Defining the Far-Red Limit of Photosystem II in Spinach C W · Department of Photochemistry and...
Transcript of Defining the Far-Red Limit of Photosystem II in Spinach C W · Department of Photochemistry and...
Defining the Far-Red Limit of Photosystem II in Spinach C W
Anders Thapper, Fikret Mamedov, Fredrik Mokvist, Leif Hammarstrom, and Stenbjorn Styring1
Department of Photochemistry and Molecular Science, Angstrom Laboratory, Uppsala University, SE-751 20 Uppsala, Sweden
The far-red limit of photosystem II (PSII) photochemistry was studied in PSII-enriched membranes and PSII core
preparations from spinach (Spinacia oleracea) after application of laser flashes between 730 and 820 nm. Light up to 800
nm was found to drive PSII activity in both acceptor side reduction and oxidation of the water-oxidizing CaMn4 cluster. Far-
red illumination induced enhancement of, and slowed down decay kinetics of, variable fluorescence. Both effects reflect
reduction of the acceptor side of PSII. The effects on the donor side of PSII were monitored using electron paramagnetic
resonance spectroscopy. Signals from the S2-, S3-, and S0-states could be detected after one, two, and three far-red
flashes, respectively, indicating that PSII underwent conventional S-state transitions. Full PSII turnover was demonstrated
by far-red flash-induced oxygen release, with oxygen appearing on the third flash. In addition, both the pheophytin anion
and the Tyr Z radical were formed by far-red flashes. The efficiency of this far-red photochemistry in PSII decreases with
increasing wavelength. The upper limit for detectable photochemistry in PSII on a single flash was determined to be 780 nm.
In photoaccumulation experiments, photochemistry was detectable up to 800 nm. Implications for the energetics and
energy levels of the charge separated states in PSII are discussed in light of the presented results.
INTRODUCTION
The action spectrum of oxygenic photosynthesis has been
extensively studied, and the overall quantum yield sharply de-
creases at wavelengths above 680 nm (Emerson and Lewis,
1943; Emerson et al., 1957; Blankenship, 2002). This red drop is
considered to be due to an unbalance of excitation between
photosystem I (PSI) and photosystem II (PSII). PSII is less
efficient in using long wavelength light than is PSI. Therefore,
there is a limited supply of electrons available for PSI above 680
nm, decreasing the photosynthetic yield in the far-red region.
The antenna system of PSI contains a small amount (3 to 10%)
of so-called red or low energy chlorophylls. These have their
absorption maxima in the red region (the Qy band) shifted to
beyond 700 nm (Gobets and van Grondelle, 2001; Karapetyan
et al., 2006). Apart from capturing far-red photons, they have
been ascribed a role in photoprotection (Gobets and van
Grondelle, 2001). The red chlorophylls originate from intermo-
lecular interactions between chlorophyll a molecules forming
strongly excitonically coupled dimers (or larger aggregates). This
intermolecular interaction does not require that the chlorophylls
are in contact with each other, only that they are electronically
interacting. The localization of the red chlorophylls in PSI is not
unambiguously determined (Jordan et al., 2001; Karapetyan
et al., 2006). There is no known corresponding system with such
far-red absorbing chlorophylls in PSII, and the available x-ray
crystal structures have not revealed any strongly coupled chlo-
rophylls in the PSII antenna (Ferreira et al., 2004; Loll et al., 2005).
Instead, the common view is that the primary donor chlorophylls,
referred to as P680, define the red-edge limit of excitation and,
therefore, the practical energy limitation for driving water oxida-
tion and plastoquinone reduction.
Some organisms can use light of longer wavelengths for
photosynthesis. For example, >95% of the antenna pigments
of PSII in the cyanobacterium Acaryochloris marina are chloro-
phyll d molecules that absorb light further to the red than
chlorophyll a (Miyashita et al., 1996, 1997, 2003). The nature of
the chlorophylls in the PSII reaction center of A. marina is still
debated. This also holds for the absorption associated with the
primary donor that has been placed at 713 nm (Tomo et al., 2007)
or at 725 nm (Itoh et al., 2007).
Surprisingly, oxygen evolution from PSII has also been re-
ported above 700 nm for green algae (GreenbaumandMauzerall,
1991) and higher plants (Pettai et al., 2005a, 2005b), both of
which have the more common chlorophyll a/b containing an-
tenna. For the green algae Chlorella vulgaris, 723-nm light
promoted the same maximum oxygen evolution (within 10%)
as shorter wavelengths (Greenbaum and Mauzerall, 1991). Oxy-
gen evolution at 723 nm followed the same light saturation
behavior as at shorter wavelengths, but a much higher photon
flux was needed to achieve maximal activity, indicating that the
effective optical cross section for the antenna wasmuch smaller.
The physiological significance is also clear, and oxygen evolution
and variable chlorophyll a fluorescence have been observed in
sunflower (Helianthus annuus) and bean (Phaseolus vulgaris) leaves
using wavelengths up to 780 nm (Pettai et al., 2005a, 2005b).
Charge separation can also be induced in PSII core complexes at
cryogenic temperatures up to 730 nm (Hughes et al., 2006a).
Here, we used spinach (Spinacia oleracea) PSII preparations,
with different degrees of purification, to focus on far-red light–
induced PSII activity in vitro. Well-defined laser flashes between
1Address correspondence to [email protected] author responsible for distribution of materials integral to thefindings presented in this article in accordance with the policy describedin the Instructions for Authors (www.plantcell.org) is: Stenbjorn Styring([email protected]).CSome figures in this article are displayed in color online but in blackand white in the print edition.WOnline version contains Web-only data.www.plantcell.org/cgi/doi/10.1105/tpc.108.064154
The Plant Cell, Vol. 21: 2391–2401, August 2009, www.plantcell.org ã 2009 American Society of Plant Biologists
730 and 820 nm were used to study PSII photochemistry and
electron transfer. Variable chlorophyll a fluorescence and elec-
tron paramagnetic resonance (EPR) spectroscopy were used to
follow reactions on both the acceptor and donor side of PSII. We
also detected a flash-dependent oxygen evolution pattern using
far-red laser flashes. Implications for the energetics in PSII to
accommodate the presented results are discussed.
RESULTS
Reduction of the Acceptor Side: Effect of Far-Red
Preillumination on Variable Fluorescence
Appearance of variable fluorescence (FV) is a consequence of the
charge separation in PSII that results in reduction of QA- (Renger
et al., 1995). Analysis of the flash-induced FV decay kinetics
provides information about the activity of the PSII acceptor side
(Joliot et al., 1971; Crofts and Wraight, 1983; Robinson and
Crofts, 1983; Renger et al., 1995). In our samples, the decay
kinetics could be resolved in three phases (Figure 1A; t1 = 1.4 ms
[38%], t2 = 26 ms [38%], and t3 = 4.8 s [24%], with relative
amplitudes within brackets). These phases are normally as-
signed to electron transfer from QA- to QB (QB
-), electron transfer
fromQA- to QB in a PSII center whereQB has to bind to theQB site
prior to electron transfer, and recombination of QA- with the
donor side, respectively. The two fast phases, t1 and t2, involved
;75% of the FV.
The application of a series of visible light flashes to PSII
membranes builds up an increased FV, compared with the effect
of only one flash (Mamedov et al., 2000; Pospısil and Dau, 2000).
This flash-dependent enhancement of FV is not observed in
intact thylakoidmembranes and has been attributed to reduction
of the limited plastoquinone (PQ) pool in the PSII membranes
leading to inefficient forward electron transfer from QA-.
We used far-red monochromatic laser flashes (730 to 820 nm)
to determine the upper limit of this flash-dependent build-up of
FV. In the experiment, preillumination with laser flashes of varying
wavelengths was used to induce the effect. This was thereafter
observed as FV induction and decay in a standard fluorescence
setup (see Methods).
Figure 1A shows the FV decay kinetics recorded in a control
(dark adapted) sample and a sample preilluminated with 100
laser flashes at 750 nm. The FV obtained after the preillumination
was about 2 times higher than that of the control sample andwas
much closer to the maximal FV level that can be obtained by
reduction with 10mMdithionite. The initial fluorescence level (F0)
also increased by about 2 times after the preillumination with 100
flashes at 750 nm.
