DOI: 10.1002/cssc.201500332
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Full Papers
Gas Transfer Controls Carbon Limitation During Biomass
Production by Marine Algae
Bojan Tamburic,*[a] Christian R. Evenhuis,[a] David J. Suggett,[a] Anthony W. D. Larkum,[a]
John A. Raven,[a, b] and Peter J. Ralph[a]
This study presents the first in-depth analysis of CO2 limitation
on the biomass productivity of the biofuel candidate marine
microalga Nannochloropsis oculata. Net photosynthesis decreased by 60 % from 125 to 50 mmolO2 L1 h1 over a 12 h light
cycle as a direct result of carbon limitation. Continuous dissolved O2 and pH measurements were used to develop a detailed diurnal mechanism for the interaction between photosynthesis, gas exchange and carbonate chemistry in the
photo-bioreactor. Gas exchange determined the degree of
carbon limitation experienced by the algae. Carbon limitation
was confirmed by delivering more CO2, which increased net
photosynthesis back to its steady-state maximum. This study
highlights the importance of maintaining replete carbon concentrations in photo-bioreactors and other culturing facilities,
either by constant pH operation or preferably by designing
a feedback loop based on the dissolved O2 concentration.
Introduction
Biofuel from microalgae
croalga Nannochloropsis oculata (N. oculata), which is known
for its high lipid productivity.[7] To develop production systems
and processes that maximise biofuel output, it is first necessary
to gain a deep understanding of photosynthetic controls for
a given algal species.
&&please provide academic titles (Prof., Dr.) for all authors.&
& Microalgae have the potential to provide sustainable and
affordable transport fuels in the future. These unicellular photosynthetic organisms use light energy to fix atmospheric CO2
and synthesise biomass. Algal biomass is then processed
chemically to either biodiesel by transesterification or to biocrude oil by hydrothermal liquefaction.[1] Algal biofuels are of
particular interest in Australia as many algae can be grown in
hostile conditions, such as saltwater ponds on arid coastal terrain.[2] Algae cultivation that covers 1 million hectares of land
(roughly the size of Sydney) would, by a conservative estimate,[3] produce enough bio-crude to replace 40 billion litres
of crude oil per annum, which is equal to the entire crude oil
demand of Australia, 85 % of which is currently imported.[4]
It has been estimated that there are over 350 000 extant species of algae, which range across the most commonly recognised green, brown, red and golden brown algae to other
forms that have been discovered only recently.[5] More than
half of the ~ 20 microalgal species that are currently used in
biofuel production are green algae (Chlorophyta), but there is
a huge biodiversity of algae yet to be explored for bio-energy
applications.[6] This includes the biofuel candidate marine mi-
Limits to biomass production
Resource availability fundamentally governs algal growth rates,
the rate of biomass accumulation and hence the maximum
achievable yield of biofuel.[8] Photosynthesis is driven by light
energy, photochemistry and downstream energy transformations, which generate a reductant and adenosine triphosphate
(ATP) that fuel metabolic reactions and consume inorganic nutrients (for example, carbon, nitrogen and phosphorus) to construct complex, energy-rich organic macromolecular compounds. The dependence of both the growth rate and biomass
yield on the availability of these resources can be described
mathematically using threshold and co-limitation theory, with
taxonomic-specific variations that determine whether light
availability and nutrient concentrations are limiting, saturating
or excessive.[9] The algal cell size, in particular, influences the
effectiveness of resource acquisition; for example, larger cells
with a smaller surface-area-to-volume quotient exhibit lower
light harvesting efficiency caused by enhanced pigment packaging as well as a lower inorganic nutrient uptake.[10] The external nutrient concentration and the intracellular demand for
inorganic nutrients both dictate the elemental stoichiometry of
an algal cell, described most commonly by the “Redfield
Ratio”.[11] Consequently, a large number of factors, which can
ultimately operate in complex positive or negative feedback
loops, influence how rapidly microalgal cells drive photosynthesis and subsequently accrue biomass.
