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Short title: Coral optics and variable chlorophyll fluorescence 1
Corresponding authors: [email protected], [email protected] 2
3
Optical properties of corals distort variable chlorophyll fluorescence 4
measurements 5
6
Daniel Wangpraseurt1,2,3a
, Mads Lichtenberg1, Steven L Jacques
4, Anthony WD Larkum
5, 7
Michael Kühl1,5a
8
9
1Marine Biological Section, Department of Biology, University of Copenhagen, 10
Strandpromenaden 5, DK-3000 Helsingør, Denmark 11
2Department of Chemistry, University of Cambridge, Lensfield Road, UK 12
3Scripps Institution of Oceanography, University of California, San Diego, USA 13
4Tufts University, USA 14
5Climate Change Cluster, University of Technology Sydney, Ultimo, New South Wales 2007, 15
Australia. 16
aCorresponding authors 17
18
Author contributions: D.W., M.L., A.W.D.L., M.K. conceived and designed the experiments; 19
D.W., M.L. and A.W.D.L. performed experiments, D.W., S.L.J. and M.K. analysed and 20
interpreted data; D.W. and S.L.J. developed optical models. D.W. wrote the article with 21
contributions from all authors. 22
23
Funding: This study was supported by a Carlsberg Foundation distinguished postdoctoral 24
fellowship (D.W.), a Carlsberg Foundation instrument grant (M.K.), and a Sapere-Aude 25
Advanced grant from the Independent Research Fund Denmark ǀ Natural Sciences (M.K.). 26
27
One-sentence summary: Variable chlorophyll fluorescence is distorted by the optical properties 28
of corals as demonstrated by experimental studies on hydrogel slabs and optical simulations. 29
30
Plant Physiology Preview. Published on January 28, 2019, as DOI:10.1104/pp.18.01275
Copyright 2019 by the American Society of Plant Biologists
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31
ABSTRACT 32
Pulse amplitude modulated (PAM) fluorimetry is widely used in photobiological studies of 33
corals, as it rapidly provides numerous photosynthetic parameters to assess coral ecophysiology. 34
Coral optics studies have revealed the presence of light gradients in corals, which are strongly 35
affected by light scattering in coral tissue and skeleton. We investigated whether coral optics 36
affects variable chlorophyll fluorescence measurements and derived photosynthetic parameters 37
by developing planar hydrogel slabs with immobilized microalgae and with bulk optical 38
properties similar to those of different types of corals. Our results show that PAM-based 39
measurements of photosynthetic parameters differed substantially between hydrogels with 40
different degrees of light scattering but identical microalgal density, yielding deviations in 41
apparent maximal electron transport rates by a factor of 2. Furthermore, system settings such as 42
the measuring light intensity affected F0, Fm and Fv/Fm in hydrogels with identical light 43
absorption but different degrees of light scattering. Likewise, differences in microalgal density 44
affected variable chlorophyll fluorescence parameters, where higher algal densities led to greater 45
Fv/Fm values and relative electron transport rates. These results have important implications for 46
the use of variable chlorophyll fluorimetry in ecophysiological studies of coral stress and 47
photosynthesis, as well as other optically dense systems such as plant tissue and biofilms. 48
49
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INTRODUCTION 50
The ecological success of coral reefs is largely due to the successful symbiotic relationship 51
between the coral animal host and its photosymbiotic microalgae belonging to the genus 52
Symbiodinium. This highly efficient symbiotic interaction is susceptible to changes in 53
environmental conditions, such as excess solar radiation and above-average seawater 54
temperatures, which can lead to the breakdown of the coral-algal symbiosis and the visible 55
paling of the coral colony known as coral bleaching (Weis, 2008). Given the importance of 56
Symbiodinium photosynthesis for coral health, coral photosynthesis has been studied intensively 57
from molecular to environmental scales (Dubinsky and Falkowski, 2011; Falkowski et al., 1990). 58
Coral photosynthesis can be studied with techniques quantifying photosynthetic O2 production or 59
carbon fixation (Hoogenboom et al., 2012; Kühl et al., 1995; Osinga et al., 2012), but 60
photophysiological measurements based on variable chlorophyll (Chl) a fluorescence are now 61
widely used in coral research and many other areas of terrestrial and aquatic photosynthesis 62
research (Ralph and Gademann, 2005; Szabó et al., 2014; Warner et al., 1996; Warner et al., 63
2010). In contrast to gas exchange or C-fixation measurements that require significant sample 64
handling, variable chlorophyll fluorescence relies on optical light pulsing schemes that are 65
applied externally with minimal sample manipulation or directly in the natural habitat, and a 66
variety of commercial instruments for cuvette-based, fiber-optic or imaging measurements are 67
available (e.g. Schreiber, 2004). In coral reef science, pulse amplitude modulated (PAM) 68
chlorophyll a fluorimeters are by far the most commonly used instrument to probe 69
photosynthesis (Warner et al., 2010). 70
Variable chlorophyll fluorimetry quantifies the fate of absorbed light energy trapped by 71
the photosynthetic apparatus via changes in Chl a fluorescence, which tracks the redox status of 72
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photosystem (PS) II and the balance between photochemical and non-photochemical quenching 73
processes. PAM-based measurements employ the so-called saturation pulse method (Schreiber, 74
2004). The PAM technique generates multiple photochemical charge separations (multiple 75
turnover) and fully reduces QA via the application of 50–1000-ms multiple turnover flashlets 76
(‘fat flashes’) (see Kromkamp and Forster, 2003). The fluorescence yield prior to the saturation 77
pulse indicates the level of fluorescence when QA is maximally oxidized and PSII reaction 78
centres are fully open. Such minimum fluorescence yield is denoted as F0 and F, referring to 79
dark- and light-acclimated samples, respectively. The saturation pulse is assumed to lead to the 80
complete closure of PSII reaction centers, such that photochemical quenching is fully inhibited 81
(Schreiber et al., 1993). Consequently, fluorescence emission is maximal and this parameter is 82
known as the maximal fluorescence yield, where Fm and Fm’ refer to dark- and light-acclimated 83
samples, respectively (Schreiber, 2004). From these measurements, many derived parameters 84
describe the photophysiology of the investigated sample. 85
In coral reef science, the most frequently used fluorescence parameter is the maximum 86
PSII quantum yield, which is calculated from saturation pulse measurements on dark-acclimated 87
samples as follows: Fv/Fm = (Fm-F0)/Fm. The Fv/Fm parameter is considered a key proxy for coral 88
health, and differences in Fv/Fm between coral measurements are interpreted as a change in coral 89
fitness (Jones et al., 2000; Wiedenmann et al., 2013). The effective quantum yield of PSII, 90
ФPSII= (Fm’-F)/Fm’, is determined via a saturation pulse measurement under a known actinic 91
irradiance of photosynthetic active radiation (PAR) (Genty et al., 1989). An estimate of the 92
relative PSII-derived photosynthetic electron transport rate is calculated as rETR = ФPSII x PAR 93
(Ralph and Gademann, 2005), whereas determination of the absolute ETR requires information 94
about the PSII absorption cross section (Szabó et al., 2014). When calculated over a range of 95
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actinic irradiance levels, rETR versus irradiance curves (i.e. light curves) can be determined, 96
which enables the calculation of the maximum electron transport rate (ETRmax) and the light-use 97
efficiency factor (α), i.e., the initial slope of the rETR vs irradiance curve. Measurement 98