The wavelength dependence of this preillumination-induced
enhancement of FV and F0 was studied in the 650- to 820-nm
region (Figure 1B). In samples preilluminated with 10 flashes
(25 mJ) between 650 and 740 nm, the FV was enhanced to near
the maximum level, while the effect decreased between 740 and
810 nm. Importantly, the enhanced FV was observed above
760 nm if the number of preillumination flashes was increased
(Figure 1B). Above 810 nm, no FV enhancement could be
observed. The same wavelength dependence also holds for
the increase of F0 by the preillumination flashes (Figure 1B). As
will be shown below, far-red flashes of 25 mJ (the maximum
power available with our laser for the whole wavelength interval)
are saturating for wavelengths up to 750 nm, but not for the
wavelengths above.
Preillumination with the far-red laser flashes also changed the
decay kinetics of FV (Figure 1A) substantially. When FV was
induced to its maximal level, three decay phases could still be
resolved (t1 = 1.0 ms [27%], t2 = 200 ms [17%], and t3 = 2.5 s
[56%]). The relative amplitude of the first two phases had
decreased from ;75% in the dark control to <50% of FV in the
preilluminated sample. In addition, t2 had increased by almost
one order of magnitude. The slow phase, which reflects recom-
bination between QA- and the water oxidizing complex (WOC),
was dominating the fluorescence decay (56%).
If the sample was incubated in the dark for 20min at 208C after
the preillumination, the effect of the far-red flashes completely
disappeared, and FV, F0, and Fv decay kinetics returned to
control values.
Although these complex effects on FV and F0 induced by far-
red preillumination of PSII have not been described earlier, they
have direct analogies to the effects seen by preillumination with
visible light on similar PSII preparations (Mamedov et al., 2000;
Pospısil and Dau, 2000). This allows assignment of the effects,
and it is highly likely that both the considerable increase of the FVand F0 and the slowed decay kinetics of QA
- reflect that the
limited PQ pool has been reduced by far-red laser flashes. Ten
laser flashes atwavelengths up to 740 nmwere enough to reduce
the PQ pool. The PQ pool was fully reduced by 900 flashes at
wavelengths up to 775 nm and partly reduced with 900 flashes
up to 800 nm. Thus, we conclude that the application of far-red
laser flashes up to 800 nm induces sufficient electron transport to
reduce both the acceptor side of PSII and the PQ pool.
This conclusion was further verified by the addition of ferricy-
anide prior to the far-red laser flashing. This completely abolished
Figure 1. Changes in FV after Preillumination of PSII Membranes with
Laser Flashes.
(A) Flash-induced fluorescence decay traces before (closed circles,
dark) and after (open circles, 750 nm) the application of 100 flashes at
750 nm. The arrow indicates the time of the actinic flash.
(B) F0 (closed squares) and FV (open squares) levels in samples that were
exposed to 10 (left) or 900 (right) laser flashes at the indicated wave-
lengths. The F0 (dotted line) and FV (broken line) levels before the
application of flashes are indicated.
2392 The Plant Cell
the enhancement of FV and the slowing of the FV decay kinetics
(see Supplemental Figure 1 online). We interpret this to reflect
ferricyanide functioning as an effective oxidant of QA-, thereby
preventing reduction of the acceptor side and the PQ pool. This
maintains FV on a low level and leaves the QA- reoxidation kinetics
unaffected.
Direct Detection of Donor Side Reactions: Oxidation of the
CaMn4 Cluster
The observation of far-red-induced photochemistry on the ac-
ceptor side of PSII prompted us to look for electron transfer at
the donor side as well. Many intermediates in the water oxida-
tion S-cycle of the CaMn4 cluster can be trapped by freezing,
followed by EPR at cryogenic temperatures. The well-studied
multiline EPR signal from the S2-state is detected at liquid helium
temperatures (Dismukes and Siderer, 1981; Miller and Brudvig,
1991). This also holds for the so-called split EPR signals origi-
nating from the S1-, S3-, and S0-states, which are inducible by
visible or IR (S3 only) illumination at 5 to 10K of PSII samples
poised in the respective S-state (Nugent et al., 2002; Zhang
and Styring, 2003; Zhang et al., 2004; Petrouleas et al., 2005;
Havelius et al., 2006; Su et al., 2007). We studied the S-cycle
advancement in samples set in the S1-state and then exposed to
0 (dark), 1, 2, or 3 flashes at 750 nm at 208C. The different
S-states were then recognized by the observation of their re-
spective EPR signals. We also exposed a sample to 10 flashes at
750 nm to scramble (if possible) the S-states.
Figure 2A shows the S2-state multiline EPR signal in samples
exposed to 1, 2, 3, or 10 flashes. One flash at 750 nm resulted in a
significant multiline EPR signal (Figure 2A, 1 fl) corresponding to
45% 6 5% of the maximally inducible signal (using one saturat-
ing 800-mJ laser flash at 532 nm), indicating that the flash at 750
nm induced the S2-state in;45%6 5% of the PSII centers. The
rest of the centers remained in theS1-state, whichwas confirmed
by the observation of a large split EPR signal from the S1-state
(Figure 2B, spectrum 1). The split S1 EPR signal corresponded
well to the 55% 6 5% of centers that had remained in the
S1-state when compared with the split S1 EPR signal from a
sample poised in the S1-state (Figure 2B, 0 fl). No sign of the split
EPR signal from the S3-state was observed in this sample (Figure
2C, 1 fl). In a sample exposed to two flashes, the Split S1 (Figure
2B, 2 fl), the S2-state multiline (Figure 2A, 2 fl), and the split S3
EPR signals (Figure 2C, 2 fl) all were observed. This reflects
turnover all the way to the S3-state.
In addition to the split EPR signal from the S3-state, there are a
few other EPR signals connected to the S2- and S3-states of the
CaMn4 cluster that are reported to be induced by excitation or
spin transitions by far-red or IR wavelengths. However, these
effects were reported only at cryogenic temperatures (<150K) at
conditions in which no charge separation can occur (Boussac
et al., 2005). Our observed effect does not involve spin transitions
in the CaMn4 cluster at low temperatures. This is further sub-
stantiated bymeasurements of far-red-induced electron transfer
in PSII preparations lacking the CaMn4 cluster (see below).
In the sample exposed to three flashes, split EPR signals from
all of the S1-, S3-, and S0-states states (Figures 2B and 2C, 3 fl)
were observed together with the multiline EPR signal from the
S2-state (Figure 2A, 3 fl), clearly indicating that the full S-cycle
could be completed by only a few flashes at 750 nm. In the
sample that was given 10 flashes at 750 nm, all of the EPR signals
had considerable amplitudes (Figure 2, 10 fl spectra). Clearly, the
10 flashes at 750 nm led to almost complete scrambling of the
S-states in the WOC. The miss factor on these far-red flashes is
Figure 2. EPR Signals from PSII Membranes after Far-Red Turnover Flashes, Representing Intermediates in the S-State Cycle in the WOC.
(A) Light minus dark difference spectra of the multiline EPR signal from the S2-state in samples exposed to 1, 2, 3, or 10 flashes (fl) at 750 nm. The
asterisks indicate the peaks used for signal quantification.
(B) EPR spectra from the S1- (Y) and the S0-states (*). The samples were exposed to 0, 1, 2, 3, or 10 flashes at 750 nm. Contributions from the QA--Fe2+
signal are indicated with bars.
(C) The split EPR signal from the S3-state (the asterisk indicates the trough of the signal) in samples exposed to 0, 1, 2, 3, or 10 flashes at 750 nm.
The EPR spectra in (B) and (C) were obtained as described in Methods. EPR conditions were as follows: temperature, 7K (A) and 5K ([B] and [C]);
microwave power, 10 mW (A) and 25 mW ([B] and [C]); modulation amplitude, 20 G (A) and 10 G ([B] and [C]); microwave frequency, 9.28 GHz.
The Far-Red Limit of Photosystem II 2393
high. This reflects the fact that the PSII sample absorbs ineffi-
ciently at 750 nm and that our laser power is too low to allow light
saturation in the concentrated EPR samples. Previously, we have
reported our initial observations of WOC turnover using exten-
sive 750-nm laser flashing. In samples exposed to >300 laser
flashes, we detected centers in the S1-, S2-, and S0-states by
EPR spectroscopy (Thapper et al., 2008). Thus, the early results
involved studies of only scrambled S-states, not allowing quan-
titative analysis of single turnover photochemistry.