[a] B. Tamburic, C. R. Evenhuis, D. J. Suggett, A. W. D. Larkum, J. A. Raven,
P. J. Ralph
Plant Functional Biology and Climate Change Cluster
University of Technology Sydney
Ultimo, New South Wales ### (Australia)
[b] J. A. Raven
Division of Plant Sciences
University of Dundee at the James Hutton Institute
Invergowrie ### (United Kingdom)
Supporting Information for this article is available on the WWW under
http://dx.doi.org/10.1002/cssc.201500332.
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If cells are in exponential growth, the allocation of energy,
reductant and assimilated inorganic nutrients are near optimal.
Under these ideal conditions, the cells are acclimated to
a steady-state supply of resources, regardless of whether the
resources are available in excess or limiting.[8, 9] In contrast, conditions in large-scale biofuel cultivation facilities (and in nature
in general) are highly variable so that an algal culture can experience different limitations depending on the time of day,
the age of the culture and the location within the culture
vessel.[12] In addition to maximising biomass production rate,
algal cells also allocate resources to fitness-increasing traits,
such as defence against grazers, parasitoids and viruses. Under
variable environmental conditions, algal cells are in a dynamic
state and the instantaneous growth rate depends on what
limit is already imposed. This is a fundamental challenge for
algae producers looking to increase algal biofuel yield, as the
insights of how algae grow under steady-state conditions in
the laboratory may not be relevant to large-scale production
conditions. For example, light availability in an algal pond decreases exponentially with depth and thus small shifts in cell
location caused by mixing or turbulence result in the algal
cells experiencing a highly stochastic light field.[13]
Microalgae have, therefore, evolved numerous mechanisms
to cope with environmental variability, which can operate on
scales of microseconds to days. For example, the reaction centres continually balance the excitation pressure required to
convert energy photochemically and produce reductant and
ATP;[14] similarly, cells regulate the supply of inorganic nutrients, which includes carbon.[15] All such regulatory mechanisms incur costs to the cells and reduce the efficiency of biomass accumulation, that is, growth.[16] It is, therefore, important
to be aware of the regulatory costs upon maximisation of the
biomass yield of a microalgal culture system. Recently, advanced molecular biology tools have become increasingly
used to identify lipid production pathways[17] as well as genetic
markers of algal stress.[18] These studies produce intriguing results, which are only reproducible and valid if physical parameters such as light, temperature and nutrient availability are
measured and controlled.
Photo-bioreactors (PBRs) are devices used to grow microalgae on a laboratory scale. They are used to maintain precise
control over the algal growth environment, such as light and
gas supply, and continuously measure key parameters, which
include the dissolved oxygen concentration and pH. PBR studies facilitate a deeper understanding of the effect of dynamic
fluctuations on conditions and limitations in biomass production and they generate more reproducible experimental results
than open systems. PBRs exist in multiple geometries, which
include flat-panel, tubular, annular and helical systems.[19] The
design of a PBR influences the limitations that the culture experiences. For example, an important consideration in any PBR
design is the provision of appropriate illumination to algal
cells.[20] Light is absorbed and scattered by algal cells, which results in the formation of an attenuation gradient normal to the
PBR surface. Another important factor is the PBR surface-tovolume quotient: a relatively large surface area increases the
effectiveness of light absorption but may lead to photoChemSusChem 0000, 00, 0 – 0
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damage in algae, whereas a relatively large volume makes
better use of space but requires additional energy for mixing,
gas exchange and aeration. Fluid dynamics control the circulation and movement of individual algal cells within this light
gradient, and the photochemical reactions of photosynthesis
and respiration add further complexity to the fluid dynamics of
gas exchange.[21]
Carbon availability and limitation
