ln(\delta'^{18}\text{O} + 1)$. $\delta$ and $\delta'$ notations are expressed in ‰ vs. VSMOW. In the $\delta'^{18}\text{O}$ vs. $\delta'^{17}\text{O}$ space, $\lambda$ represents the slope of the line linking $\Delta'^{17}\text{O}_{\text{A-B}}$ to $\Delta'^{18}\text{O}_{\text{A-B}}$. In hydrological studies, the triple oxygen isotope composition of water is expressed by the ¹⁷O-excess ($\text{¹⁷O-excess} = \delta'^{17}\text{O} - 0.528 \times \delta'^{18}\text{O}$). In the $\delta'^{17}\text{O}$ vs. $\delta'^{18}\text{O}$ space, the ¹⁷O-excess depicts the $\delta'^{17}\text{O}$ departure from a reference line with a slope $\lambda$ of 0.528. This is the slope of the Global Meteoric Water Line (expressed as $\delta'^{17}\text{O} = -0.528 \times \delta'^{18}\text{O} + 0.33$ per meg; Luz and Barkan, 2010). The average ¹⁷O-excess of meteoric waters range from 35 to 41 per meg (Luz and Barkan, 2010; Sharp et al., 2018). As the reference slope is close to the liquid-vapour equilibrium exponent $\theta_{\text{equil}}$ (0.529), the ¹⁷O-excess is very convenient to highlight kinetic processes that result from evaporation.

## 3 Material

In three growth chambers, the grass species *F. arundinacea* was sown and grown in commercial potting soil in a 35 L container (53 cm × 35 cm × 22 cm, L × W × D). A total of 10 d after germination, agar-agar was spread on the soil surface around the seedlings to prevent any evaporation from the soil as described in Alexandre et al. (2018). Ambient RH was kept constant in the growth chamber by combining a flow of dry air and an ultrasonic humidifier that produces vapour without any isotope fractionation. The vapour and the soil irrigation water (IW) came from the same source, and their triple oxygen isotope composition was similar (−5.59 ‰ and 26 per meg for $\delta'^{18}\text{O}$ and ¹⁷O-excess, respectively).

### 3.1 Experiment 1

This experiment was designed to examine the grass leaf water and phytolith isotope signatures in different parts of the leaf and at different stages of the leaf development. Briefly, the stages considered were (i) young leaf, where only the end of the blade is visible as it emerges from the sheath of the preceding leaf; (ii) adult leaf where the blade is fully developed, the ligule is visible and the sheath is well formed; and (iii) yellow and desiccated senescent leaf.

*F. arundinacea* was grown for 39 d, in a climate chamber where light, air temperature and RH were set constant at 290 µmol m⁻² s⁻¹, 20 °C and 73 %, respectively. On day 28, irrigation was stopped to force senescence of the leaves. A total of 197 g of biomass was collected 11 d later. From this biomass, young leaf (visible end of the blade), adult leaf and senescent leaf (blade only) were separated. Adult leaves, of 24 cm length in average, were sectioned into three parts: sheath, proximal part of the blade (10 cm long) and apical part of the blade. Five samples resulted (Table 1). For all samples, except the senescent leaves, 3–5 g biomass were put in gastight glass vials and kept frozen for bulk leaf water extraction. Senescent leaves were too dry for water extraction. The rest of the biomass (between 10 and 70 g depending on the sample, Table 1) was dried for phytolith extraction.

### 3.2 Experiment 2a

Light triggers the opening of plant stomata with, as an inevitable consequence, an increase in water loss through these stomata. At night, however, stomata often do not close totally. Night transpiration is often 5 % to 15 % of day transpiration (Caird et al., 2007). In *F. arundinacea*, stomatal conductance at night can be as high as 30 % of conductance during the day (Pitcairn et al., 1986). Together with difference in air RH between day and night, this could affect isotope enrichment of leaf water (Barbour et al., 2005). This experiment was thus designed to assess whether light–dark alternation may impact the isotope signature of *F. arundinacea* leaf water.

In a growth chamber, *F. arundinacea* was grown for 22 d with constant light. Then, a 12 h light–12 h dark alternation was introduced. Temperature and RH were kept constant at 25 °C and 60 %, respectively. Half of the biomass was harvested at the end of day 22 (constant light). Then the alternation period was set up, and the second half of the biomass was harvested at the end of day 26. In order to consider potential spatial heterogeneity, leaf blades (both young and adult leaves) were collected from four different places in the culture for each harvest. The eight resulting samples (Table S1 in the Supplement) were put in gastight glass vials and kept frozen for bulk leaf water extraction.

### 3.3 Experiment 2b

In natural conditions, day-night alternations imply changes in temperature and RH in addition to changes in light intensity. This experiment was designed to assess whether over a period of several day-night alternations, changes in RH during the night impacted the mean isotope signature of grass leaf phytoliths.