Single flashes between 730 and 790 nm were applied to PSII,
and the multiline EPR signal from the S2-state was measured to
investigate further the far-red edge of the action spectrum of PSII
(Figure 3A). The S1 to S2 turnover in a single flash was high at
730 nm (85% 6 5% compared with the multiline signal induced
by a saturating flash at 532 nm) but decreased as the wavelength
was increased. At 790 nm, the amount of themultiline EPR signal
from the S2-state was hardly detectable after one flash (see
Supplemental Figure 2 online). In a separate sample given 100
flashes at 790 nm, both the S2-state multiline (Figure 3A, 790 nm
100 fl) and the split S3 EPR signals (Figure 3A, inset) were induced
to significant extents. By contrast, in a sample given 100 flashes
at 810 nm, only the split EPR signal from the S1-state, and no
S2-state multiline EPR signal (Figure 3A, 810 nm 100 fl), could be
detected, indicating that the CaMn4 cluster did not turn over at
this wavelength. This puts the far-red limit for photochemical
oxidation of the CaMn4 cluster using multiple flashes at around
800 nm. This is very similar to the limit for the photochemical
reduction of the acceptor side of PSII obtained from the fluores-
cence experiments (Figure 1B).
Minimal PSII core preparations from plants with fully active
oxygen evolution contain the D1/D2 heterodimer, the chlorophyll
binding proteins CP43 and CP47, cyt b559, the psbO protein, and
a set of small subunits (Smith et al., 2002). The PSII core
preparation does not contain LHCII or the minor antenna com-
ponents CP24, CP26, or CP29. To elucidate further the location
of the far-red absorbing species in PSII, we exposed a PSII core
sample to 1 and 100 flashes at 750 nm. In both cases, we
observed the induction of the multiline EPR signal from the
S2-state (Figure 3B), which demonstrated that far-red photo-
chemistry occurs also in PSII core preparations. The multiline
EPR signal from the S2-state after one flash corresponded to 10
to 15% of the maximum inducible signal (Figure 3B, top spec-
trum). One hundred flashes gave ;30% of the multiline EPR
signal from the S2-state (Figure 3B, bottom spectrum). Seem-
ingly, the turnover capability is considerably lower (no acceptor
was used in this experiment) than the almost 50% turnover that
was observed after a single 750-nm flash in the PSII membranes.
However, in the context of this study, the observation of any
S2-state multiline signal at all is important because it shows that
light at 750 nmcan lead to photochemical oxidation of theCaMn4cluster in a PSII core preparation lacking a large part of the
chlorophyll antenna.
Direct Detection of Donor Side Reactions: Tyr Z Oxidation
PSII contains two redox active Tyr residues, YZ and YD. The light-
induced formation and subsequent decay of the radical from YZ,
YZd
, can be studied by EPR spectroscopy in PSII membranes in
Figure 3. The Multiline EPR Signal from the S2-State after Application of
Far-Red Flashes of Different Wavelengths.
(A) The multiline EPR signal from the S2-state in PSII membrane samples
exposed to one flash (25 mJ) at 730, 750, and 770 nm and in samples
exposed to 100 flashes at 790 and 810 nm. The vertical lines indicate the
position of five peaks in the multiline EPR signal, and the asterisks
indicate the three peaks used for signal quantification. The amounts of
PSII centers in the S2-state after a single flash at 730, 750, or 770 nm
were 87% 6 5%, 45% 6 5%, and 14% 6 10%, respectively (the S2-
state multiline EPR signal induced by a saturating flash at 532 nm is taken
as 100%). The inset shows the split EPR signal from the S3-state
(obtained as in Figure 2C) from the sample exposed to 100 flashes at
790 nm.
(B) The multiline EPR signal from the S2-state in PSII core samples
exposed to one flash (25 mJ) or 100 flashes at 750 nm. EPR conditions
were as follows: temperature, 7K, (inset 5K); microwave power, 10 mW
(inset 25 mW); modulation amplitude, 20 G, (inset 10 G); microwave
frequency, 9.28 GHz.
2394 The Plant Cell
which theCaMn4 cluster has been removed by Tris washing. This
treatment significantly (100-fold) slows down YZd
reduction and
allows its detection by EPR spectroscopy at room temperature
(Babcock et al., 1976, 1989; Roffey et al., 1994). We used far-red
laser flashes to induce YZ oxidation in Tris-washed samples
between 730 and 790 nm (Figure 4A). A 730-nm flash induced a
YZd
radical EPR signal corresponding to 55% 6 3% of the YZd
EPR signal induced by a 532-nm flash (70 mJ). The amount of
radical induced decreased with increasing wavelength and,
at 780 nm, the signal was at the detection limit, even after
averaging 250 traces (Figure 4A, inset, cyan trace). Both the
shape of the YZd
signal and the decay kinetics of the signal in the
dark were identical to a YZd
signal induced by a 532-nm laser
flash (Figure 4A).
Thus, the application of far-red light resulted in YZd
radical
induction in Tris-washed PSII membranes in which the CaMn4cluster was destroyed and removed. This rules out the possibility
of Mn excitation and Mn-driven reactions as an explanation for
the far-red photoactivity.
Direct Detection of Acceptor Side Reactions: FV Induced by
Single Far-Red Laser Flashes
It is also possible to induce directly QA reduction using far-red
laser flashes and measure the resulting FV. The power depen-
dence of FV induction by a single flash, in the far-red region
(Figure 4B) and at 532 nm (see Supplemental Figure 3 online),
was measured using a double modulation fluorometer. The laser
flash was used as the actinic flash to induce PSII photochem-
istry, and the fluorometer’s internal LEDs were used as measur-
ing flashes. The measurements were done in the presence of
DCMU. For all wavelengths up to 760 nm, the power depen-
dence is linear at the lower laser powers and saturates at the
higher powers; ;20 times stronger flashes must be used to
reach saturation at 730 nm compared with 532 nm. Above 760
nm, the level of FV induction is very low even when the strongest
available laser flash is used and saturation cannot be reached
with our laser system (Figure 4B, 770 nm, orange, and 780 nm,
cyan). The limit at which the effect of a single flash could be
observed was determined to be 780 nm. Importantly, the FV level
at saturation decreases strongly with increasing wavelength (see
Discussion).
Reduction of the Acceptor Side: Photoaccumulation of the
Pheophytin Anion
Addition of dithionite in millimolar concentrations to PSII mem-
branes efficiently reducesQA. This treatmentmakes it possible to
accumulate a pheophytin anion (Phe-) under intense illumination
at room temperature because forward electron transfer to the
Figure 4. Characterization of Far-Red-Induced Redox Activity in PSII.
(A) Kinetic EPRmeasurements of the YZ
d
radical induced by far-red flashes in Tris-washed PSII membranes. The traces were induced by laser flashes at
532 nm (black), 730 nm (red), 740 nm (green), 750 nm (blue), 760 nm (pink), 770 nm (orange), 780 nm (cyan), and 790 nm (grey). The inset shows an
expanded view of YZ
d
induction at higher wavelengths (760 to 790 nm). The traces are normalized for the laser flash power and number of
accumulations. Details of the experiment are given in Methods. EPR conditions were as follows: temperature, 293K; microwave power, 20 mW;
modulation amplitude, 10 G; time constant, 2.56 ms; microwave frequency, 9.76 GHz.
(B) The fraction of FV induced after a single flash in the presence of DCMU as a function of the laser flash power at 730 nm (red), 740 nm (green), 750 nm
(blue), 760 nm (pink), 770 nm (orange), or 780 nm (cyan). The maximum FV (100%) was obtained by a 639-nm flash (LEDs, 50 ms). The full lines are a fit of
the expression FV = FV(sat) (1� e-N) to the experimental data. FV(sat) is the saturating FV signal, andN = fabs nhy/nPSII, where fabs is the fraction of photons
absorbed, nhy is the number of photons in a flash, and nPSII is the number of PSII reaction centers (seeMethods). The dashed lines are straight lines given
as an estimation of the FV induction at 770 and 780 nm.