protocols for the application of PAM on corals are well-described (e.g. Warner et al. 2010), and 99
the maximum PSII quantum yield and rETR vs irradiance curve parameters are frequently used 100
to interpret the health and photo-physiological acclimation state of Symbiodinium within the 101
coral host (Ralph et al., 2005). 102
However, the application of variable chlorophyll fluorescence is based on the 103
assumptions that all photosynthetic entities (cells/chloroplasts) are (i) equally exposed to the 104
incident actinic light levels, (ii) equally exposed to the measuring light and emitting fluorescence 105
equally, and (iii) effectively saturated by the saturation pulse (Schreiber et al., 1996; Serôdio, 106
2004). In other words, it is assumed that (1) each photosynthetic cell has identical fluorescence 107
excitation/emission, and (2) the generated fluorescence from each cell has equal probability to be 108
detected by the fluorimeter. These assumptions are only met, if the light distribution within the 109
sample is homogenous, such as in optically dilute algal cultures (see e.g. Ting and Owens, 1992). 110
In contrast, most photosynthetic tissues exhibit strong scattering and absorption, leading to a 111
heterogenous distribution of irradiance within the sample (e.g., Evans, 2009; Evans et al., 2017; 112
Oguchi et al., 2011, Lichtenberg et al., 2017; Serôdio, 2004; Szabó et al., 2014). For instance, 113
steep light gradients exist in biofilms (Kuhl et al. 1994) which can lead to an effective 114
overestimation of ФPSII and ETR (Serôdio, 2004). Such gradients can also affect measurements 115
of the Chl a fluorescence kinetics (Susila et al., 2004). Re-absorption of fluorescence emission 116
can pose a challenge for Chl a fluorimetry in optically dense tissues (Naus et al., 1994; 117
Bartošková et al., 1999). A method for correcting variable fluorescence measurements in 118
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optically dense algal media under constant optical geometries (e.g. cuvettes) has been proposed 119
(Klughammer and Schreiber, 2015), but this approach assumes a simple exponential light 120
attenuation (Lambert-Beer’s law), which is too simplistic for light-scattering photosynthetic 121
tissues (Kuhl et al. 1994, Wangpraseurt et al. 2016). 122
Knowledge of the tissue inherent optical properties (IOPs) allows us to predict light 123
propagation by solving the radiative transfer equation. The IOPs are defined as the probability of 124
light absorption per infinitesimal path length (µa, [mm-1
]), the probability of light scattering per 125
infinitesimal path length (µs, [mm-1
]), the anisotropy of scattering (g) (i.e. the average cosine 126
⟨cos θ⟩ of the scattering angle θ), and the refractive index (n). In strongly light-scattering 127
samples, µs is combined with g to define the reduced scattering coefficient µs’ = µs · (1-g) 128
(Jacques et al. 2013). The reduced scattering coefficient describes photon diffusion in a random 129
walk of step sizes of 1/ µs’, where each step involves isotropic scattering. Recent progress in 130
coral optics (Swain et al., 2016; Wangpraseurt et al., 2016a; Wangpraseurt et al., 2014b) revealed 131
that coral tissues and skeletons can be strongly light-scattering and that µs’ is variable between 132
coral species. For instance, µs’ of coral skeletons can vary by one order of magnitude (Marcelino 133
et al., 2013), thus substantially affecting the amount of light that is backscattered into the 134
overlying algal layer (Marcelino et al., 2013; Wangpraseurt et al., 2016a). Thick-tissued corals 135
can have light-scattering host pigments (e.g. green fluorescent protein, GFP) situated on top of 136
the algal layer (Lyndby et al., 2016; Wangpraseurt et al., 2017b). In such a scenario, light is 137
effectively scattered before it reaches Symbiodinium cells, leading to a strong surface 138
enhancement of scalar irradiance, E0 (=fluence rate) (Lyndby et al., 2016). 139
The absorption coefficient (µa) of corals is largely dependent on Symbiodinium cell 140
density and Chl a content per cell (Wangpraseurt et al. 2016). Algal densities in corals vary 141
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seasonally (Chen et al., 2005) and in response to environmental stress (Glynn, 1996). 142
Symbiodinium density affects vertical light attenuation, where densely pigmented corals are 143
characterised by steep light gradients, while less-pigmented corals have a diffusely enhanced 144
tissue light environment (Wangpraseurt et al. 2017). The photosynthetic yield of Symbiodinium 145
can be vertically stratified within the coral tissue (Lichtenberg et al., 2016; Wangpraseurt et al., 146
2016b). During coral bleaching, microalgal symbionts experience photoinhibition (Warner et al., 147
1999) and such damage is likely more prominent in the light-exposed top layers of coral tissue 148
(Lichtenberg et al., 2016; Wangpraseurt et al., 2016b). Corals thus represent a challenging study 149
organism for variable Chl fluorimetry; yet, to our knowledge, no studies have aimed at ground 150
truthing the central assumptions of PAM measurements on corals. 151
The use of natural coral samples for such study would be easily contrived by variability 152
of the inherent optical properties of individual samples (e.g. changes in µa, µs’). To avoid this 153
variability, we developed optical analogues to corals using a biomedical tissue optics approach. 154
Optical phantoms are often created to solve problems related to the propagation of light in 155
scattering tissues, e. g., for calculating the light dose in photodynamic therapy and cancer 156
treatment (Pogue and Patterson, 2006). The optical response of human tissue is mimicked by 157
optical phantoms consisting of (1) a gel-like planar matrix (e.g. gelatin, agar or agarose), (2) 158
light-scattering particles (e.g. SiO2, TiO2, polystyrene microspheres) and (3) light absorbers (e.g. 159
intralipid, india ink) (Tuchin, 2007). 160
In this study, we created multiple planar hydrogel slabs to replicate the bulk optical 161
properties of corals and characterised their variable Chl fluorescence-derived parameters, 162
including Fv/Fm, Y(II) and rETR (Supplemental Table S1). Specifically, we examined the role of 163
light scattering by replicating three major coral categories: (1) corals with strongly 164
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backscattering skeletons (‘skeleton’ hydrogel), (2) corals with low-scattering skeletons 165
(‘transparent’ hydrogel) and (3) corals with light scattering in skeleton and tissue (e.g. due to 166
GFP host pigments) (‘GFP’ hydrogel). We also assessed the role of light absorption for Chl a 167
fluorimetry by creating hydrogels with different microalgal densities and PS II efficiencies. 168
Furthermore, we developed a light-propagation model (chlorophyll fluorescence Monte Carlo 169
simulation, Chf-MC) that allows for prediction of the generated fluorescence and detected 170
fluorescence as a function of tissue optical properties. Although we focused on the widely 171
applied PAM method, it is also relevant for other variable Chl fluorescence methods such as fast 172
repetition rate fluorimetry (Gorbunov et al., 2001). The optical phantom approach (Fig. 1) and 173
numerical models can easily be altered to address identical questions in other light-scattering 174
samples such as leaves and biofilms. 175
RESULTS 176
Effects of measuring light settings and light scattering on variable chlorophyll fluorescence 177
Hydrogels with identical absorber density but different light-scattering properties showed up to 178
5-fold differences in F0 for the same measuring light (ML) intensity (Fig. 2 a-d). Highest F0 179
values were achieved for the skeleton hydrogel (F0=0.162, Fig. 2 b,d). ML intensity also affected 180
measurements of the maximal fluorescence yield (Fm) and the calculation of Fv/Fm (Fig. 2 e-f). 181
For ML=3-4, Fv/Fm values were about 0.74 for all three coral-mimicking hydrogels, while for 182