For this experiment, the leaf water was not analysed as it only gives a snapshot of its isotope composition. *F. arundinacea* was grown in two growth chambers. In the first chamber, light, temperature and RH were kept constant
<table><caption>**Table 1.** Growth chamber experiment 1: Experimental set-up, phytolith content and triple oxygen isotope data obtained for phytoliths (Phyto), leaf water (LW) and irrigation (IW). Growth conditions: duration: 39 d from 25 July to 2 September 2016; atmospheric temperature: 20 °C; leaf temperature: 18 °C; atmospheric relative humidity: 73 %, no irrigation; samples labelling: P4-75-02-09-2016. Phyto “C” and “P” stand for phytolith concentration and proportion; “av.” stands for weighted average. “% d.w.” stands for % dry weight. Phytolith proportion was calculated using a mass loss correction factor of 0.7 for senescent leaves (see text for explanation).</caption><thead><tr><th rowspan="2">Samples</th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th rowspan="2"></th><th colspan="5">Phytoliths (Phyto)</th><th colspan="5">Leaf water (LW) and irrigation water (IW)</th></tr><tr><th>Total biomass g</th><th>Phyto C. % d.w.</th><th>Phyto P %*</th><th>n</th><th>δ<sup>18</sup>O</th><th>SD</th><th>δ<sup>17</sup>O</th><th>SD</th><th>δ<sup>18</sup>O</th><th>SD</th><th>δ<sup>17</sup>O</th><th>SD</th><th>δ<sup>17</sup>O-excess per meg</th><th>λ</th><th>n</th><th>δ<sup>18</sup>O</th><th>δ<sup>17</sup>O</th><th>δ<sup>18</sup>O</th><th>δ<sup>17</sup>O</th><th>δ<sup>17</sup>O-excess per meg</th><th>λ</th></tr></thead><tbody><tr><td>Y</td><td>Young leaves</td><td>blade</td><td>57.2</td><td>0.8</td><td></td><td>3</td><td>39.22</td><td>0.17</td><td>20.27</td><td>0.21</td><td>38.47</td><td>0.17</td><td>20.07</td><td>0.21</td><td>-243</td><td>7</td><td>0.522</td><td>1</td><td>13.8</td><td>7.20</td><td>13.67</td><td>7.17</td><td>-46</td><td>0.525</td></tr><tr><td>Sh</td><td>Adult leaves</td><td>sheath</td><td>55.57</td><td>0.8</td><td>17</td><td>3</td><td>36.24</td><td>0.12</td><td>18.77</td><td>0.14</td><td>35.60</td><td>0.12</td><td>18.59</td><td>0.14</td><td>-202</td><td>23</td><td>0.522</td><td>1</td><td>1.54</td><td>0.83</td><td>1.54</td><td>0.83</td><td>15</td><td>0.538</td></tr><tr><td>A &lt; 10</td><td></td><td>proximal blade</td><td>35.5</td><td>0.7</td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td></tr><tr><td rowspan="3">A &gt; 10</td><td></td><td>apical blade</td><td>35.9</td><td>2.1</td><td>52</td><td>2</td><td>41.60</td><td>0.02</td><td>21.47</td><td>0.02</td><td>40.76</td><td>0.02</td><td>21.25</td><td>0.02</td><td>-275</td><td>5</td><td>0.521</td><td>1</td><td>12.7</td><td>6.63</td><td>12.58</td><td>6.60</td><td>-38</td><td>0.525</td></tr><tr><td></td><td>bulk blade</td><td>71.4</td><td>1.4</td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td></tr><tr><td></td><td>av.</td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td></tr><tr><td rowspan="2">S</td><td rowspan="2">Senescent leaves</td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td></tr><tr><td></td><td>blade</td><td>12.54</td><td>3.0</td><td>3</td><td>39.66</td><td>0.19</td><td>20.51</td><td>0.23</td><td>38.89</td><td>0.19</td><td>20.30</td><td>0.23</td><td>-235</td><td>7</td><td>0.522</td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td></tr><tr><td>IW</td><td>Irrigation water</td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td><td></td></tr></tbody></table>

<footnote>* % of bulk leaf (sheath and blade).</footnote>
(290 mmol m⁻² s⁻¹, 25 °C and 60 %, respectively). In the second chamber, 12 h day–12 h night alternations were set. During the day (light 290 µmol m⁻² s⁻¹), temperature and RH were set to 25 °C and 60 %, respectively, whereas during the night (no light) they were set to 20 °C and 80 %, respectively. The leaf blades (both young and adult leaves) were harvested after a first growth of 16 d and a second growth of 18 d (Table S1) and dried for phytolith extraction.