(C) Photoaccumulation of Phe- radical in dithionite-reduced PSII membrane samples detected with EPR after 650 flashes at 532 nm (black), 4000
flashes at 730 nm (red), 4000 flashes at 750 nm (blue), and 10000 flashes at 770 nm (orange). The inset shows the fraction of the induced Phe- radical (as
a percentage of PSII centers) at 532 nm (black circles), 730 nm (red triangles), 750 nm (blue squares), and 770 nm (orange diamond). EPR conditions
were as follows: temperature, 15K; microwave power, 1.3 mW; modulation amplitude, 3.5 G; microwave frequency, 9.28 GHz.
The Far-Red Limit of Photosystem II 2395
now doubly reduced QA is not possible (Klimov et al., 1980;
Rutherford and Zimmermann, 1984; Styring et al., 1990). We
investigated the formation of Phe- at room temperature using far-
red flashes. After application of laser flashes, the samples were
frozen rapidly inN2(l), andEPR spectra from thePhe- radical were
recorded. As shown in Figure 4C, we were able to accumulate
Phe- under these conditions. It should be noted that the exten-
sive flashing resulted in an initial increase and subsequent
decrease of the amount of Phe- radical (Figure 4C, inset). This
decrease of Phe- is due to photoinhibition of PSII, which takes
place rapidly at reduced conditions at room temperature. The
amount of the Phe- that could be photoaccumulated dropped
with increasing wavelength, and at 780 nm no Phe- could be
observed.
The three measurements of electron transfer components,
reflecting stable charge separation, themultiline EPR signal from
the S2-state (Figure 5, black), the YZd
radical (Figure 5, red), and
the FV induction (Figure 5, green), all gave comparable wave-
length dependence curves even though the measurement
method and the state of the samples varied greatly. Thus, the
final state after light absorption and primary charge separation is
the same, independent of the wavelength. These wavelengths
dependences are compared with the P680* fluorescence exci-
tation spectrum at 684 nm after excitation between 725 and
780 nm (Figure 5, full line). This fluorescence intensity decreases
more quickly with increasing excitation wavelength than do all of
the other measurements. This difference is interesting and sug-
gests that excitation of P680 is not sufficient to explain the
wavelength dependence of the far-red photochemistry.
Flash-Induced Oxygen Evolution
Given that we observe photochemical electron transfer at both
the donor and the acceptor sides of PSII with far-red light, would
it also be possible to observe flash dependent oxygen evolution?
The bottom traces in Figure 6 show the results in thylakoid
membranes. Green flashes (532 nm; Figure 6B, bottom) induced
the known period four oscillation pattern with the oxygen
appearing on the third flash. Far-red flashes at 750 nm (Figure
6A, bottom) also yielded the first oxygen release on the third
flash. However, the period four oscillation cannot be observed,
and the oxygen yield instead reaches a steady state level with
approximately the same amount of oxygen being formed at each
flash. This lack of oscillation could be simulated by assuming a
miss factor of ;50%, similar to what we observed for the
formation of themultiline EPR signal from the S2-state and the FVinduction.
Similar results were obtained for the PSII membranes (Figure
6, top traces). No oxygen is formed on the first two flashes, and
oxygen formation occurs on the third flash, indicating that the
S-state chemistry works as normal. At 750 nm (Figure 6A, top),
the oscillation is less pronounced than at 532 nm (Figure 6B, top)
and is dampened faster due to low light absorption and to the
limited PQ pool in the PSII membrane preparations. The impor-
tant fact, however, is that in both PSII membranes and thylakoid
membranes, we observe the first oxygen formation at the third
flash when light at 750 nm is used.
DISCUSSION
This study has shown that far-red light up to 800 nm is able to
drive PSII electron transfer. We observed (1) formation of Phe-
and QA-, and multiple electron transfer to PQ on the acceptor
side; (2) formation of the YZd
radical and complete S-state
turnover in the CaMn4 cluster on the donor side that lead to (3)
a flash-induced oxygen evolution pattern. Our study has thereby
confirmed an earlier prediction (Trissl, 2006a) that far-red pho-
tosynthesis and photochemistry should be possible to observe in
isolated chloroplasts or thylakoid membranes. We were able to
prove this experimentally and have extended the observations to
PSII-enrichedmembranes and purified core preparations of PSII.
Thus, except for the low yield that is mainly due to the low light
absorption, PSII functions at wavelengths as high as 800 nm. The
OD in this region is low (OD ;0.01 at 730 nm at the concentra-
tions used for our fluorescence measurements) when measured
in an integrating sphere and decreases with increasing wave-
length (see Supplemental Figure 4 online).
The origin of the earlier observed far-red photosynthesis in vivo
has been discussed in terms of three different mechanisms. The
first proposal, that far-red forms of chlorophylls could also exist
in the PSII antenna, was discussed in the original publication
(Pettai et al., 2005a). A second mechanism, in which far-red light
Figure 5. Correlation between Wavelength Dependence of Different
Far-Red-Induced Signals in PSII.
Wavelength dependence of the amplitude of the multiline EPR signal
from the S2-state (black circles) from Figure 3A, the amplitude of the EPR
signal from YZd
(red triangles) from Figure 4A, and the fraction of light
absorbed (fabs) in the FV induction experiment (green squares) from
Figure 4B. The values at 770 and 780 nm are estimations using the fabsvalue at 760 nm and the difference in FV induction for these three
wavelengths. The solid line shows the excitation spectrum of PSII
membranes at 684 nm after excitation at far-red wavelengths. All data
are normalized to the value at 730 nm.
2396 The Plant Cell
directly excites vibrational sublevels of PSII chlorophyll a mole-
cules, was debated in a discussion of that article (Pettai et al.,
2006; Trissl, 2006a, 2006b). The third proposed mechanism
involves reversed (uphill) spillover from the far-red chlorophyll
excitations in the PSI antenna to the PSII antenna (Pettai et al.,
2005a).
There are no reported far-red chlorophylls in the PSII antenna.
The long wavelength components from chlorophyll a species
that have been observed in the PSII absorption spectrum have
absorption bands just above 680 nm. Studies of the absorption
spectrumof LHCII isolated fromplants at room temperature have
identified low energy bands with peaks at 684 and 693 nm
(Zucchelli et al., 1990). Other studies performed at low temper-
ature, however, have not identified any significant absorption
bands higher than 677 to 678 nm in LHCII (Brown and Schoch,
1981; van Dorssen et al., 1987).
Spectral hole burning measurements at low temperatures on
spinach PSII core complexes have revealed that QA- formation
can be observed up to 730 nm (Hughes et al., 2006a, 2006b).
Two different photochemical events leading to QA reduction
could be distinguished. An absorption band, with a maximum at
689 nm,was linked to the lowest energy chlorophyll apigments in
CP47, and stretches out to 704 nm at 1.7K. For a second
absorption with a maximum at 705 nm, 80 and 30% of QA could
still be reduced using 708- and 728-nm light, respectively
(Hughes et al., 2006a, 2006b). This absorption was proposed
to be linked directly to a charge separating state of the special
pair chlorophylls (Hughes et al., 2006a, 2006b). No QA- formation
could be observed with illumination at 750 nm at 1.7K (Hughes
et al., 2006a).
When the three earlier suggestions for the origin of the far-red
absorbing species are reviewed in the light of this work, the
proposed uphill reversed spillover from PSI can immediately be
ruled out. The amount of PSI in PSII-enriched membranes is
insignificant and cannot account for the 45% S1 to S2 turnover
observed with a single laser flash at 750 nm. The fact that we see
an appreciable turnover on a single flash at 750 nm also in the
PSII core particles, which does not contain PSI, strengthens this
conclusion.
For the proposal of far-red chlorophylls in the PSII antenna, it is
interesting to study the PSII core particles that completely lack
the outer antenna components. Since far-red photosynthesis
was observed also in PSII cores, it is not (only) dependent on the
presence of these antenna components. If far-red chlorophylls
are present in PSII and act as the absorbing species, at least one
of these special chlorophylls (or chlorophyll dimers) has to be
located in the PSII core complex. Furthermore, the S1 to S2
turnover following a single flash in the PSII core preparation was
less efficient than in the PSII membranes. This could, in turn,
indicate that the outer antenna complex does contribute to the
absorption of the far-red light. However, estimations by Pettai
et al. (2005a) suggested on average only one far-red chlorophyll
per PSII. Another way of explaining the observed photochemistry
would be that a two-photon process is involved at longer
wavelengths to produce an excited state of sufficient energy to
initiate charge separation. In that case, we would expect the PSII
activity, as measured for example by the induction of FV, to rise
with the square of the applied laser power. However, the ob-
served power dependence does not give any support for this
explanation (see Supplemental Figure 5 online).