Carbon is an essential element for the biosynthesis of organic
molecules within a cell; algae have developed (or inherited)
a series of metabolic mechanisms that harvest and fix inorganic carbon. Microalgal photosynthesis fixes inorganic carbon
into sugars, which then act as substrates for more complex
molecules, such as starch and lipids. CO2 is fixed by the Calvin–
Benson cycle by the enzyme ribulose bisphosphate carboxylase oxygenase (RuBisCO) using ATP as energy and nicotinamide adenine dinucleotide phosphate (NADPH) as the reductant. Importantly, O2 competes continuously with CO2 for RuBisCO, and the process of O2 consumption by RuBisCO is
known as photo-respiration.[22] Photo-respiration reduces CO2
fixation efficiency by 20 to 30 %, and the rate of photo-respiration increases under a carbon-limited environment.[23, 24] Microalgae have evolved a series of carbon-concentrating mechanisms (CCMs) independently that increase the concentration of
CO2 available at the RuBisCO active site and thereby inhibit
photo-respiration competitively.[25] Many of these CCMs actively pump bicarbonate (HCO3) into algal cells, in which it is dehydrated to CO2 by the carbonic anhydrase enzyme, which elevates intracellular CO2 that, in turn, decreases photo-respiration
and potentially increases the energetic efficiency of photosynthesis.[16]
The rate of photosynthesis in the PBR can be calculated immediately from changes in oxygen concentration.[26] In an algal
monoculture, the concentration of dissolved O2 and CO2 in
a PBR is in dynamic equilibrium with air that is bubbled
through the PBR (Figure 1). The relationship for oxygen may
be described by Fick’s Law &&which one is meant?&
&[Eq. (1)]:
d½O2
dt
¼ ðP RÞ kL að½O2 ½O2 eq Þ
ð1Þ
in which [O2] is the dissolved O2 concentration; (PR) is the
rate of net photosynthetic O2 production, that is, the rate of
photosynthesis P minus the rate of dark (mitochondrial) respiration R; kLa is the gas exchange (or mass transfer) coefficient;
and [O2]eq is the equilibrium or Henry’s Law O2 concentration.
Dissolved O2 concentrations can be measured directly by using
an optode or an electrode.
A similar mathematical expression can be written for CO2.[27]
Although the mass transfer coefficient is scaled by the ratio of
molecular masses, there is an additional complication in that
dissolved CO2 is in equilibrium with HCO3 and carbonate ions
(CO32 ; Figure 1). The addition of CO2 to seawater increases
the concentration of HCO3 but decreases the concentration of
CO32.[28] The formation of HCO3 leads to the dissociation of
2
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internal conversion to CO2 and a leak of some of the CO2 back
to the medium.[34] Importantly, the conversion of bicarbonate
to CO2 involves the production of equal quantities of hydroxyl
ions or the uptake of equal quantities of protons. Intracellular
acid–base regulation involves the efflux of these hydroxyl ions
or protons, so that the effect on the medium acid–base and
equilibrium concentrations of inorganic carbon species is the
same for bicarbonate entry as would have been the case for
CO2 uptake.[26, 36]
Therefore, the pH increases during the photo-period in the
diurnal light cycle because the consumption of bicarbonate,
and the corresponding influx of protons and/or efflux of hydroxyl ions by photosynthesis is faster than the re-supply of inorganic carbon as CO2 from the gas stream. Some of this pH
increase is also the result of nitrate assimilation if nitrate is the
nitrogen source.[36, 37] There are strong experimental indications
that inorganic carbon may limit algal growth across the diurnal
photo-period.[38, 39] The concept of using a constant pH system,
or pH-stat, to control carbon availability in a PBR has been
used extensively.[40–43] The pH-stat solves many of the challenges associated with managing carbonate chemistry in largescale culturing facilities, however, there are some advantages
in alternative methods. Firstly, if CO2 addition was managed
more precisely, it may be possible to reduce running costs or
to improve yields of algal biomass production. Secondly, if the
pH (or equivalently CO2) is controlled, the rate of carbon fixation cannot be estimated from changes in pH.
Figure 1. The major continuous inputs to a gas-bubbled PBR (light, O2, CO2)
and the main processes [P: photosynthesis; R: respiration; kLa: gas exchange; carbonate chemistry including bicarbonate ions (HCO3), carbonate
ions (CO32) and protons (H+)].