# 4 Methods

## 4.1 Phytolith chemical extraction, counting and analysis

Phytoliths were extracted using a high-purity protocol with HCl, H₂SO₄, H₂O₂, HNO₃, KClO₃ and KOH at 70 °C following Corbineau et al. (2013) and Alexandre et al. (2018). Phytoliths were weighed and their mass reported to the initial leaf dry weight (d.w.). To account for leaf mass loss during senescence, a mass loss correction factor of 0.7, previously estimated for graminoids (Vergutz et al., 2012), was applied to the phytolith concentration in senescent leaves (Table 1).

Most grass phytoliths have a morphology characteristic of their cell of origin. Phytolith morphological assemblages were thus determined to follow the spatial evolution over time of the leaf silicification. Phytoliths assemblages from experiment 1 were mounted on microscope slides in Canada Balsam and counted using light microscopy at a 600× magnification. More than 200 phytoliths with a dimension greater than 5 µm and with a characteristic morphology were counted. Phytolith types were named using the International Code for Phytolith Nomenclature 1.0 (Madella et al., 2005) and categorised as follows: “trapeziform short cell” and “trapeziform sinuate short cell” coming from the short cell silicification, “elongate cylindric” and “elongate echinate” coming from the intercoastal long cell silicification, “acicular” produced by hair silicification and “parallellepipedal” produced by bulliform cells silicification (Table 1, Fig. 1). These characteristic phytoliths are commonly used for palaeoenvironmental reconstructions when recovered from buried soils or sediments (e.g. Woodburn et al., 2017). In addition, thin silica particles with uncharacteristic shape and with a refractive index too low to be accurately described using light microscopy were also counted. Abundance of the phytolith categories are expressed in percentage of the sum of counted particles. Three repeated counts usually give an error lower than ±5 % (SD). The phytolith assemblages were further observed with a scanning electron microscope (FEG-SEM, HITACHI SV6600, accelerating voltage of 3 kV, 15° tilt, working distance of 14 mm and probe current of a few picoampere to avoid charging issues), after carbon coating.

Phytoliths triple oxygen isotope analysis was performed as described in details in Alexandre et al. (2018). The in-

<figure><img src="image_3.png" /><figcaption>**Figure 1.** Growth chamber experiment 1: SEM pictures of phytoliths from young, adult and senescent leaf blade: silicified trapeziform short cell (1, 2 and 3), silicified trapeziform sinuate short cell (4), undefined silicified short cell or broken elongate cylindric long cell (5), silicified elongate cylindric long cell (6a, 6b, 7 and 8) and silicified cell wall also reported as silica sheets (9 and 10).</figcaption></figure>

frared (IR) laser-heating fluorination technique (Alexandre et al., 2006; Crespin et al., 2008; Suavet et al., 2010) was used to extract the oxygen gas (O₂) after dehydration and dehydroxylation under a flow of N₂ (Chaplin et al., 2010). Then, the O₂ was passed through a –114 °C slush to refreeze gases interfering with the mass 33 (e.g. NF). These interfering gases may be produced during the fluorination of residual N in the line. The purified O₂ was sent to a dual-inlet mass spectrometer (ThermoQuest Finnigan Delta Plus). The composition of the reference gas was determined through the analyses of NBS28 for which isotope composition has been set to δ¹⁸O = 9.60‰ vs. VSMOW, δ¹⁷O = 4.99‰ vs.
VSMOW and ¹⁷O-excess = 65 per meg. Each analysis consisted of two runs of eight dual-inlet measurements with an integration time of 26 s. The sample isotope compositions were corrected on a daily basis using a quartz laboratory standard (Boulangé) with δ¹⁸O = 16.284‰ vs. VSMOW, δ¹⁷O = 8.463‰ vs. VSMOW. During the measurement period, Boulangé reproducibility (SD) was ±0.13‰, ±0.07‰ and ±11 per meg for δ¹⁸O, δ¹⁷O and ¹⁷O-excess, respectively (n = 9). For a given sample, two to three phytoliths aliquots were analysed. Measured reproducibility ranged from 5 to 23 per meg for ¹⁷O-excess.

## 4.2 Leaf water extraction and analysis

Leaf water was extracted over 6 h using a distillation line. Then a fluorination line was used to convert water to oxygen using CoF₃. Oxygen was analysed by dual-inlet IRMS (ThermoQuest Finnigan MAT 253) against a working O₂ standard calibrated against VSMOW. The detailed procedure was previously described in Landais et al. (2006) and Alexandre et al. (2018). The reproducibility (two replicates) was 0.015‰ for δ¹⁷O, 0.010‰ for δ¹⁸O and 5 per meg for ¹⁷O-excess.

## 4.3 Irrigation and vaporisation water analysis

The irrigation and vaporisation waters were analysed with an isotope laser analyser (Picarro L2140-i) operated in ¹⁷O-excess mode using an autosampler and a high-precision vaporiser as described in detail in Alexandre et al. (2018). The reproducibility (three replicates) was 0.02‰, 0.01‰ and 10 per meg for δ¹⁷O, δ¹⁸O and ¹⁷O-excess, respectively.