ML=<3 and >5, Fv/Fm values differed by up to 0.1 (Fig. 2f). 183
The in vivo light microenvironment measured with fibre optic microsensors differed for 184
the three coral-mimicking hydrogels, and photon scalar irradiance (400–700 nm) at the hydrogel 185
surface reached 109% (±0.85 SE; n=8) of the downwelling photon irradiance, Ed (Supplemental 186
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Table S1) for the transparent hydrogel, 142% Ed (±9 SE; n=8) for the skeleton hydrogel, and 187
244% Ed (± 12.3 SE; n=8) for the GFP hydrogel (Fig. 3). The steepest light attenuation was 188
measured in the GFP hydrogel, and the lowest, in the transparent hydrogel (Fig. 3). The top layer 189
(0 µm to 750 µm) of the light-scattering GFP hydrogel (Fig. 1d) created a subsurface maximum 190
in scalar irradiance (at about 250 µm below the hydrogel surface); this was followed by rapid 191
light attenuation within the light-absorbing algal layer (750 µm to 1500 µm). For the skeleton 192
hydrogel, light attenuated to 125% Ed within the first 300 µm, after which light scattering by the 193
underlying layer caused a subsurface maximum around 700 µm from the hydrogel surface that 194
reached 170% Ed (Fig. 3). 195
Steady-state light curves revealed that the effective quantum yield of PSII (ФPSII) and the 196
derived relative electron transport rates (rETR) differed between the three coral-mimicking 197
hydrogels (Fig. 4a-d), where the shape of the curves depended on the light field parameter used 198
to quantify the actinic light level. When plotted as a function of downwelling photon irradiance 199
(Ed), the ФPSII was higher for the GFP hydrogel than for the skeleton and transparent hydrogel, 200
and this difference was larger for rETR calculations. For instance, at Ed =1000 µmol photons m-2
201
s-1
, rETR was about 1.5 times higher for the GFP vs the other two hydrogels (Fig. 4c). Correction 202
of ETR for in vivo scalar irradiance (E0) led to similar patterns between the GFP and skeleton 203
hydrogel, which now both showed higher rETRs than the transparent hydrogel (Fig. 4d). 204
Effects of light absorption on variable chlorophyll fluorescence 205
We constructed hydrogels with identical scattering properties but different light absorption 206
properties (Fig. 1j-m). Surface photon scalar irradiance (400–700 nm) in the hydrogel with 207
medium algal density (1.0 x 106 cells cm
-2) was about 1.4-fold higher than that in the hydrogel 208
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with high algal density (3.5 x 106 cells cm
-2) (205% Ed ±. 0.27 SE vs 146% Ed ±. 0.51 SE; n=4). 209
This difference increased as a function of vertical depth, and measurements at depths of >2000 210
µm showed up to 3-fold enhanced scalar irradiance values in the medium- vs high–algal-density 211
hydrogel (Fig. 5a). 212
Microalgal density had a significant effect on estimates of the maximum quantum yield, where 213
hydrogels with 3.5 x 106 cells cm
-2 showed about 0.04 units higher Fv/Fm values than hydrogels 214
with 1.0 x 106 cells cm
-2 (student’s t-test: t(6)=11.25, p<0.01, Fig. 5b). Likewise, microalgal 215
density affected rETR, and at Ed=500 µmol photons m-2
s-1
, rETR was about 2.7-fold higher for 216
the high vs medium algal density hydrogel (rETR= 41.1 ± 0.1 vs 14.7 ± 0.8; n=4) (Fig. 5c). 217
Additionally, rETR values were corrected for the in vivo scalar irradiance, as determined with 218
scalar irradiance microsensors for each respective photic zone (i.e. the hydrogel layer that 219
contained microalgal cells). Correction for in vivo scalar irradiance slightly improved this 220
discrepancy, but calculations of rETRmax and the light-use efficiency factor (α) were still about 221
1.35 (rETRmax=80 vs 59) and 2-fold higher (α=0.22 and 0.11) for high- vs medium–algal-density 222
hydrogels. 223
Effects of bio-optical properties and simulated coral bleaching on variable chlorophyll 224
fluorescence 225
Hydrogels mimicking a stressed but not bleached coral, i.e., harbouring a top layer with high 226
algal density but low photosynthetic potential, showed low rETR and onset of photoinhibition 227
(Fig. 6). However, hydrogels mimicking a partially bleached and stressed tissue, i.e., harbouring 228
a top layer with reduced microalgal density and photosynthetic potential, showed moderate rETR 229
with rETRmax = 38 (at Ed> 500 µmol photons m-2
s-1
) and no signs of photoinhibition (Fig. 6). 230
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DISCUSSION 231
Variable chlorophyll fluorimetry is a key tool for probing photosynthesis in vivo (Baker, 2008). 232
However, the assumptions underlying the calculation of variable chlorophyll fluorescence 233
parameters might not be fulfilled when measuring externally on highly stratified and dense 234
photosynthetic tissues, such as corals, biofilms and plant tissues (Evans, 2009; Serôdio, 2004; 235
Szabó et al., 2014). Our results showed that F0, Fm and Fv/Fm were affected by the scattering 236
properties of coral-mimicking hydrogels (Fig. 2). In a first approximation, we can describe the 237
detected F0 signal by using three simple terms: (1) the measuring light intensity incident on an 238
algal cell, i.e., fluorescence excitation, (2) the fluorescence emission per cell, which is governed 239
by the bio-physical properties of the cell, such as Chl a content and dark acclimation (Warner et 240
al., 2010), and (3) the probability that such emitted fluorescence is detected by the imaging 241
instrument (fluorescence escape) (see supplementary information). Because algal cells can 242
collect light from all directions, the excitation term is not described by the downwelling 243
irradiance of the measuring light, but by the scalar irradiance (=fluence rate) of measuring light 244
(Kühl et al., 1995), which in turn is affected by the tissue optical properties (Jacques, 2013) (see 245
optical simulations in supplementary information). In the first experiment (Fig. 1), we kept µa 246
constant while modulating µs’, which created characteristic differences in the light 247
microenvironment between three different coral tissue mimics (Fig. 3). The enhancement of 248
photon irradiance at the tissue surface of the skeleton hydrogel was due to the strong 249
backscattering (Fig. 3). In contrast, light attenuation was described by a simple exponential 250
attenuation for the transparent hydrogel (Fig. 3). 251
The observed differences in the F0 signal between the skeleton and transparent hydrogels 252
for a given measuring light intensity were due to two mechanisms (Fig. 7). Firstly, the fluence 253
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rate of the measuring light was enhanced in the absorbing layer (0–750 µm depth) for the 254
skeleton vs. the transparent hydrogel (Fig. 3). The higher fluence rate led to an increased chance 255
of photon absorption and thus higher levels of fluorescence generation (see optical simulations in 256
Supplemental Figure S2). Secondly, although an individual algal cell acts as an isotropic point 257
source (i.e. emitting fluorescence equally well in all directions) (Schreiber, 2004), the detected 258
fluorescence signal depends on the propagation of fluorescent light from this point source, 259
through the tissue towards the fluorimeter (Welch et al., 1997). Because intact corals are 260
typically monitored externally using a fiber or camera in backscattering configuration, the 261
reflectivity of the skeleton controls the upwelling fluorescence towards the detector. For the 262
transparent hydrogel, the downwelling fluorescence was essentially lost, while backscattering by 263
the skeleton hydrogel led to an effective redirection of the otherwise-lost downwelling 264
fluorescence (Fig. 7). 265
For the GFP hydrogel, the light-scattering elements were placed on top of the light-266
absorbing algal layer (Fig. 1). Scattering diffuses the incident light, and diffuse light penetrates 267
less into biological tissue than collimated light (Tuchin, 2007; Wangpraseurt and Kühl, 2014) 268