protons, which reduces the pH of the solution in the PBR;
however, this pH shift is buffered by the corresponding decrease in CO32.[29] This dampened pH response in saltwater
cultures calls for greater measurement precision to resolve
changes in carbonate chemistry. The various dissociation constants of carbonate chemistry have been measured as a function of temperature, salinity and alkalinity[26, 28] and can be used
to calculate the concentrations of carbonate species in solution. The equations can be solved conveniently using the
spreadsheet “CO2 sys”.[30] Hence, pH is an indirect measure of
the quantity of inorganic carbon available in a stable marine
environment. However, once biology becomes involved, photosynthesis (P) and dark respiration (R) processes alter the pH
value. Algal photosynthesis fixes CO2 and produces O2 as a byproduct, whereas respiration is essentially the elemental reversal of this photosynthesis (Figure 1). So, if pH and [O2] are
monitored continuously and provided that gas exchange and
carbonate chemistry are measured, it is possible disentangle
the rate of photosynthesis from the dynamics of gas transfer in
a PBR.[24, 31]
The carbonate chemistry of seawater equilibrated with air at
the ambient CO2 concentration of 400 ppm indicates that the
predominant inorganic carbon species is bicarbonate, with carbonate next most abundant and CO2 even less abundant.[26, 27]
The CO2 concentration in air-equilibrated seawater is approximately the same as that in air; however, the mass transfer coefficient of CO2 is 10 000-fold lower in seawater, therefore, the
supply of CO2 to the surface of photosynthesising cells in seawater is much slower than that in air.[32] This makes bicarbonate, present at 200 times the concentration of CO2, a clear
candidate for transport across the plasmalemma by the CCM
present in most marine microalgae, which include many candidate biofuel species.[33–35] The Nannochloropsis CCM is based
on an active bicarbonate influx across the plasmalemma with
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Aims and objectives
The aims of this study are to determine the carbon availability
in PBRs using measurements of dissolved oxygen concentration [O2] and pH, and to investigate the effects of carbon limitation on the green microalga N. oculata. The objectives are to
determine when N. oculata cells become carbon limited during
the diurnal light cycle, to quantify to what extent this carbon
limitation affects their photosynthetic activity and to examine
whether CO2 addition can alleviate the situation.
Results and Discussion
Diurnal [O2] and pH variations
Nannochloropsis oculata cells were cultivated to an exponential
growth phase under a 12:12 h diurnal light/dark cycle in two
PBRs. The dissolved oxygen concentration [O2] and pH were
measured continuously, and the cell density was measured by
automated cell counts (complete results profile available in the
Supporting Information, page 1). Diurnal [O2] and pH profiles
consistently follow the characteristic and reproducible trends
shown on page 2 in the Supporting Information. To investigate
this phenomenon in more detail, a single representative light/
dark period is shown in Figure 2; five distinct phases (A, B, C,
D and E) have been assigned to represent the variations in [O2]
and pH value.
During the dark cycle (phases D and E) the [O2] profile remains steady at, or near, the [O2] minimum of 218 mmol L1
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cantly slower than the corresponding [O2] response (Figure 2 a).
The rate of pH increase slows gradually, and the pH reaches
a maximum value of 9.5 near the end of the light cycle
(phase C). During the dark cycle (phases D and E), the pH gradually returns to its &&dark&& minimum of 8.0.
[O2] as a measure of net photosynthesis
The net rate of photosynthetic O2 production or consumption
can be calculated from the dissolved oxygen concentration.[26]
In this experiment, the “spikes” in the [O2] profile (Figure 2 a)
are artefacts that were introduced deliberately to measure the
rate of photosynthesis and gas exchange at specific time
points.[38, 44] The spikes were created by switching off air bubbling for approximately 15 min before turning it back on again
(Figure 3).
Initially, there is a dynamic equilibrium between gas exchange and the biological processes, which gives an [O2] of
[O2]de.[32] If the gas supply is turned off, the gas transfer coefficient is negligible and Equation (1) can be simplified to Equations (2) and (3):
Figure 2. Representative a) [O2] and b) pH profiles over a single day (12:12 h
light/dark cycle) for N. oculata in linear growth phase; both profiles show
evidence of carbon limitation that occurs towards the end of the light cycle.