# 5 Results

## 5.1 Phytolith concentration, assemblage and origin in grass leaf (experiment 1)

From young to adult and senescent blade, the phytolith content increases sharply from 0.8 % d.w. to 1.1 % d.w. and 3.0 % d.w. (Table 1). This makes 58 % of blade phytoliths precipitating at the start of senescence. In adult leaves, the phytolith concentration of 0.8 % d.w. and 0.7 % d.w. in the sheaths and proximal blade increases to 2.1 % d.w. in the apical blade. This makes apical blade phytoliths representing 52 % of adult leaf phytoliths.

Short cell phytoliths are found in all samples, while long cell phytoliths are absent from the adult sheath (Table S2). The ratio of long cell vs. short and long cell phytoliths increases with phytolith concentration from young (29 % of counted phytoliths) to adult (49 % of counted phytoliths) and senescent (67 % of counted phytoliths) leaf blades (Fig. 2). In adult leaves, it increases from sheath (1 % of counted phytoliths) to proximal (19 % of counted phytoliths) and apical (59 % of counted phytoliths) blades. Parallelepipedal bulliform and acicular hair phytoliths can be observed but in

<figure><img src="image_4.png" /><figcaption>**Figure 2.** Growth chamber experiment 1: Phytolith concentration vs. long cell phytolith proportion. Error bars represent the 5% error on counting (refer to text for details).</figcaption></figure>

small amounts (< 2 % of counted phytoliths) in young and senescent leaf blade samples. All phytolith assemblages contain thin silica particles with low refractive index, difficult to count with accuracy in light microscopy. SEM observation shows they are composed of multi-cellular silica sheets (mostly silicified cell walls and a few silicified stomata complexes) (Fig. 1, Table S2). Their abundance ranges from 24 % to 18 % of counted phytoliths in young and adult blades and increases up to 52 % of counted phytoliths in senescent leaf blades. Because these silica sheet particles are very thin, their weight contribution to the isotope signature of bulk phytolith assemblages is expected to be significantly lower than their number.

## 5.2 Heterogeneity in the triple oxygen isotope composition of leaf water

Irrigation and leaf water (IW and LW, respectively) δ¹⁸O, δ¹⁷O, and ¹⁷O-excess values obtained from experiment 1 are presented in Table 1 and Fig. 3. As expected, the lowest δ¹⁸O_LW and δ¹⁷O_LW values occur in the adult leaf sheath. The sheath water is still ¹⁸O-enriched by 7.1‰ relative to the irrigation water, whereas the difference in ¹⁷O-excess is not significant (11 per meg). In adult leaf waters, an evaporative fractionation trend (¹⁷O-excess_LW-IW decreases and δ¹⁸O_LW increases) occurs from the sheath to the proximal and apical blade. Water from the young leaf blade plots close to the adult apical blade.

## 5.3 Heterogeneity in the triple oxygen isotope composition of leaf silica

When plotted in the ¹⁷O-excess vs. δ¹⁸O space (Fig. 3), the triple oxygen isotope composition of phytoliths in adult leaf also show a clear evaporative fractionation trend from the sheath to the proximal and apical blade. λ<sub>Phyto-LW</sub> decreases from 0.522 in the sheath and proximal blade to 0.521 in the apical blade (Table S2).
<figure><img src="image_5.png" /><figcaption>**Figure 3.** Growth chamber experiment 1: leaf water and phytolith triple oxygen isotope data and estimates. Observed ¹⁷O-excess vs. δ¹⁸O for leaf water (triangles) and phytoliths (squares) in young, adult and senescent leaves (black symbols) and along adult leaf (sheath, proximal blade, apical blade) (white symbols) (Table 1). Error bars are displayed when larger than the symbols. Estimated ¹⁷O-excess vs. δ¹⁸O for bulk leaf water (Table S3) and along the leaf length (Table S4) according to the Craig and Gordon (C&G) model (Cernusak et al., 2016; Farquhar et al., 2007) and the C&G model complemented with a mixing equation.</figcaption></figure>

Given the measurement precision, young, adult and senescent blades have close δ¹⁸O<sub>Phyto</sub> (38.47, 39.47, 38.89‰, respectively) and ¹⁷O-excess<sub>Phyto</sub> (–243, –257 and –235 per meg, respectively) values (Table S2). The ¹⁷O-excess<sub>Phyto</sub> value of the bulk leaf (–238 per meg) is very close to the estimate calculated from the ¹⁷O-excess<sub>Phyto</sub> vs. RH relationship obtained from growth chamber experiment in Alexandre et al. (2018) (–222 per meg).