In the following, we discuss the consequences our data and
these considerations have for our understanding of the energet-
ics in PSII. Formation of P680*, which is the excited state of the
primary electron donor in PSII, from the excited antenna normally
initiates the primary charge separation to form P680+ and a Phe-,
which subsequently lead onwards to S-cycle advancement and
quinone reduction. However, it does not seem that this pathway
can explain our data in the far-red region. The photochemical
action spectra in Figure 5 are markedly red shifted also com-
pared with the 705-nm absorption band of Hughes et al. (2006a),
more shifted than can be explained by the higher temperature in
our measurements. For example, at 750 nm, we obtain almost
50% yield of the S2-state in a single flash (Figure 5, black). The
thermal energy (kBT) corresponds to only 10 nm at these wave-
lengths. Thus, only vibrational sublevels of P680 at several times
kBT of thermal energywill be possible to excite with 750-nm light.
Therefore, the fractional population of these sublevels will be
very small (<<1%) and would give only insignificant yields of, for
example, the S2-state compared with what we observe.
Direct excitation of vibrational sublevels in a single chlorophyll
a molecule in the antenna would be equally improbable, but the
fact that PSII membranes contain ;200 chlorophylls per PSII
center could give a combined contribution to the far-red absorp-
tion. However, when exciting in the far-red region, the steady
state fluorescence measured at 684 nm from PSII membranes
does not have the same excitation wavelength dependence as
our EPR and FV induction experiments (Figure 5). The FV induc-
tion indicates that efficient electron transfer to QA can be driven
at longer wavelengths than can induce fluorescence at 684 nm,
suggesting that different processes are involved in the two
phenomena. In addition, the maximal inducible FV is lower at
the far-red wavelengths. That stronger flashes must be used to
reach saturation at longer wavelengths is explained by the lower
absorbance. However, the saturation value at 532 and 730 nm is
95% 6 5% of the value obtained with a red (639 nm, 50 ms)
saturating actinic flash, while the saturation value at 760 nm is
only around 30%. The fact that the yield is lower at higher far-red
Figure 6. Demonstration of Oxygen Evolution Induced by Far-Red Light.
Flash-induced oxygen evolution patterns using 750-nm (A) and 532-nm
(B) laser flashes on PSII membranes (top) or thylakoid membranes
(bottom). The arrows indicate the first five flashes.
[See online article for color version of this figure.]
The Far-Red Limit of Photosystem II 2397
wavelengths, although saturating excitation is obtained, points
to a different intrinsic yield of charge separation in PSII for the far-
red light.
Therefore, we propose a model in which an excited state, X*,
different from P680*, can be generated by far-red light (Figure
7A). The different intrinsic yields of charge separation suggested
by the FV saturation data supports an alternative charge sepa-
ration pathway for far-red excitation. It is important to point out
that we are not suggesting that X is an unknown chromophore in
PSII, but rather that X* is an excited state from a known chro-
mophore that has not been previously observed and linked to
PSII activity. Direct measurement of the absorption spectrum of
PSII at wavelengths above 700 nm and at room temperature to
identify X is difficult due to the strong scattering by PSII mem-
branes (Hughes et al., 2006a). We have used an integrating
sphere to reduce scattering effects in the measurements of the
absorption spectrum of PSII membranes. In the region of interest
(730 to 800 nm), we have a substantial absorption (OD 0.005 to
0.01 in a 10-mg chlorophyll/mL sample) that could contain a
chromophore responsible for the far-red photoactivity of PSII
membranes (see Supplemental Figure 4 online). To account for
the photochemical yield obtained still at 780 nm, we estimate
that the energy of the first excited state of X* should not be higher
than ;1.65 eV (photon energy at 750 nm) above the ground
state. The much lower energy than P680* suggests that X* may
not be efficient in populating P680* by uphill energy transfer
(Figure 7A). This is supported by the fact that the red flank of the
684-nm fluorescence excitation spectrum (Figure 5, full line)
decreases more steeply with wavelength than the variable fluo-
rescence, the YZd
signal, and the multiline signal from the
S2-state, showing that population of P680* from X* cannot be
quantitative. As the OD above 700 nm was moderate and
identical in the measurement of the fluorescence excitation
spectrum and the variable fluorescence measurement, this dif-
ference cannot be attributed to optical saturation effects. It
should be noted that the multiline EPR signal from the S2-state
and the Phe- signal were induced at high sample concentration,
the YZd
signal at high concentration in a flat cell with short path
length, and the variable fluorescence in a sample with low
concentration, all of whichmakes direct quantitative comparison
difficult. If X* is not able to populate P680* directly, we suggest
that X* might undergo charge separation directly to form
P680+Phe- or an alternative primary charge separated state
that we denote X+Phe- (Figure 7A). Irrespective of which is the
primary charge separated state, our results indicate that it leads
to the same final YZd
QA- state because we observe efficient QA
reduction, YZd
formation (in Tris-washed samples), and S-state
turnover (in intact samples). Importantly, our data and the
scheme we propose put further constraints on the upper energy
limit of the primary charge separated state, be it P680+Phe- or
X+Phe-.
In Figure 7B, we compare estimated energies of different
states in PSII with the energy of photons at a few wavelengths.
Generally, P680* is assumed to be 1.83 V above the level of P680.
The energies of photons at 750 nm (1.65 eV), where we have
observed oxygen evolution, and at 790 nm (1.53 eV), close to our
outer edge for detected photochemistry, are also shown. Figure
7B also shows the proposed free energy of two charge separated
states in PSII. Earlier estimations of the free energy for the
primary charge separated state, P680+Phe-, that were based on
direct titration of the Phe/Phe- couple and equilibrium constants
between redox centers within PSII, were placed around 1.77 eV
(Klimov et al., 1978, 1979; Rutherford et al., 1981; Holzwarth,
1986) (Figure 7B, P680+Phe- i)), very close to the value assumed
for P680*. This has been questioned in two more recent mea-
surements of the charge recombination of the S2QA- state
(Rappaport et al., 2002) and the free energy difference between
an excited antenna state and the YZd
QA- pair (Grabolle and Dau,
2005). Both studies place the P680+Phe- pair around 1.65 V
(Figure 7B, P680+Phe- ii)). The latter assignment (P680+Phe-
;1.65 eV) is better in line with our results that far-red photons
can drive efficient charge separation. However, the observation
of light-driven electron transfer as high as 790 nm (photon energy
1.53 eV) might indicate that further adjustments of the primary
charge pair level could become necessary.
It is interesting to discuss which redox component(s) in PSII
in that case would be most likely to be adjusted. The YZd
QA- pair
has a considerably lower free energy (Rappaport et al., 2002)
(Figure 7B, ;1.29 V) than the P680+Phe- pair, mainly reflecting
the large free energy drop in the electron transfer fromPhe- toQA.
Consequently, there might exist some thermodynamic freedom
in the placement of the Phe/Phe- couple. By contrast, YZd
and the
higher S-states are all placed around +0.9 to 1.1 V to allow water
Figure 7. Proposal of an Alternative Charge Separation Pathway in PSI
Using the Energy of Far-Red Photons.
(A) Energy level scheme and reactions for the states involved in the
primary charge separation of PSII. We propose the existence of a state X*
that is directly generated by far-red light and that lies substantially lower
in energy than P680*. We further suggest that X* undergoes primary
charge separation to form either P680+Phe- or the new state X+Phe- and
ultimately leads to the same YZd
QA- state as with P680 excitation.
(B) Energies of photons of different wavelengths in comparison with
proposed free energies of charge separated states in PSII. From top to
bottom: energies of photons of at 680, 750, and 790 nm. Proposed free
energy for the P680+Phe- state; P680+Phe- i) based on Klimov et al. (1978,
1979), Rutherford et al. (1981), and Holzwarth (1986) and P680+Phe- ii)
based on Rappaport et al. (2002) and Grabolle and Dau (2005). Proposed
free energy for the YZ
d
QA- state (Rappaport et al., 2002).
2398 The Plant Cell
oxidation (;0.8 V). These values are critical for function, and
there are no large drops in free energy on the donor side of PSII.