(Supplemental Figure S2). Thus, although intense scattering in the top tissue layer would 269
enhance the chance of fluorescence emission and subsequent upwelling of generated 270
fluorescence, it also leads to a steep attenuation of the measuring light within the algal layer 271
(Lyndby et al., 2016; Fig. 3, Supplemental Figure S2). The vertical attenuation of photon scalar 272
irradiance (400–700 nm) within the light-absorbing layer was described according to Lambert–273
Beer’s law for the transparent and GFP hydrogels, yielding an attenuation coefficient that was 274
1.4-fold higher for the GFP vs. transparent hydrogel (1.7 mm-1
and 1.2 mm-1
, respectively; data 275
not shown). Together, these results exemplify that the F0 signal can be strongly affected by the 276
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13
scattering properties of the photosynthetic tissue and the spatial arrangement of light-scattering 277
vs light-absorbing elements in the tissue. 278
Our results suggest that coral light-scattering modulated (i) the ability of the saturation 279
pulse to fully saturate PSII, (ii) the likelihood for actinic effects during ML probing, and (iii) the 280
operational volume that is probed during Fv/Fm measurements (Fig. 7). Fv/Fm values for the 281
skeleton hydrogel were more than 0.1 units (dimensionless) higher than for the transparent and 282
GFP hydrogels when probed with low ML intensities (Fig. 2). This likely indicates that skeleton 283
backscattering facilitated the full saturation of all photosynthetic cells within the tissue volume, 284
creating a homogenous light environment (Fig. 3) (Enriquez et al., 2005). In contrast, the steep 285
light gradient in the GFP hydrogels led to rapid attenuation of the saturation pulse light (Fig. 3), 286
leaving only about 50% of Ed in the lowest layers of the photic zone. In such a scenario, the 287
likelihood of incomplete PSII saturation increases with vertical tissue depth (Serôdio, 2004), thus 288
inducing lower Fm values for deeper tissue layers. Optical simulations using Chf-MC showed that 289
increased tissue scattering (from µs’=1 mm-1
to 10 mm-1
) reduced the tissue depth for which PSII 290
was fully saturated by >50% (for µa=0.1–1 mm-1
) (see supplementary information and 291
Supplemental Figure S4b). Chf-MC can serve as an initial point of reference for assessing the 292
likelihood of incomplete PSII saturation in the sample (Supplemental Figure S4b). Other 293
approaches, including the multiphase flash method, which uses ~1-s–long multiphase flashes to 294
saturate PSII, could provide additional instrument improvements that reduce the likelihood of 295
incorrect Fm’ estimates (Loriaux et al., 2013). 296
Optical scattering affected the ML intensity within the photosynthetic tissue and thus the 297
likelihood of ML inducing actinic effects (Supplemental Figure S5). The relationship between 298
measuring light used to probe for F and Fm can be nonlinear at higher light intensity settings, 299
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14
leading to a decrease in the Fm to F ratio and thus a reduction in Fv/Fm values (Ting and Owens, 300
1992). Such non-linearity is caused by instrument optics, and although this has been tested only 301
for the PAM 101 (Ting and Owens, 1992), it is likely that the same artefacts contributed to the 302
observed decrease in Fv/Fm for higher ML settings when using the I-PAM system (Fig. 2f). 303
Light scattering affected the operational volume of the PAM instrument, i.e. the 304
contribution of fluorescence from different vertical tissue depths to observed fluorescence from 305
the sample (Supplemental Figures S2, S4a). For samples containing photosynthetic cells with 306
variable intrinsic PS II efficiency, differences in the operational volume could lead to a complex 307
mixture of fluorescence signals from different tissue depths (Fig. 6). Such mixed fluorescence 308
signals could theoretically be decomposed by calculating the depth-specific contribution to 309
observed fluorescence using Chf-MC (supplementary information). However, it is a pre-requisite 310
that the intrinsic properties of PS II efficiency are known (Klughammer and Schreiber, 2015). 311
The effective quantum yield of PSII (ФPSII) and rETR differed between the three light-312
scattering coral mimics (Fig. 4), and the rETR of the GFP hydrogel was greater than that of the 313
skeleton and transparent hydrogels when calculated with Ed as a measure of actinic light (Fig. 314
4c). Using the average E0 within the photic zone as a measure of actinic light reduced the 315
difference in rETR between the GFP and skeleton hydrogels, and the two light curves were 316
identical for E0 <400 µmol photons m-2
s-1
. This suggests that for low actinic light levels, 317
measurements of the average in vivo scalar irradiance within the entire photic zone can, to some 318
extent, correct for rETR estimates from corals with different degrees of light scattering 319
(Marcelino et al., 2013). For higher actinic irradiance, such correction was not successful, and 320
rETR was greater for the GFP hydrogel than for the skeleton hydrogel (Fig. 4d). The 321
enhancement of rETR in the GFP scenario was likely due to the presence of the steep light 322
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15
gradient (Fig. 3), ensuring that the irradiance incident on lower cell layers enabled optimal 323
conditions for photosynthesis. 324
We found that both Fv/Fm and rETR were reduced for hydrogels with lower microalgal 325
cell density (Fig. 5b-d). Lower microalgal cell density decreased light absorption, which 326
enhanced the internal light microenvironment (Fig. 5a) and consequently lowered ФPSII. Given 327
that rETR is calculated by multiplying ФPSII with PAR, differences in the internal light 328
microenvironment can lead to substantial artefacts in the calculation of rETR (Fig. 4c). 329
Additionally, correct calculations of absolute ETR require knowledge of the absorption factor 330
(AF), which in itself is affected by optical scattering (Supplemental Figure S6; Szabo et al. 331
2014). 332
The Fv/Fm measurements were performed for hydrogels with different absorber densities 333
(at ML=2), which yielded the same F0 but higher Fm values for the hydrogel with enhanced 334
microalgal cell densities. Although the exact mechanisms underlying these differences are 335
unclear, these first measurements have important implications for coral science, given that 336
microalgal cell density is highly variable between coral species (Drew, 1972) and within a 337
species due to factors such as differences in light acclimation (Falkowski and Dubinsky, 1981), 338
seasonal fluctuations (Chen et al., 2005), and environmental stress (e.g. coral bleaching) (Weis, 339
2008). Bleached corals can exhibit an approximate doubling of the fluence rate within coral 340
tissues compared to healthy corals (Swain et al., 2016; Wangpraseurt et al., 2017a), and such 341
change in the internal light microenvironment was successfully mimicked with our hydrogels 342
with different absorber densities (Fig. 5a). Thus, differences in Fv/Fm and rETR between coral 343
individuals with different algal cell densities should be interpreted with caution and might, to 344
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16
some extent, reflect different optical properties as well as differences in photophysiological 345
status. 346
PAM-based measurements are often used to assess changes in photochemical efficiency 347
during coral bleaching (Jones et al., 2000; Rodriguez-Roman et al., 2006). During such 348
environmental stress, both the optical properties of the coral and ФPSII of the algal symbiont 349
undergo changes over time (Iglesias-Prieto et al., 1992; Wangpraseurt et al., 2017a). Cells from 350
top layers exposed to supra-optimal irradiance are likely to be stressed to a greater extent than 351
cells from deeper layers (Lichtenberg et al., 2016; Wangpraseurt et al., 2016b). We found that 352