## 5.4 Effect of light–dark and day–night alternation on the triple oxygen isotope composition of leaf water and leaf silica

Plant water isotope data from experiment 2a where light–dark alternations were set without changing RH, are presented in Table S1. Variations within a given set of samples (e.g. F4-02-03-17 Day or F4-02-03-17 Night in Table S1)

are important, alerting that interpretation in term of kinetic vs. equilibrium fractionation of small variations of δ¹⁸O<sub>LW</sub> (< 1‰) or ¹⁷O-excess<sub>LW</sub> (< 14 per meg) should be avoided. When considering the margins of error, the averaged values of δ¹⁸O<sub>LW</sub> and ¹⁷O-excess<sub>LW</sub> obtained after the dark period are similar to the ones obtained after the light period. It was not possible to measure the night and day transpiration flows or the stomatal conductance during the experiment. In experiment 2b, where temperature and RH changed with light–dark alternations, transpiration and leaf blade phytolith concentrations did not change by more than 0.1 L d⁻¹ and 0.2 % d.w., respectively, when light was set constant or alternates with dark (Table S1). Differences in δ¹⁸O<sub>Phyto</sub> and ¹⁷O-excess<sub>Phyto</sub> are lower than 1.4‰ and 30 per meg, respectively, but are not always in the same direction. In summary, under the experimental set up conditions (high RH), light–
dark alternation has no obvious impact on the oxygen triple isotope composition of leaf water and phytoliths.

# 6 Discussion

## 6.1 Silicification dynamics

The phytolith content and assemblages obtained from experiment 1 can be discussed in light of previous studies investigating silica deposition in grasses. At the cell level, silicification, which is a rapid process taking a few hours (Kumar and Elbaum, 2017), initiates either in the extra-membranous space or in the cell wall and proceeds centripetally until the cell lumen is filled up (Bauer et al., 2011). During cell lumen silicification, some cells are still viable and transfer their content to each other before their full silicification (Kumar and Elbaum, 2017). Long and short cell phytoliths polymerise that way. Cell wall silicification, not followed by complete cell lumen filling, has been also frequently observed both in the epidermis (Kumar et al., 2017) and in the bundle sheath parenchyma cells surrounding the veins (Motomura, 2004). Cell wall silicification produces the multi-cellular silica sheets observed in the phytolith samples from experiment 1.

Over the course of leaf development, short cells are the first to silicify. This silicification is metabolically controlled (Kumar et al., 2017, 2019 and references therein). Then, when the leaves become mature, long cell silicification takes over (Motomura, 2004; Kumar et al., 2016). In this case, silicification is supposed to be passive, i.e. its extent depends on silica saturation during cell dehydration at the evaporation sites. Passive silicification applies also to bulliform and hair cell silicification (Kumar et al., 2017, 2019 and references therein). Increase of long vs. long and short cell phytoliths from young to adult and senescent leaf blade, observed in experiment 1 (Fig. 2), confirms this pattern of silicification when the leaf develops. Cell wall silicification added to short and long cell silicification occurs mainly when the leaf reaches senescence.

## 6.2 Impact of leaf length on the triple oxygen isotope compositions of grass leaf water

δ¹⁸O_LW of the bulk leaf water can be estimated from the Craig and Gordon model applied to plant leaf water by Farquhar et al. (2007) (Table S3, adapted from spreadsheet provided in Cernusak et al., 2016). For that purpose, the grass transpiration is supposed to be at steady state as climatic conditions were set constant during the 39 d of growth. We also assumed that the vapour has the same isotope composition as the irrigation water since (i) the vaporised water comes from the same source as the irrigation water and is not fractionated by the vaporiser, (ii) there is no soil evaporation and (iii) transpiration should produce a vapour with a composition similar to the one of the soil water pumped by the roots (e.g. Welp

et al., 2008). We measured the temperature of an adult leaf of *F. arundinacea* grown under conditions similar to those of experiment 1. The leaf was systematically 2 °C cooler than the surrounding air and no significant temperature difference was detected between the sheath, proximal and apical blade. Thus, the model was run for a leaf temperature of 18.4 °C. For estimating the δ¹⁷O_LW, we used the equilibrium and kinetic fractionation (¹⁷αₐₗ and ¹⁷αₖ, respectively, Table S3) calculated according to ¹⁷αₐₗ=¹⁸αₐ₀.⁵²⁹ and ¹⁷αₖ=¹⁸αₖ⁰.⁵¹⁸.