This probably indicates that our results will lead to few readjust-
ments of the oxidation potentials among these donor-side com-
ponents.
In conclusion, we have observed photosynthetic activity in
PSII, in vitro, using long wavelength light up to 790 nm. The
efficiency of the far-red photons to induce full charge separation
and electron transfer leading to water oxidation leads us to
tentatively introduce a low energy excited state X* in PSII that can
be induced by far-red light. This excited state nevertheless leads
to the same charge separated YZd
QA- state as obtained when
exciting P680 with light below 700 nm. This suggests that the
action spectrum of PSII is wider than has been previously
thought and that PSII operates at wavelengths beyond those
that have been considered to be able to only drive PSI reactions.
The photosynthetic reactions in PSII in the far red occur at all
levels, from very purified PSII core samples to intact leaves
(Pettai et al., 2005a, 2005b). There is no reason that it would not
occur under natural conditions. Although the absorption is low,
an absorbed photon at, for example, 750 nm will drive PSII
electron transfer rather efficiently. It would thus be a valuable
addition for an organism living under conditions in which most of
the photosynthetically important radiation is lacking, for exam-
ple, in the shade of a dark forest. Of course, if such an organism is
exposed to normal sunlight, it will use this instead. Furtherwork is
needed to address the physiological consequences of this new
finding. It is also necessary to assess how the two photosystems
cooperate at these longer wavelengths.
METHODS
Growth Conditions
Spinach (Spinacia oleracea) was grown hydroponically at 208Cunder cool
white fluorescent light with light–dark periods of 12 h and with the light
intensity of 300 mE m22 s21. As a light source, dysprosium lamps of the
type Osram Power star HQI-E 400W/DV, relatively close to daylight, were
used.
PSII Membrane Preparation
PSII (BBY)membraneswere prepared fromspinach as described (Berthold
et al., 1981; Volker et al., 1985) and resuspended in 25 mM MES-NaOH,
pH 6.1, 400 mM sucrose, 15 mM NaCl, and 3 mM MgCl2 for storage at
2808C. For the EPR measurements, the salt composition was changed
to 10 mM NaCl, 10 mM MgCl2, and 5 mM CaCl2. Thylakoid membranes
were prepared as described (Mamedov et al., 2000) and used in a 10 mM
phosphate buffer, pH 7.4, with 100 mM sucrose and 5 mMNaCl. PSII core
particles were prepared as described (Smith et al., 2002).
Tris washing to remove the WOC was performed by suspending the
PSII membranes in 1.0 M Tris, pH 9.1, and incubating in light on ice for
30 min. After centrifugation, the pellets were washed twice in the
measuring buffer before storage at 2808C. This procedure removed
>90% of the bound Mn and the three extrinsic proteins from PSII
(Gadjieva et al., 1999).
Fluorescence Excitation Spectra
Steady-state fluorescence excitation spectra were obtained with a SPEX
Fluorolog 3 at 208C on PSII membrane samples (10 mg chlorophyll/mL).
Excitations were made between 725 and 780 nm, and the emission was
measured at 684 nm. The data were collected in 1-nm steps with an
integration time of 5 s at each point, and 30 scans were averaged. The
excitation and emission monochromator slits were 3 and 2 nm, respec-
tively.
Laser Light Source
A Spectra Physics Quanta Ray MOPO 730 optical parametric oscillator
pumped by a Spectra Physics PRO-290 Q-switched Nd:YAG laser (6-ns
flashes, 5 Hz) was used as the laser source. The bandwidth of the MOPO
730was60.1 nm.Control experimentsweremade to assure the quality of
the laser light as described in the Supplemental Methods online.
Flash-Induced Oxygen Evolution
The oxygen evolution pattern was measured on a Joliot-type bare
platinum electrode with 50 mM KCl. The samples (750 mg chlorophyll/
mL) were dark adapted on the electrode for 3 min prior to the measure-
ments. Laser flashes from theMOPO730 triggered at 1Hzwere usedwith
a power of ;4 mJ for the 532-nm flashes and ;2.5 mJ for the 750-nm
flashes.
Application of Laser Flashes for Fluorescence Measurements
A thermostated (208C) and stirred quartz cell was filled with 3.5 mL of PSII
membranes at 25 mg chlorophyll/mL and exposed to 1 to 900 flashes of
;25 mJ at indicated wavelengths using the MOPO 730.
Variable Fluorescence Decay Kinetics
First, the PSII sample was exposed to the far-red laser flashes as
described above. One minute after the last far-red flash, the induction
and subsequent decay of the FV wasmeasured. Themeasurements were
done in a double modulation fluorometer (PSI Photon Instruments). After
the actinic flash of the fluorometer (LEDs at 639 nm, 50 ms), eight
measuring light pulses (2.0ms) were applied per decade in the range from
150ms to 180 s. Fittings of a triple exponential function to the decay traces
were made as described (Mamedov et al., 2000).
Power andWavelength Dependence of FV Induced by Single
Far-Red Flashes
With the same laser systemas above, the far-red flashwas used to induce
directly FV in a cuvette with 1.5 mL of PSII membranes at 10 mg
chlorophyll/mL inhibited by 10 mM DCMU. The level of fluorescence
was recorded with a measuring light pulse every 10 ms. The normalized
FV (nFV) was corrected using FV(corrected) = nFV/(1 2 0.5(1 2 nFV)) to
account for the nonlinear relationship between FV and [QA-] (Joliot and
Joliot, 1964). The corrected fluorescence data can thereby be used as a
measure of the level of reaction centers in which QA is reduced. Assuming
independent photon absorption events by the reaction center pigments,
the fraction of reaction centers that are not excited by a single flash will be
given by a Poisson distribution: P(0) = e-N, whereN is the average number
of photons absorbed per reaction center. Then, the power dependence
becomes: FV = FV(sat) · (1-e-N), where FV(sat) is the saturating FV signal. N
can also be expressed as fabs/nPSII · nhy, where fabs is the fraction of light
absorbed, nPSII is the number of PSII reaction centers in the sample (;0.1
nmol), and nhy is the number of photons in a flash. From a plot of FV as a
function of nhy, it is then possible to determine FV(sat) and fabs.
Application of Laser Flashes for EPR Spectroscopy of the S-States
Synchronized S1-state samples (1.8 mg chlorophyll/mL) were prepared
as described (Zhang and Styring, 2003). Phenyl-p-benzoquinone (50 mM
in DMSO, final concentration 1 mM) was used as electron acceptor.
The Far-Red Limit of Photosystem II 2399
Thereafter, laser flashes from the MOPO 730 (25 mJ) of the desired
wavelength were applied to the EPR tubes at 208C. The samples were
frozen within 1 to 2 s in a dry-ice ethanol bath and transferred to N2(l). In
experiments with the PSII core preparation, the dark-adapted EPR
sample (1.0 mg chlorophyll/mL) was used in the absence of phenyl-
p-benzoquinone. The sample was given one and 100 flashes at 750 nm at
208C and was then directly frozen.
For the Phe- measurement, PSII-enriched membranes (2.0 mg chloro-
phyll/mL) were fully reduced using sodium dithionite (Na2S2O4, final
concentration 50 mM). Laser flashes from the MOPO 730 of desired
wavelength were applied to the EPR tubes at 208C. The samples were
frozen within 1 s in a dry-ice ethanol bath and transferred to N2(l) before
the measurements.
YZd
measurements at room temperature were performed in Tris-
washed PSII membranes (2.0 mg chlorophyll/mL) in the presence of the
ferricyanide (K3[Fe(CN)6])/ferrocyanide (K4[Fe(CN)6]) couple (10 mM).
EPR Spectroscopy
EPR spectra were recordedwith an ELEXSYSE500 spectrometer (Bruker
Biospin) equipped with a SuperX bridge and a SHQE4122 cavity. For the
low temperaturemeasurements, anOxford InstrumentCryostat and ITC-4
temperature controller were used. The split EPR signal from the S3-state
was induced by IR illumination (830 nm) for 30 min at 5K as described (Su
et al., 2007). This was followed by visible illumination for 10 min at 5K to
induce the split EPR signals from the S0- and S1-states (Su et al., 2007).
EPR spectra were analyzed with the Bruker Xepr 2.1 software. The split
EPR signal from the S3-state was obtained as the IR light minus dark
difference spectra. The split EPR signals from the S1- and S0-states were
obtained as the visible light illuminated minus IR light illuminated differ-
ence spectra.