changes in cell density and spatial differences in ФPSII lead to a misinterpretation of variable 353
fluorescence signals. For instance, hydrogels mimicking stressed corals by containing a top layer 354
with normal algal cell density but with reduced photochemical efficiency, showed much lower 355
rETR than hydrogels mimicking bleached corals (see Fig. 1 and Table 1 for hydrogel 356
configurations). The high density of the low-performing cells in the top hydrogel layer, limited 357
the operational volume in the stressed-coral scenario. In contrast, a reduction in the cell density 358
of top layers, enhanced the operational volume to measurements of well-performing lower cell 359
layers, effectively enhancing rETR (Fig. 6). 360
The present experimental study has shown that coral optical properties can contrive the 361
interpretation of PAM-based fluorescence measurements. The next step is to develop theoretical 362
models that predict the likelihood of optical artefacts in a sample and ideally correct for such 363
artefacts. We have taken first steps by developing a Chl a fluorescence Monte Carlo model (Chf-364
MC) for photosynthetic tissues that allows for predicting the likelihood of PSII saturation, the 365
actinic effects of ML, the operational volume and depth distribution of the collected fluorescence 366
(see supplementary information). The simulations can be adjusted to account for absorption of 367
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17
emitted fluorescence. The optical model is limited to a 1-layer system, which is best applicable 368
to structurally simple photosynthetic tissues. Future efforts should include the modelling of 369
chlorophyll a fluorescence in multiple tissue layers and in a 3D architecture (Fang, 2010). The 370
use of tissue phantoms with defined optical properties is a promising approach to examine and 371
qualify the precision of variable chlorophyll fluorimetry in plant tissues and biofilms. 372
Quantification of inherent optical parameters in photosynthetic tissues might furthermore lay the 373
experimental basis for better light-propagation models (Jacques, 1998; Mycek and Pogue, 2003; 374
Swartling et al., 2003), which will enable optimal measurement protocols and instrument 375
configurations. 376
METHODS 377
Experimental approach 378
Experiment 1 was aimed at understanding how differences in coral light scattering affect variable 379
chlorophyll fluorescence measurements in identical algal populations, i.e., same algal culture at 380
identical cell densities. Thick-tissued faviid corals often have light-scattering GFP granules on 381
top of the light-absorbing algal layer, which is also subject to light scattering from the coral 382
skeleton (Lyndby et al., 2016; Wangpraseurt et al., 2017b). The ‘GFP’ hydrogel consisted of a 3-383
layer system with a thin (750 µm) light-scattering upper layer (mimicking GFP scattering), a 384
light-absorbing layer (algae), and a thick light-scattering base layer (skeleton) (Fig. 1, Table 1). 385
However, not all corals follow this tissue arrangement, and other corals do not have light-386
scattering GFP granules. In thin-tissued corals, light scattering can be dominated by the 387
backscattering properties of the skeleton (Enriquez et al., 2005). To mimic this optical 388
configuration, the ‘skeleton hydrogel’ was prepared to be identical to the GFP hydrogel but 389
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18
without the top GFP layer. In the ‘transparent’ hydrogel, the light-scattering skeleton layer was 390
replaced with a 1% agarose gel layer (see schematics in Fig. 1). 391
In Experiment 2, we examined how changes in coral light absorption might affect 392
variable chlorophyll fluorescence measurements. In healthy corals, algal densities can vary 393
seasonally from approximately 1.5 to 6 x 106 cells cm
-2 (Chen et al., 2005). We therefore created 394
hydrogels with microalgal densities of 3.5 x 106 cells cm
-2 (‘high density’) and 10
6 cells cm
-2 395
(‘medium density’) (Fig. 1, Table 1). 396
Experiment 3 mimicked a coral stress scenario in order to explore systematically, how 397
combined changes in microalgal density and photophysiology affect variable chlorophyll 398
fluorescence measurements in corals. We mimicked a ‘stressed coral’, where top algal layers 399
have reduced photosynthetic quantum yields, while lower layers are operating with high yields. 400
For this, we created a light-absorbing algal layer with Nanochloropsis sp. (thickness = 750 µm, 401
algal density = 2 x 106 cells cm
-2) on top of a Rhodomonas salina layer (thickness = 750 µm, 402
algal density = 2 x 106 cells cm
-2), exhibiting a Fv/Fm = 0.7. The double layer was placed on top 403
of the light-scattering skeleton hydrogel. We also created a hydrogel mimicking a ‘stressed and 404
bleached coral’ by using a reduced density of Nanochloropsis (3 x 105 cells cm
-2) in the top layer 405
(Table 1). The ‘healthy coral’ consisted of two layers of Rhodomonas salina (each 750 µm thick 406
and with an algal density of 2 x 106 cells cm
-2) on top of the high-backscatter hydrogel. 407
Hydrogel fabrication 408
To develop a hydrogel with light-scattering properties similar to those of corals, we used a 409
protocol developed for human tissues (Wagnières et al., 1997), where hydrogels with tissue-like 410
properties for visible light were constructed with a reduced scattering coefficient of µs’= 1.5 – 411
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19
3.4 cm-1
between 400 to 450 nm (Wagnières et al., 1997). The reduced scattering coefficient of 412
coral skeletons is highly variable, with µs’ ranging between 3 and 140 cm-1
(Marcelino et al., 413
2013; Swain et al., 2016), and the optical properties of living coral tissue apparently exhibit a 414
similar variability (Wangpraseurt et al., 2016a). Given the variability in coral scattering, we did 415
not aim to quantify in detail the reduced scattering coefficient of our hydrogel, but rather to 416
develop a hydrogel that falls within the bulk part of light scattering observed in corals. 417
The developed hydrogels were composed of (1) a gel-like matrix, (2) light-scattering 418
particles, and (3) light-absorbing algae. We used a 1% agarose (Ultrapure low-melting-point 419
agarose; Thermo Scientific, Rochford, USA) solution in filtered (0.2 µm) seawater, which is 420
rather optically clear in the visible part (Wagnières et al., 1997). The agarose was prepared by 421
heating the agarose-seawater mixture in a microwave, ensuring that the solution was clear and 422
free of gas bubbles. The low agarose concentration ensured that the hydrogel was mechanically 423
similar to soft tissues such as coral tissue and exhibited gas diffusion properties similar to 424
seawater. Light scattering was achieved by mixing the hydrogel with defined concentrations of 425
silicon dioxide particles (size fraction: 99% between 0.5 – 10 µm and 80% between 1-5 µm, 426
Sigma Aldrich, USA) to achieve the desired scattering (see Table 1) (Wagnières et al., 1997). 427
Such silicon dioxide particles are non-toxic to microalgae and cyanobacteria (Dickson and Ely, 428
2013) and exhibit a good broadband scattering of white light at the chosen particle size 429
distribution (Wagnières et al., 1997). 430
After adding the silicon dioxide particles, the agarose solution was vortexed for about 30 431
seconds, ensuring a homogenous distribution of the light-scattering particles. The solution was 432
cooled down to about 30ºC, after which the microalgae were added at defined concentrations 433
(see Fig. 1). We selected two types of light-absorbing microalgae, Symbiodinium sp. and 434
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20
Rhodomonas salina. Preliminary experiments were performed with Symbiodinium sp., while the 435
main experiments were performed with Rhodomonas salina, which was similar in cell size (8–10 436
µm) and was easier to grow and maintain in a healthy state. For both algal species, PAM-437