The bulk leaf water δ¹⁸O_LW estimate is 3.35‰ higher than the observed value. However, the ¹⁷O-excess_LW estimate is only 16 per meg lower than the observed one (Table S3, Fig. 3). δ¹⁸O_LW (and thus δ¹⁸O_LW) overestimation is common, and different corrections have been proposed to take into account advection of less evaporated stem water in the bulk leaf water (synthesis in Cernusak et al., 2016). Assuming a mixture between evaporated water and irrigation water, with the proportion of evaporated water (E) being 0.8, brings the estimated isotope composition of the bulk leaf water close to the observed one (differences in δ¹⁸O_LW and ¹⁷O-excess_LW of 0.43‰ and 10 per meg, respectively) (Table S3 and Fig. 3). Our experimental setup, where the vapour isotope composition is similar to the irrigation isotope composition and RH is relatively high, makes the ¹⁷O-excess_LW weakly sensitive to unevaporated water advection. However, this should not be the case under natural conditions, especially at low RH.

For modelling the strong increase in δ¹⁸O_LW, concomitant with a ¹⁷O-excess_LW decrease from the irrigation water to the sheath, proximal and apical blade of the leaf, the string-of-lakes approach (Gat and Bowser, 1991; Helliker and Ehleringer, 2000; Farquhar and Gan, 2003) can be used. This approach, which implies progressively ¹⁸O-enriched water segments along the leaf, is particularly adapted to the longitudinal veinal structure of grasses. Using the Farquhar and Gan (2003) Eqs. (2), (3) and (5), we calculated δ¹⁸O_LW and δ¹⁷O_LW from 0 to 24 cm length (Table S4). In the triple oxygen isotope space, the modelled curve (green continuous curve in Fig. 3) is characteristic of an evaporation trend (Surma et al., 2018). The ranges of estimated and observed δ¹⁸O_LW and ¹⁷O-excess_LW values are close. However, the observed data plot systematically on the left of the modelled curve. A mixture between evaporated water and irrigation water must be added for the new modelled curve (green dashed curve in Fig. 3) to fit the data. This presumes that part of the irrigation water entering the grass circulates in the parallel veinal structure of the blade without participating to the pool of water successively evaporated. The contribution of evaporated water (E in Table S4) increases from 0 at the leaf base to 1 at the apex. According to this new modelled curve, the sheath, where stomata are few but still present (e.g. Chaffey, 1985), already contains about 60 % of evaporated water. This is in agreement with previous observations showing ¹⁸O enrichment in the sheath of different grass species
(Webb and Longstaffe, 2003). The fact that the isotope sig-
nature of the young blade plots close to the signature of the
apical adult leaf blade suggests that the young leaf proximal
part was not entirely sampled. More importantly, the string-
of-lakes model implies that the δ¹⁸O_LW and ¹⁷O-excess_LW
values do not evolve as a function of absolute leaf length but
as a function of distance relative to the maximum leaf length
(Table S3). This makes both the maximum ¹⁸O and ¹⁷O en-
richments in the grass leaf apical part and the isotope com-
position of grass bulk leaf water independent of grass leaf
length.

**6.3 Impact of leaf length on the triple oxygen isotope compositions of grass leaf phytoliths**

Polymerisation of silica is supposed to occur in isotope equi-
librium with the formation water, and, therefore, its iso-
tope composition should only be governed by temperature
and the isotope composition of the leaf water (Alexandre
et al., 2018; Dodd and Sharp, 2010; Sharp et al., 2016).
From the δ¹⁸O_LW and δ¹⁷O_LW values estimated using the
string-of-lakes approach, we calculated δ¹⁸O<sub>Phyto</sub> and ¹⁷O-
excess<sub>Phyto</sub> (Table S4). We used two thermo-dependent re-
lationships, empirically established from diatom samples, to
calculate ¹⁸α<sub>Phyto-LW</sub>, δ¹⁸O<sub>Phyto</sub> (Dodd and Sharp, 2010) and
α¹⁷O<sub>Phyto-LW</sub> assuming λ<sub>Phyto-LW</sub> equals 0.524 (Sharp et al.,
2016, Eq. 10).

In the ¹⁷O-excess vs. δ¹⁸O space, the modelled phytolith
curve (green curve on Fig. 3) is above the data observed
for phytoliths from the sheath, proximal and apical blade.
Changing values for ¹⁸αPhyto-LW or for leaf temperature,
stomatal or boundary layer conductance, air vapour or leaf
vapour pressure in the model, do not reconcile observed
and estimated isotope compositions. Assuming a λPhyto-LW
value of 0.522 moves the modelled curve (blue curve on
Fig. 3) lower but still above the observed data. λPhyto-LW must
decrease from 0.522 to 0.520, from the base to the apex of
the leaf, for the modelled curve (red continuous curve on
Fig. 3) to encompass the observed ¹⁷O-excessPhyto values.
When the mixing hypothesis previously described for mod-
elling the leaf water composition with length is added, the
new modelled curve (red dashed curve on Fig. 3) correctly
fits the data.