For the kinetic measurements of YZ
d
at room temperature, the sample
was placed in an EPR flat cell (250 mL). The laser flashes were directed
directly into the EPR cavity and were synchronized with EPR acquisition
using a home-built triggering system. The data were obtained at the low
field peak of the YZ
d
radical EPR spectrum (3345 G). Fifty or 250
accumulations were used at 532 or 730 to 790 nm, respectively.
Supplemental Data
The following materials are available in the online version of this article.
Supplemental Figure 1. Effect of Ferricyanide on FV in a Far-Red-
Treated PSII Membrane Sample.
Supplemental Figure 2. The Multiline EPR Signal from the S2-State
Induced by 730- and 790-nm Light.
Supplemental Figure 3. The Fraction of FV Induced after a Single
Flash at 532 nm.
Supplemental Figure 4. The Absorption Spectrum of PSII Mem-
branes at 208C Measured Using an Integrating Sphere.
Supplemental Figure 5. Power Dependence of FV Induction at 750
nm Fit with Functions Representing One- or Two-Photon Processes.
Supplemental Methods. Control Experiments with Optical Filters.
ACKNOWLEDGMENTS
This article is dedicated to Achim Trebst (Ruhr Universitat Bochum,
Germany) on the occasion of his 80th birthday. Paul Smith, Ron Pace,
and Elmars Krausz (The Australian National University, Canberra,
Australia) are acknowledged for providing the PSII core preparation.
This work was supported by the Swedish Research Council, the Knut
and Alice Wallenberg Foundation, and the Swedish Energy Agency.
Received October 31, 2008; revised July 8, 2009; accepted August 4,
2009; published August 21, 2009.
REFERENCES
Babcock, G.T., Blankenship, R.E., and Sauer, K. (1976). Reaction
kinetics for positive charge accumulation on the water side of
choloplast photosystem II. FEBS Lett. 61: 286–289.
Babcock, G.T., Barry, B.A., Debus, R.J., Hoganson, C.W., Atamian,
M., McIntosh, L., Sithole, I., and Yocum, C.F. (1989). Water oxida-
tion in photosystem II. From radical chemistry to multielectron chem-
istry. Biochemistry 28: 9557–9565.
Berthold, D.A., Babcock, G.T., and Yocum, C.F. (1981). A highly
resolved, oxygen-evolving photosystem II preparation from spinach
thylakoid membranes. FEBS Lett. 134: 231–234.
Blankenship, R.E. (2002). Molecular Mechanisms of Photosynthesis.
(Oxford, UK: Blackwell Science).
Boussac, A., Sugiura, M., Kirilovsky, D., and Rutherford, A.W. (2005).
Near-infrared-induced transitions in the manganese cluster of photo-
system II: Action spectra for the S2 and S3 redox states. Plant Cell
Physiol. 46: 837–842.
Brown, J.S., and Schoch, S. (1981). Spectral analysis of chlorophyll-
protein complexes from higher plant chloroplasts. Biochim. Biophys.
Acta 636: 201–209.
Crofts, A.R., and Wraight, C.A. (1983). The electrochemical domain of
photosynthesis. Biochim. Biophys. Acta 726: 149–185.
Dismukes, G.C., and Siderer, Y. (1981). Intermediates of a polynuclear
manganese center involved in photosynthetic oxidation of water.
Proc. Natl. Acad. Sci. USA 78: 274–278.
Emerson, R., Chalmers, R., and Cederstrand, C. (1957). Some factors
influencing the long-wave limit of photosynthesis. Proc. Natl. Acad.
Sci. USA 43: 133–143.
Emerson, R., and Lewis, C.M. (1943). The dependence of the quantum
yield of chlorella photosynthesis on wave length of light. Am. J. Bot.
30: 165–178.
Ferreira, K.N., Iverson, T.M., Maghlaoui, K., Barber, J., and Iwata, S.
(2004). Architecture of the photosynthetic oxygen-evolving center.
Science 303: 1831–1838.
Gadjieva, R., Mamedov, F., Renger, G., and Styring, S. (1999).
Interconversion of low- and high-potential forms of cytochrome b559
in Tris-washed photosystem II membranes under aerobic and anaer-
obic conditions. Biochemistry 38: 10578–10584.
Gobets, B., and van Grondelle, R. (2001). Energy transfer and trapping
in photosystem I. Biochim. Biophys. Acta 1507: 80–99.
Grabolle, M., and Dau, H. (2005). Energetics of primary and secondary
electron transfer in Photosystem II membrane particles of spinach
revisited on basis of recombination-fluorescence measurements.
Biochim. Biophys. Acta 1708: 209–218.
Greenbaum, N.L., and Mauzerall, D. (1991). Effect of irradiance level
on distribution of chlorophylls between PS II and PS I as determined
from optical cross-sections. Biochim. Biophys. Acta 1057: 195–207.
Havelius, K.G.V., Su, J.-H., Feyziyev, Y., Mamedov, F., and Styring,
S. (2006). Spectral resolution of the split EPR signals induced by
illumination at 5 K from the S1, S3, and S0 states in photosystem II.
Biochemistry 45: 9279–9290.
Holzwarth, A.R. (1986). Fluorescence lifetimes in photosynthetic sys-
tems. Photochem. Photobiol. 43: 707–725.
Hughes, J.L., Smith, P., Pace, R., and Krausz, E. (2006a). Charge
separation in photosystem II core complexes induced by 690–730 nm
excitation at 1.7 K. Biochim. Biophys. Acta 1757: 841–851.
Hughes, J.L., Smith, P.J., Pace, R.J., and Krausz, E. (2006b). Spectral
hole burning at the low-energy absorption edge of photosystem II
core complexes. J. Lumin. 119: 298–303.
2400 The Plant Cell
Itoh, S., Mino, H., Itoh, K., Shigenaga, T., Uzumaki, T., and Iwaki, M.
(2007). Function of chlorophyll d in reaction centers of photosystems I
and II of the oxygenic photosynthesis of Acaryochloris marina. Bio-
chemistry 46: 12473–12481.
Joliot, A., and Joliot, P. (1964). Etude cinetique de la reaction photo-
chimique liberant l’oxygene au cours de la photosynthese. C. R. Acad.
Sci. Paris 258: 4622–4625.
Joliot,P., Joliot,A.,Bouges,B., andBarbieri,G. (1971). Studiesof system
II photocenters by comparative measurements of luminescence fluores-
cence and oxygen emission. Photochem. Photobiol. 14: 287–305.
Jordan, P., Fromme, P., Witt, H.T., Klukas, O., Saenger, W., and
Krauß, N. (2001). Three-dimensional structure of cyanobacterial
photosystem I at 2.5 A resolution. Nature 411: 909–917.
Karapetyan, N.V., Schlodder, E., van Grondelle, R., and Dekker, J.P.
(2006). The long wavelength chlorophylls of photosystem I. In Photo-
system I: The Light-Driven Plastocyanin:Ferredoxin Oxidoreductase, J.
H. Golbeck, ed (Dordrecht, The Netherlands: Springer), pp. 177–192.
Klimov, V.V., Allakhverdiev, S.I., Demeter, S., and Krasnovskii, A.A.
(1979). Photo-reduction of pheophytin in the photosystem-2 of chlo-
roplasts depending on the oxidation-reduction potential of the me-
dium. Dokl. Akad. Nauk SSSR 249: 227–230.
Klimov, V.V., Allakhverdiev, S.I., and Pashchenko, V.Z. (1978). Mea-
surement of activation-energy and lifetime of fluorescence of photo-
system 2-chlorophyll. Dokl. Akad. Nauk SSSR 242: 1204–1207.
Klimov, V.V., Dolan, E., and Ke, B. (1980). EPR properties of an
intermediary electron acceptor (pheophytin) in photosystem-II reac-
tion centers at cryogenic temperatures. FEBS Lett. 112: 97–100.
Loll, B., Kern, J., Saenger, W., Zouni, A., and Biesiadka, J. (2005).
Towards complete cofactor arrangement in the 3.0 A resolution
structure of photosystem II. Nature 438: 1040–1044.
Mamedov, F., Stefansson, H., Albertsson, P.-A., and Styring, S. (2000).