relevant blue light absorption is dominated by Chl a along with additional contributions by Chl c 438
(Kaňa et al., 2013; Wangpraseurt et al., 2014). However, for the purpose of this study, the type of 439
algal strain is largely irrelevant, as we investigated the effect of basic light-scattering 440
mechanisms on variable Chl a fluorescence measurements. The solution of agarose, SiO2 and 441
microalgae was transferred rapidly into petri dishes (diam. 35 mm, height 10 mm), where they 442
were left to cure for at least 30 min. 443
Apparent optical properties of tissue hydrogels 444
The light microenvironment of coral mimics was measured in vivo using scalar irradiance 445
microsensors (Rickelt et al., 2016) as described in detail elsewhere (Kühl, 2005; Wangpraseurt et 446
al., 2012). Briefly, scalar irradiance probes were constructed with a spherical isotropic light-447
collecting tip of ~80 µm (Rickelt et al. 2016). The probe was mounted on a motorised 448
micromanipulator (PyroScience GmbH, Germany) controlled by a PC running dedicated 449
software (Profix; PyroScience GmbH, Germany) and oriented at an angle of ~45º relative to the 450
vertically incident light. Measurements of spectral scalar irradiance were performed from the 451
surface of the hydrogel in vertical step sizes of 80 µm. The spectral scalar irradiance was then 452
integrated over the spectral range of photosynthetically active radiation (PAR, 400–700 nm) and 453
expressed in percentage of the incident downwelling irradiance (Ed) (Kühl 2005). 454
Variable chlorophyll fluorescence imaging 455
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21
We used a variable chlorophyll fluorescence imaging system (Mini I-PAM, Walz, Effeltrich, 456
Germany) (Ralph et al., 2005; Kühl and Polerecky, 2008). The I-PAM was equipped with blue 457
LEDs (460 nm) and delivered a maximum saturation pulse intensity (SP =10) of >2700 µmol 458
photons m-2
s-1
. The ML intensity was calibrated for ML1-12 at frequency 1 using a fast data 459
logger (ULM 500, Walz GmbH, Germany) connected to cosine-corrected PAR sensor, yielding 460
an average photon irradiance output of 0.3, 0.4, 0.6, 0.8, 1, 1.2, 1.4, 1.6, 1.8, 2.1, 2.3, 2.6 µmol 461
photons m-2
s-1
. The I-PAM system was mounted on a heavy stand and the hydrogels 462
illuminated vertically from above. Initial measurements were performed to calibrate the focal 463
distance and aperture settings between the camera head and hydrogel samples, after which, focus 464
and aperture were fixed. All measurements were performed with the hydrogels within petri 465
dishes that were placed on top of a black light-absorbing surface. Measurements were performed 466
in a darkened room. 467
Measurements were performed with dark-acclimated samples (after about 30 min in 468
darkness) to examine differences in the background fluorescence between the ‘transparent, 469
‘skeleton’ and ‘GFP’ hydrogels. For each measurement, the PAM settings were fixed (measuring 470
light intensity, ML= 4, gain=1, damping=2, frequency=1). Measurements were also performed to 471
examine the effects of changes in measuring light intensity on F0, Fm and the calculated Fv/Fm. 472
Each sample was measured at a range of measuring light intensities (ML settings ranging 473
between 1 and 12), beginning with the lowest measuring light intensity setting. For each 474
measuring light intensity, a saturation pulse was applied for 720 ms (intensity setting =10, 475
yielding 2700 µmol photons m-2
s-1
), and a resting period of 1 min was used between saturation 476
pulses. 477
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22
We also examined the effects of light scattering on samples illuminated with defined 478
actinic irradiance levels, i.e., light-acclimated samples. Steady-state light curves of rETR versus 479
photon irradiance were measured over a range of actinic incident photon irradiances of PAR 480
(400–700 nm) ranging from 0 to about 1600 µmol photons m-2
s-1
. For each light curve, the 481
sample was dark-acclimated for about 15 min before a light curve was measured using an 482
exposure time of 5 min at each irradiance level. Prior to starting the steady-state light curves, the 483
measuring light intensity was adjusted such that F0 for the different coral mimics yielded 484
comparable values (i.e. F0=0.08). Likewise, measuring light intensity was adjusted such that 485
F0=0.08 for experiments 2 and 3 (Fig. 1). 486
Data analysis 487
The effective photosynthetic quantum yield of PSII was calculated as ФPSII= (Fm’-F)/Fm’ and 488
relative photosynthetic PSII electron transport rates were calculated as rETR = PAR x ФPSII 489
(Baker, 2008). Calculated rETR versus photon irradiance curves were fitted with an exponential 490
function (Webb et al., 1974) to estimate the maximal relative PSII electron transport rates 491
(rETRmax) and the light-use efficiency factor, α. Non-linear curve fitting was performed in Origin 492
(Origin Pro 9.3, USA) using a Levenberg-Marquart least squares fitting algorithm. 493
Optical simulations 494
A probability light distribution model was developed to calculate the depth-dependent generation 495
and escape of Chl fluorescence (Chf-MC). Details of the model and optical simulations can be 496
found in the supplementary information (Supplemental Text S1). 497
498
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23
Supplemental Data 499
500
Supplemental Text S1. Fluorescent Monte Carlo model to simulate the effect of changes in light 501
scattering and pigment density on calculations of the PSII maximum quantum yield. 502
Supplemental Figure S1. Schematic of photon energy flow in PAM-based variable chlorophyll 503
fluorescence measurements. 504
Supplemental Figure S2. Chlorophyll fluorescence Monte Carlo model simulating the 505
penetration of measuring light. 506
Supplemental Figure S3. Chlorophyll fluorescence Monte Carlo model investigating the effect 507
of re-absorption on observed fluorescence. 508
Supplemental Figure S4. Chlorophyll fluorescence Monte Carlo model calculating the 509
penetration depth of the generated fluorescence. 510
Supplemental Figure S5. Chlorophyll fluorescence Monte Carlo model calculating the % of 511
photosynthetic tissue overexposed by ML. 512
Supplemental Figure S6. 2-Layer Monte Carlo Simulation of light absorption by microalgal 513
cells for the skeleton hydrogel showing the effect skeletal backscattering on the tissue absorption 514
factor. 515
Supplemental Table S1. Abbreviations 516
517
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24
Supplemental Text S1. Fluorescent Monte Carlo model to simulate the effect of changes in light 518
scattering and pigment density on calculations of the PSII maximum quantum yield (Fv/Fm). 519
Supplemental Figure S1. Schematic of photon energy flow in PAM-based variable chlorophyll 520
fluorescence measurements. 521
Supplemental Figure S2. Chlorophyll fluorescence Monte Carlo model (chf-MC) simulating the 522
penetration of measuring light MLd (675 nm) in J mm-2
(A), the depth-dependent F0 generation [J 523
mm-2
](B), the depth-dependent escape of generated fluorescence Fesc(700 nm) [dimensionless] 524
(C), and the observed fluorescence Fobs [J mm-2
](D). 525
Supplemental Figure S3. Chlorophyll fluorescence Monte Carlo model (chf-MC) investigating 526
the effect of re-absorption on observed fluorescence. The penetration of measuring light MLd 527
(675 nm) in J mm-2
(A), the depth-dependent F0 generation [J mm-2
] (B), the depth-dependent 528
escape of generated fluorescence (700nm) [dimensionless] (C) and the observed fluorescence 529
(D). The absorption coefficient at 675 nm was µa=0.15 mm-1
and the reduced scattering 530
coefficient was µs’= 1 mm-1
. The absorption coefficient of the re-emitted fluorescence was varied 531
between µa=0.05 mm-1
(red), 0.03 mm-1
(black), 0.01 mm-1
(green) and 0 mm-1
(blue). 532
Supplemental Figure S4. Chlorophyll fluorescence Monte Carlo model (chf-MC) calculating 533