For the adult bulk leaf δ¹⁸O<sub>Phyto</sub> and ¹⁷O-excess<sub>Phyto</sub> esti-
mates to be nearest to the observed values, a mean λ<sub>Phyto-LW</sub>
value must be set at 0.521. In this case, the estimated
δ¹⁸O<sub>Phyto</sub> value is 3.44 ‰ higher than the observed one. The
estimated ¹⁷O-excess<sub>Phyto</sub> value is similar to the observed
one (10 per meg difference, Table S3, Fig. 3). Adding a
mixing process with E equals to 0.8 (as is the case for the
bulk adult leaf water estimate, refer to Sect. 6.1) brings the
δ¹⁸O<sub>Phyto</sub> estimate very close to the observed one (differ-
ences in δ¹⁸O<sub>Phyto</sub> and ¹⁷O-excess<sub>Phyto</sub> of 0.51 ‰ and 6 per
meg, respectively) (Table S3 and Fig. 3).

The comparison between modelled and observed isotope
compositions brings insights on the factors driving δ¹⁸OPhyto
and ¹⁷O-excessPhyto in grass leaves. The λPhyto-LW value be-
ing lower than the θsilica-water value of 0.524 calculated after
Sharp et al. (2016) implies that either the θsilica-water value
previously established is overestimated or a kinetic fraction-
ation occurs during phytolith formation. Our modelling ex-
ercise suggests that the amplitude of such a kinetic fraction-
ation would increase from the base to the apex of the leaf
(λPhyto-LW decreasing regularly from 0.522 to 0.520). The
proportion of short cell phytoliths for which silica polymeri-
sation is genetically controlled, decreases from the base to
the apex (Table S2). This would go against a kinetic frac-
tionation being enzymatically controlled. However, further
knowledge on the mechanisms of silica polymerisation is
needed to further discuss this point.

Positions of the phytolith data on the modelled phytolith
curve are not exactly the same as positions of the leaf water
data of the modelled leaf water curve, especially for the api-
cal part. This discrepancy suggests that *E* in the apical leaf
water is higher than *E* in the phytolith-forming water. This
can be explained assuming the following: phytolith-forming
water integrates the whole grass elongation period (Kumar et
al., 2016, 2019; Kumar and Elbaum, 2017) while the sam-
pled leaf water only represents a snapshot. In grass leaf, the
epidermal cells close to the apex were produced at the base of
the leaf and pushed upward during the growth. Hence apical
epidermal cells are older than the cells close to the base, and
phytoliths in these cells gather early and late phytoliths that
are formed at long and short distances relative to the maximal
length, with low and high *E* values, respectively.

For the grass bulk leaf, despite this discrepancy along leaf
length, and assuming a mean λ<sub>Phyto-LW</sub> of 0.521, δ¹⁸O<sub>Phyto</sub>
and ¹⁷O-excess<sub>Phyto</sub> record δ¹⁸O<sub>LW</sub> and ¹⁷O-excess<sub>LW</sub>. In
other terms, whatever the grass leaf length, δ¹⁸O<sub>Phyto</sub> and
¹⁷O-excess<sub>Phyto</sub> should be determinable from the Craig
and Gordon model complemented by an unevaporated-
evaporated water mixing equation. The main controls on
δ¹⁸O<sub>Phyto</sub> and ¹⁷O-excess<sub>Phyto</sub> are thus the soil water and
vapour isotope compositions, the difference of temperature
between leaf water and atmosphere, RH and *E*.

6.4 Potential impact of stem phytoliths on the triple oxygen isotope compositions of grass phytoliths

In addition to grass leaf length, the stem vs. leaf biomass ra-
tio can be very heterogeneous from one grass development
stage to another and from one grass genus to another. Pre-
vious studies showed that phytoliths from grass stems repre-
sent less than 10 % d.w. of the overall above-ground grass sil-
ica content (e.g. Webb and Longstaffe, 2002) even in grasses
with high stem biomass such as bamboos (e.g. Ding et al.,
2008). Stem phytoliths are only weakly enriched in ¹⁸O com-
pared to leaf phytoliths (Webb and Longstaffe, 2006). Thus,
the contribution of stem phytoliths to a soil phytolith assem-
blage should slightly decrease $\delta^{18}$O$_{Phyto}$ and increase ¹⁷O-excess$_{Phyto}$ average values. Assuming a ¹⁷O-excess$_{Phyto}$ difference between stem and bulk leaf of 200 per meg, this would lead to a ¹⁷O-excess$_{Phyto}$ value for stem (10% d.w.) and leaf (90% d.w.) phytolith assemblage higher by 20 per meg relative to an only leaf phytolith assemblage, which is lower than the lowest reproducibility obtained when measuring three aliquots of phytoliths (23 per meg). We conclude that grass physiognomy should impact only very slightly the triple oxygen isotope composition of bulk grass phytoliths.