Photosystem II in different parts of the thylakoid membrane: A functional
comparison between different domains. Biochemistry 39: 10478–10486.
Miller, A.F., and Brudvig, G.W. (1991). A guide to electron paramag-
netic resonance spectroscopy of Photosystem II membranes. Bio-
chim. Biophys. Acta 1056: 1–18.
Miyashita, H., Adachi, K., Kurano, N., Ikemoto, H., Chihara, M., and
Miyachi, S. (1997). Pigment composition of a novel oxygenic photo-
synthetic prokaryote containing chlorophyll d as the major chlorophyll.
Plant Cell Physiol. 38: 274–281.
Miyashita, H., Ikemoto, H., Kurano, N., Adachi, K., Chihara, M., and
Miyachi, S. (1996). Chlorophyll d as a major pigment. Nature 383: 402.
Miyashita, H., Ikemoto, H., Kurano, N., Miyachi, S., and Chihara, M.
(2003). Acaryochloris marina gen. et sp nov (Cyanobacteria), an
oxygenic photosynthetic prokaryote containing Chl d as a major
pigment. J. Phycol. 39: 1247–1253.
Nugent, J.H., Muhiuddin, I.P., and Evans, M.C. (2002). Electron
transfer from the water oxidizing complex at cryogenic temperatures:
The S1 to S2 step. Biochemistry 41: 4117–4126.
Petrouleas, V., Koulougliotis, D., and Ioannidis, N. (2005). Trapping of
metalloradical intermediates of the S-states at liquid helium temper-
atures. Overview of the phenomenology and mechanistic implica-
tions. Biochemistry 44: 6723–6728.
Pettai,H.,Oja,V., Freiberg,A.,andLaisk,A. (2005a).Photosyntheticactivity
of far-red light in green plants. Biochim. Biophys. Acta 1708: 311–321.
Pettai, H., Oja, V., Freiberg, A., and Laisk, A. (2005b). The long-
wavelength limit of plant photosynthesis. FEBS Lett. 579: 4017–4019.
Pettai, H., Oja, V., Freiberg, A., and Laisk, A. (2006). Response to the
“Comments to water-splitting activity of Photosystem II by far-red light
in green plants” by H.-W. Trissl. Biochim. Biophys. Acta 1757: 158–159.
Pospısil, P., and Dau, H. (2000). Chlorophyll fluorescence transients of
Photosystem II membrane particles as a tool for studying photosyn-
thetic oxygen evolution. Photosynth. Res. 65: 41–52.
Rappaport, F., Guergova-Kuras, M., Nixon, P.J., Diner, B.A., and
Lavergne, J. (2002). Kinetics and pathways of charge recombination
in photosystem II. Biochemistry 41: 8518–8527.
Renger, G., Eckert, H.J., Bergmann, A., Bernarding, J., Liu, B.,
Napiwotzki, A., Reifarth, F., and Eichler, H.J. (1995). Fluorescence
and spectroscopic studies of exciton trapping and electron transfer in
photosystem II of higher plants. Aust. J. Plant Physiol. 22: 167–181.
Robinson, H.H., and Crofts, A.R. (1983). Kinetics of the oxidation-
reduction reactions of the photosystem II quinone acceptor complex,
and the pathway for deactivation. FEBS Lett. 153: 221–226.
Roffey, R.A., van Wijk, K.J., Sayre, R.T., and Styring, S. (1994).
Spectroscopic characterization of tyrosine-Z in histidine 190 mutants
of the D1 protein in photosystem II (PSII) in Chlamydomonas rein-
hardtii. Implication for the structural model of the donor side of PSII. J.
Biol. Chem. 269: 5115–5121.
Rutherford, A.W., Mullet, J.E., and Crofts, A.R. (1981). Measurement
of the midpoint potential of the pheophytin acceptor of photosystem
II. FEBS Lett. 123: 235–237.
Rutherford, A.W., and Zimmermann, J.L. (1984). A new EPR signal
attributed to the primary plastosemiquinone acceptor in Photosystem
II. Biochim. Biophys. Acta 767: 168–175.
Smith, P.J., Peterson, S., Masters, V.M., Wydrzynski, T., Styring, S.,
Krausz, E., and Pace, R.J. (2002). Magneto-optical measurements of
the pigments in fully active photosystem II core complexes from
plants. Biochemistry 41: 1981–1989.
Styring, S., Virgin, I., Ehrenberg, A., and Andersson, B. (1990). Strong
light photoinhibition of electrontransport in photosystem II. Impair-
ment of the function of the first quinone acceptor, QA. Biochim.
Biophys. Acta 1015: 269–278.
Su, J.H., Havelius, K.G., Ho, F.M., Han, G., Mamedov, F., and Styring,
S. (2007). Formation spectra of the EPR split signals from the S0, S1,
and S3 states in photosystem II induced by monochromatic light at 5
K. Biochemistry 46: 10703–10712.
Thapper, A., Mamedov, F., and Styring, S. (2008). IR-induced photo-
chemistry in photosystem II. In Photosynthesis. Energy from the Sun:
14th International Congress on Photosynthesis, J.F. Allen, E. Gantt,
J.H. Golbeck, and B. Osmond, eds (Dordrecht, The Netherlands:
Springer), pp. 521–524.
Tomo, T., Okubo, T., Akimoto, S., Yokono, M., Miyashita, H.,
Tsuchiya, T., Noguchi, T., and Mimuro, M. (2007). Identification of
the special pair of photosystem II in a chlorophyll d-dominated
cyanobacterium. Proc. Natl. Acad. Sci. USA 104: 7283–7288.
Trissl, H.-W. (2006a). Comments to water-splitting activity of photosystem
II by far-red light in green plants. Biochim. Biophys. Acta 1757: 155–157.
Trissl, H.-W. (2006b). Reply to Pettai et al.’s response. Biochim.
Biophys. Acta 1757: 160.
van Dorssen, R.J., Plijter, J.J., Dekker, J.P., den Ouden, A., Amesz,
J., and van Gorkom, H.J. (1987). Spectroscopic properties of chlo-
roplast grana membranes and of the core of Photosystem II. Biochim.
Biophys. Acta 890: 134–143.
Volker, M., Ono, T., Inoue, Y., and Renger, G. (1985). Effect of trypsin
on PSII particles. Correlation between Hill activity, Mn-abundance and
peptide pattern. Biochim. Biophys. Acta 806: 25–34.
Zhang, C., Boussac, A., and Rutherford, A.W. (2004). Low-
temperature electron transfer in photosystem II: a tyrosyl radical
and semiquinone charge pair. Biochemistry 43: 13787–13795.
Zhang, C., and Styring, S. (2003). Formation of split electron para-
magnetic resonance signals in photosystem II suggests that tyrosineZcan be photooxidized at 5 K in the S0 and S1 states of the oxygen-
evolving complex. Biochemistry 42: 8066–8076.
Zucchelli, G., Jennings, R.C., and Garlaschi, F.M. (1990). The presence of
long-wavelength chlorophyll a spectral forms in the light-harvesting chlo-
rophyll a/b protein complex II. J. Photochem. Photobiol. B 6: 381–394.
The Far-Red Limit of Photosystem II 2401
DOI 10.1105/tpc.108.064154; originally published online August 21, 2009; 2009;21;2391-2401Plant Cell
Anders Thapper, Fikret Mamedov, Fredrik Mokvist, Leif Hammarström and Stenbjörn StyringDefining the Far-Red Limit of Photosystem II in Spinach
This information is current as of September 11, 2020
Supplemental Data /content/suppl/2009/08/07/tpc.108.064154.DC1.html
References /content/21/8/2391.full.html#ref-list-1
This article cites 54 articles, 5 of which can be accessed free at:
Permissions https://www.copyright.com/ccc/openurl.do?sid=pd_hw1532298X&issn=1532298X&WT.mc_id=pd_hw1532298X
eTOCs http://www.plantcell.org/cgi/alerts/ctmain
Sign up for eTOCs at:
CiteTrack Alerts http://www.plantcell.org/cgi/alerts/ctmain
Sign up for CiteTrack Alerts at:
Subscription Information http://www.aspb.org/publications/subscriptions.cfm
is available at:Plant Physiology and The Plant CellSubscription Information for
ADVANCING THE SCIENCE OF PLANT BIOLOGY © American Society of Plant Biologists