the penetration depth, i.e., the depth over which at least 90% of the generated fluorescence 534
originates from (a), and the saturation depth, i.e., the depth for which all photosynthetic cells are 535
saturated by a saturation pulse of 2800 µmol photons m-2
s-1
, assuming a saturation threshold of 536
1500 µmol photons m-2
s-1
(b). The dependency on the reduced scattering coefficient µs’ and µa is 537
modeled using chf-MC. 538
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25
Supplemental Figure S5. Chlorophyll fluorescence Monte Carlo model (chf-MC) calculating 539
the % of photosynthetic tissue overexposed by ML, for standard setting of the measuring light of 540
ML=3 (A), ML=4 (B) and ML=5 (C). A threshold for overexposure is assumed (0.5 µmol 541
photons m-2
s-1
). 542
Supplemental Figure S6. 2-Layer Monte Carlo Simulation of light absorption by microalgal 543
cells for the skeleton hydrogel showing the effect skeletal backscattering on the tissue absorption 544
factor. 545
Supplemental Table S1. Abbreviations 546
547
548
Acknowledgements 549
This study was supported by a Sapere-Aude Advanced grant from the Independent Research 550
Fund Denmark ǀ Natural Sciences (MK), and by the Carlsberg Foundation via a distinguished 551
postdoctoral scholarship grant (DW), and an instrument grant (MK). We thank Sofie Jakobsen 552
for excellent technical assistance, and Lars Rickelt for manufacturing scalar irradiance 553
microprobes. 554
555
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26
Table 1. Material properties of coral tissue–mimicking hydrogels. The algal species was 556
Rhodomonas salina unless indicated otherwise. 557
Experiment Hydrogel Top layer Mid layer Base layer
Coral
scattering
GFP matrix ASW+ 1% agarose ASW+ 1% agarose ASW+ 1% agarose
SiO2 4% / 5%
algae / 2.5 x 106 cells cm-2 /
thickness 0.75 mm 0.75 mm 2.5 mm
Skeleton matrix / ASW+ 1% agarose ASW+ 1% agarose
SiO2 / / 15%
algae / 2.5 x 106 cells cm-2 /
thickness / 0.75 mm 2.5 mm
Transparent matrix ASW+ 1% agarose ASW+ 1% agarose
SiO2 / / /
algae / 2.5 x 106 cells cm-2 /
thickness / 0.75 mm 2.5 mm
Coral absorption High matrix / ASW+ 1% agarose ASW+ 1% agarose
SiO2 / 1% 5%
algae / 3.5 x 106 cells cm-2 /
thickness / 0.75 mm 2.5 mm
Medium matrix / ASW+ 1% agarose ASW+ 1% agarose
SiO2 / 1% 5%
algae / 1 x 106 cells cm-2 /
thickness / 0.75 mm 2.5 mm
Coral stress Stressed matrix ASW+ 1% agarose ASW+ 1% agarose ASW+ 1% agarose
SiO2 / / 5%
algae 2 x 106 cells cm-2
(N. oculata)
2 x 106 cells cm-2
/
thickness 0.75 mm 0.75 mm 2.5 mm
Stressed and
bleached
matrix ASW+ 1% agarose ASW+ 1% agarose ASW+ 1% agarose
SiO2 / / 5%
algae 0.3 x 106 cells cm-2
(N. oculata)
2 x 106 cells cm-2
/
thickness 0.75 mm 0.75 mm 2.5 mm
Healthy matrix ASW+ 1% agarose ASW+ 1% agarose ASW+ 1% agarose
SiO2 / / 5%
algae 2 x 106 cells cm-2
2 x 106 cells cm-2
/
thickness 0.75 mm 0.75 mm 2.5 mm
558
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27
Figure Legends 559
Figure 1: Coral tissue organisation and artificial tissue design. a-c) Basic organisation of 560
scleractinic corals. a) Small fragment of a faviid coral (scale bar = 1 mm). b) close-up of the 561
cross-section, revealing the white coral skeleton, the brown algal layer on top of the skeleton, 562
and the green fluorescent protein like-pigment granules (GFP) on the coral tissue surface (scale 563 bar = 1mm). c) close-up of GFP granules (scale bar = 200 µm). d-i) Coral tissue mimicking 564
hydrogels. Schematics of 3-layer ‘GFP’ (d), 2-layer ‘skeleton’ (e), and 2-layer ‘transparent’(f) 565
designs. g-i) Respective photographs of thin cross sections of hydrogels. j-m) Hydrogels for 566
investigating the effect of changes in coral absorption. j-k) High microalgal density tissue design 567
(j) and top view photograph (k). l-m) Medium microalgal density hydrogel (l) and top view 568
photograph (m). n-p) Hydrogels for investigating the effect of coral stress. n) ‘Healthy’ coral 569
design with 2 layers of Rhodomonas sp., o) ‘Stressed’ coral design with 1 layer of 570
Nanochloropsis sp. on top of 1 layer of Rhodomonas sp., p) ‘Bleaching’ design with 1 layer of 571
Nanochloropsis sp. of a reduced cell density on top of Rhodomonas salina. 572
Figure 2. Effect of light scattering on variable chlorophyll fluorescence parameters of dark 573 acclimated coral tissue mimicking hydrogels. (a-c) Example images of minimal fluorescence 574
yields (F0) for measuring light intensity = 4, showing GFP (a), skeleton (b) and transparent (c) 575
hydrogels. The white circle shows the area over which F0 was integrated. Effect of measuring 576
light intensity on F0, (d), Fm, maximal fluorescence yield (e), and the maximum PSII quantum 577 yield, Fv/Fm (f). Note that no measurements are shown at ML>4 (=0.8 µmol photons m
-2 s
-1) and 578
ML>8 (= 1.6 µmol photons m-2
s-1
) for skeleton and transparent hydrogels, respectively due to 579
indications of actinic effects in these hydrogels at higher measuring light levels. 580
Figure 3. In vivo light microenvironment in coral tissue mimicking hydrogels with different 581 scattering properties. Photon scalar irradiance of PAR (400-700 nm) was normalised to the 582 incident downwelling irradiance of PAR and plotted against the vertical depth (µm) of the coral 583
mimics. The algal layer is distributed between depth = 0 µm to 750 µm for the transparent (red) 584
and skeleton (blue) mimic, while the algal layer is between 750-1500 µm in the GFP (green) 585
mimic. Four replicate gels were measured at 2 random spots (total n=8 ± SE). 586
Figure 4. Effect of light scattering on the effective quantum yield ФPSII (a-b) and relative 587
electron transport rates (rETR) (c-d) of coral tissue mimicking hydrogels. Measured ФPSII 588
and calculated rETR were plotted as a function of the incident downwelling irradiance (Ed) (a,c) 589
and with the corrected in vivo scalar irradiance (E0) (b,d). Symbols with error bars represent 590
means ± SE (n=5 biological replicates). 591
Figure 5. Effect of coral light absorption on the light microenvironment and variable 592
chlorophyll fluorescence measurements. Photon scalar irradiance (400-700 nm) was 593
normalised to the incident downwelling irradiance (Ed) and plotted against the vertical depth 594
(µm) in the coral mimics. The algal layer is distributed between 0-750 µm depth (a). The 595
maximum quantum yield of PSII, Fv/Fm (b). Relative electron transport rates (rETR) calculated 596
as a function of the incident downwelling irradiance (Ed) (c) and corrected for in vivo scalar 597
irradiance (E0) (d). All measurements were performed in coral hydrogels mimicking high algal 598
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28
density (3.5 x 106 cells cm
-2) and medium algal density (1.0 x 10
6 cells cm
-2). Symbols represent 599
means ± SE (n=4 biological replicates) in panel a-c. The curve fit shown in panel d was the best 600
fit to the experimental data (R2= 0.98 and 0.80) yielding values of ETRmax= 80 and 59, and 601
α=0.22 and 0.11 for the high and medium algal density coral hydrogels, respectively. 602
Figure 6. Combined effects of bio-optical properties and simulated coral bleaching on 603
measured relative electron transport rates (rETR). Hydrogels mimicking healthy tissue 604
contained two dense layers of R. salina (4 x 106 cells cm
-2), hydrogels mimicking stressed tissue 605
contained one dense layer of N. oculata (2 x 106 cells cm
-2) and one dense layer of R. salina (2 x 606
106 cells cm
-2), and hydrogels mimicking bleached tissue contained one layer of N. oculuata at 607
low density (0.3 x 106 cells cm
-2) and one dense layer of R. salina. Data are means ± SE (n=2-3 608
hydrogel replicates). 609
Figure 7. Propagation of PAM-based measuring light in biological tissues with different 610
scattering coefficients. a-b) Excitation (blue) and chlorophyll fluorescence (red) for transparent 611
hydrogel (a) and skeleton hydrogel (b). The optical properties of the light absorbing top layer 612