## 6.5 Impact of senescence on the triple oxygen isotope composition of grass phytoliths

Our data show that 58% of leaf phytoliths form at the end of the growth when the leaf reaches senescence. Leaf senescence is age related or a stress-induced developmental ageing during which transpiration decreases to minimal level but is still efficient (Norton et al., 2014) as epidermal conductance progressively prevails over stomatal conductance (Smith et al., 2006). If the cells already contain dissolved silica, epidermal evaporation, not balanced by water input due to decreasing transpiration at the start of leaf senescence, may lead to silica saturation and polymerisation. Thus, the bulk phytolith assemblage of a senescent leaf will gather phytoliths formed during both the leaf growth and start of senescence. In our experimental conditions, where RH stays constant during both periods, the triple isotope composition of phytoliths stays constant. However, in nature, if RH decreases (e.g. due to seasonal decrease of precipitation in Mediterranean and tropical areas or to colder temperatures in temperate areas) when generalised grass leaf senescence occur, then both periods should be considered when assessing the ¹⁷O-excess$_{Phyto}$ vs. RH relationship from bulk phytolith assemblages from plant, soil or sediment.

## 6.6 Impact of day-night alternations on the triple oxygen isotope composition of leaf water and leaf silica

The results obtained from experiment 2a show very close isotope compositions of leaf water during light and dark periods. The constancy of atmospheric relative humidity and temperature, as well as the shortness of experiment 2a (4 d with dark-light alternations after more than 2 months of constant daylight) may have played against the closure of the stomata at dark. A previous study on elongating leaves of *F. arundinacea* showed that spatial distribution of water content within the elongation zone can stay almost constant during the dark and light period (Schnyder and Nelson, 1988), supporting that dark/light alternations do not always impact the stomata openness. Anyhow, a sensitivity test shows that whatever the stomatal behaviour, change in stomatal conductance does not impact significantly the Craig and Gordon ¹⁷O-excess$_{LW}$ and $\delta^{18}$O$_{LW}$ estimates. Experiment 2b shows that under the

study high RH conditions (60% during the day and 80% during the night in experiment 2b), transpiration, silicification, $\delta^{18}$O$_{Phyto}$ and ¹⁷O-excess$_{Phyto}$ do not vary significantly from constant day to day-night conditions.

## 7 Conclusions

The data and estimates presented here contribute to a more precise identification of the parameters to take into consideration when using the ¹⁷O-excess$_{Phyto}$ as a RH proxy (Alexandre et al., 2018). Neither grass height nor grass physiognomy should significantly impact the isotope composition of bulk grass leaf water and phytoliths. By contrast, RH prevailing at the start of senescence should be considered in addition to RH prevailing during leaf growth when interpreting ¹⁷O-excess$_{Phyto}$. If future studies show that the fractionation between leaf water and phytoliths, expressed by a mean $\lambda_{Phyto-LW}$ value of 0.521, is not climate dependent, then the triple oxygen isotope composition of bulk leaf water should be obtainable from the triple oxygen isotope composition of grassland phytolith assemblages. The parameters driving the triple oxygen isotope composition of both grass leaf water and phytoliths are given by the Craig and Gordon model applied to leaves (Farquhar et al., 2007) and the unevaporated-evaporated water mixing equation. Thus the most important parameters are the difference between soil water and vapour isotope compositions, the difference between leaf and atmosphere temperatures, RH and E. Being able to record the triple oxygen isotope composition of grassland leaf water would bring some significant insights into (i) estimating the triple oxygen isotope composition of CO₂ equilibrated with leaf water and partitioning gross fluxes of CO₂ from vegetation at the regional scale (e.g. Helliker and Ehleringer, 2000) or (ii) estimating at the global scale the triple oxygen isotope composition of O₂ produced by the biosphere and quantifying its productivity from air bubbles trapped in ice cores (Blunier et al., 2002).

*Data availability.* Data may be extracted directly from the current article or requested from the corresponding author.

*Supplement.* The supplement related to this article is available online at: https://doi.org/10.5194/bg-16-4613-2019-supplement.

*Author contributions.* AA, AL, CP, SD, CS, MP and JR designed the experiments and carried them out. AA, AL, CP, SD, CS, MC, JCM, MP and FP did the extractions and isotope analyses. AA prepared the paper with contributions from all co-authors.

*Competing interests.* The authors declare that they have no conflict of interest.
*Acknowledgements.* This study benefited from the CNRS human and technical resources allocated to the Ecotrons Research Infrastructure. We thank Daniel Herwartz, Claudia Voigt and an anonymous reviewer for their in-depth reviews that substantially improved the modelling approach and the paper.

*Financial support.* This research has been supported by INSUL-EFE and the ANR (grant nos. ANR-17-CE01-0002 and ANR-11-INBS-0001).

*Review statement.* This paper was edited by Christopher Still and reviewed by Daniel Herwartz and one anonymous referee.

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