(layer 1) are constant (i.e. identical algal density and bio physical properties of an algal cell) for 613
both gels, but layer 2 is either transparent or light scattering. For the transparent hydrogel, 614
measuring light absorption by an algal cell (s) is a function of the primary incident beam (solid 615
blue line), while indirect light (dotted blue lines) is lost through the transparent layer. For the 616
skeleton hydrogel, indirect light is redirected via backscattering by layer 2. Such scattering 617
enhances the chance of measuring light absorption and thus leads to greater fluorescence 618
emission (bold red arrows). Fluorescence emission is an isotropic process but the propagation of 619
fluorescent light is affected by tissue optical properties. For the transparent hydrogel, only 620
primary upwelling fluorescence (Fu1) contributes to the detected fluorescence signal, while for 621
the skeleton hydrogel the downwelling fluorescence (Fd) is redirected and adds to the upwelling 622
fluorescence (Fu2). c) A steep light gradient (green line) leads to an underrepresentation of 623
fluorescence detection from lower cell layers compared to a homogenous light environment 624
(black line), given that the operational volume (dotted lines) from which fluorescence is 625
collected is a function of the theoretical instrument detection limit (Elimit) which is modulated by 626
the in vivo photon scalar irradiance. 627
628
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1
Figure 1: Coral tissue organisation and artificial tissue design. a-c) Basic organisation of
scleractinic corals. a) Small fragment of a faviid coral (scale bar = 1 mm). b) close-up of the
cross-section, revealing the white coral skeleton, the brown algal layer on top of the skeleton,
and the green fluorescent protein like-pigment granules (GFP) on the coral tissue surface (scale bar = 1mm). c) close-up of GFP granules (scale bar = 200 µm). d-i) Coral tissue mimicking
hydrogels. Schematics of 3-layer ‘GFP’ (d), 2-layer ‘skeleton’ (e), and 2-layer ‘transparent’(f)
designs. g-i) Respective photographs of thin cross sections of hydrogels. j-m) Hydrogels for
investigating the effect of changes in coral absorption. j-k) High microalgal density tissue design
(j) and top view photograph (k). l-m) Medium microalgal density hydrogel (l) and top view
photograph (m). n-p) Hydrogels for investigating the effect of coral stress. n) ‘Healthy’ coral
design with 2 layers of Rhodomonas sp., o) ‘Stressed’ coral design with 1 layer of
Nanochloropsis sp. on top of 1 layer of Rhodomonas sp., p) ‘Bleaching’ design with 1 layer of
Nanochloropsis sp. of a reduced cell density on top of Rhodomonas salina.
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1
Figure 2. Effect of light scattering on variable chlorophyll fluorescence parameters of dark
acclimated coral tissue mimicking hydrogels. (a-c) Example images of minimal fluorescence
yields (F0) for measuring light intensity = 4, showing GFP (a), skeleton (b) and transparent (c)
hydrogels. The white circle shows the area over which F0 was integrated. Effect of measuring
light intensity on F0, (d), Fm, maximal fluorescence yield (e), and the maximum PSII quantum yield, Fv/Fm (f). Note that no measurements are shown at ML>4 (=0.8 µmol photons m
-2 s
-1) and
ML>8 (= 1.6 µmol photons m-2
s-1
) for skeleton and transparent hydrogels, respectively due to
indications of actinic effects in these hydrogels at higher measuring light levels.
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1
Figure 3. In vivo light microenvironment in coral tissue mimicking hydrogels with different
scattering properties. Photon scalar irradiance of PAR (400-700 nm) was normalised to the incident downwelling irradiance of PAR and plotted against the vertical depth (µm) of the coral
mimics. The algal layer is distributed between depth = 0 µm to 750 µm for the transparent (red)
and skeleton (blue) mimic, while the algal layer is between 750-1500 µm in the GFP (green)
mimic. Four replicate gels were measured at 2 random spots (total n=8 ± SE).
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1
Figure 4. Effect of light scattering on the effective quantum yield ФPSII (a-b) and relative electron transport rates (rETR) (c-d) of coral tissue mimicking hydrogels. Measured ФPSII and calculated rETR were plotted as a function of the incident downwelling irradiance (Ed) (a,c) and with the corrected in vivo scalar irradiance (E0) (b,d). Symbols with error bars represent means ± SE (n=5 biological replicates).
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1
Figure 5. Effect of coral light absorption on the light microenvironment and variable
chlorophyll fluorescence measurements. Photon scalar irradiance (400-700 nm) was
normalised to the incident downwelling irradiance (Ed) and plotted against the vertical depth
(µm) in the coral mimics. The algal layer is distributed between 0-750 µm depth (a). The
maximum quantum yield of PSII, Fv/Fm (b). Relative electron transport rates (rETR) calculated
as a function of the incident downwelling irradiance (Ed) (c) and corrected for in vivo scalar
irradiance (E0) (d). All measurements were performed in coral hydrogels mimicking high algal
density (3.5 x 106 cells cm
-2) and medium algal density (1.0 x 10
6 cells cm
-2). Symbols represent
means ± SE (n=4 biological replicates) in panel a-c. The curve fit shown in panel d was the best
fit to the experimental data (R2= 0.98 and 0.80) yielding values of ETRmax= 80 and 59, and
α=0.22 and 0.11 for the high and medium algal density coral hydrogels, respectively.
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1
Figure 6. Combined effects of bio-optical properties and simulated coral bleaching on
measured relative electron transport rates (rETR). Hydrogels mimicking healthy tissue
contained two dense layers of R. salina (4 x 106 cells cm
-2), hydrogels mimicking stressed tissue
contained one dense layer of N. oculata (2 x 106 cells cm
-2) and one dense layer of R. salina (2 x
106 cells cm
-2), and hydrogels mimicking bleached tissue contained one layer of N. oculuata at
low density (0.3 x 106 cells cm
-2) and one dense layer of R. salina. Data are means ± SE (n=2-3
hydrogel replicates).
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2
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1
Figure 7. Propagation of PAM-based measuring light in biological tissues with different
scattering coefficients. a-b) Excitation (blue) and chlorophyll fluorescence (red) for transparent
hydrogel (a) and skeleton hydrogel (b). The optical properties of the light absorbing top layer
(layer 1) are constant (i.e. identical algal density and bio physical properties of an algal cell) for
both gels, but layer 2 is either transparent or light scattering. For the transparent hydrogel,
measuring light absorption by an algal cell (s) is a function of the primary incident beam (solid
blue line), while indirect light (dotted blue lines) is lost through the transparent layer. For the
skeleton hydrogel, indirect light is redirected via backscattering by layer 2. Such scattering
enhances the chance of measuring light absorption and thus leads to greater fluorescence
emission (bold red arrows). Fluorescence emission is an isotropic process but the propagation of
fluorescent light is affected by tissue optical properties. For the transparent hydrogel, only
primary upwelling fluorescence (Fu1) contributes to the detected fluorescence signal, while for
the skeleton hydrogel the downwelling fluorescence (Fd) is redirected and adds to the upwelling
fluorescence (Fu2). c) A steep light gradient (green line) leads to an underrepresentation of
fluorescence detection from lower cell layers compared to a homogenous light environment
(black line), given that the operational volume (dotted lines) from which fluorescence is
collected is a function of the theoretical instrument detection limit (Elimit) which is modulated by
the in vivo photon scalar irradiance.
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