Spikes in [O2] were used for oxygen evolution measurements (see Figure 3).
d½O2
dt
ð2Þ
¼PR
solution : ½O2 ¼ ðP RÞt þ ½O2 de
ð3Þ
Net photosynthesis (PR) is, therefore, equal to the gradient
(Figure 2 a). This [O2] minimum is slightly lower than the [O2] of
of the linear increase in [O2]. Once gas exchange is turned
seawater in equilibrium with air (221 mmol L1 at 20 8C), calcuback on, Equation (1) can now be solved because the start
lated from Henry’s Law[32] because of the consumption of
point [O2] and the end point [O2]eq are both known [Eq. (4)]:
oxygen by N. oculata cells by dark respiration. If the light is
turned on, photosynthetic O2 production starts up within
ð4Þ
solution : ½O2 ¼ D½O2 ekL a t þ ½O2 de
a matter of minutes, and [O2] reaches its maximum of
252 mmol L1 within the first hour (phase A). At this point, [O2]
The decrease in [O2] is described as an exponential function,
reflects the maximum rate of photosynthesis achievable
and the gas exchange coefficient (kLa) determines the half-life
through the steady-state acclimation of N. oculata to the averof this exponential decay.[26] The gas exchange coefficient is
age photon availability within the PBR, if we assume
replete nitrate and phosphate concentrations (approximately 300 mg L1 of nitrate and 40 mg L1 of
phosphate). Following this steady-state maximum,
[O2] begins to decrease (phase B) and approaches
a new plateau of 236 mmol L1, the “terminal [O2]”,
near the end of the light cycle (phase C). This decrease in [O2] may be attributed to a decrease in the
rate of photosynthesis and/or an increase in the rate
of respiration over the light cycle. As the light intensity does not change, this behaviour indicates either
the presence of nutrient limitation or photo-inhibition. If the light is turned off, [O2] returns quickly to
its dark cycle minimum of 218 mmol L1.
The pH is at its minimum value of 8.0 at the end of
the dark cycle (Figure 2 b). This is lower than the
equilibrium pH of 8.2 because of CO2 production by
dark respiration during the dark cycle. The pH increase during the light cycle (phases A, B and C) is an
indication of photosynthetic carbon consumption by Figure 3. A typical spike in the [O2] profile, which was used to calculate the net photoN. oculata cells. Notably, the pH response is signifi- synthesis (PR) and the gas exchange coefficient (kLa) at a specific point in time.
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strongly dependent on temperature, pressure, salinity and
bubble size,[30] but these are all assumed to be constant
throughout the experiment. Once kLa is known, it is possible
to calculate (PR) directly from the [O2] profile without performing a spike by using the expected dissolved oxygen concentration calculated from Henry’s Law ([O2]eq) and considering
Fick’s Law solution under steady-state conditions [Eq. (5)]:
solution : ½O2 de ¼ ½O2 eq þ
PR
kL a
based system. Net photosynthesis (PR) is at its steady-state
maximum of 125 mmolO2 L1 h1 &&at the start of the light
cycle&& and decreases to the terminal rate of 50 mmolO2 L1 h1 by the end of the light cycle. This corresponds to
a 60 % decrease in net photosynthesis by the end of the light
cycle, or a ~ 30 % decrease in net productivity.
pH as a measure of carbon availability
ð5Þ
As outlined in the Introduction (Figure 1), dissolved CO2 increases the concentration of HCO3 ions and decreases the
concentration of CO32 ions in seawater; pH can be used as an
indirect measure of carbon availability in a PBR.[47] The increase
in pH over the light cycle (Figure 2 b) can be attributed to the
removal of dissolved inorganic carbon (DIC) by N. oculata cells,
which shifts the equilibrium of the carbonate system. Dissolved
CO2 molecules have little direct influence on N. oculata photosynthesis as bicarbonate dominates the extracellular carbon
pool (Figure 5) and is also the inorganic carbon species taken
up by the CCM. At the minimum pH of 8.0, the bicarbonate
pool is almost full at ~ 2500 mmol L1, whereas at the maximum
pH of 9.5, the bicarbonate concentration is reduced to
~ 300 mmol L1 and carbonate is the dominant carbon species
(Figure 5). The pH of the medium normally increases with time
if algae are grown with nitrate because of the excretion of
OH anions,[37, 48] but this does not occur here as the pH returns
to the same dark cycle minimum after 24 h. This is consistent
with the fact that N. oculata uses an acid–base regulation
mechanism to synthesise organic acids to neutralise excess
OH and store the resulting organic anion salts in vacuoles.[49]
N. oculata cells, like most algae, cannot use carbonate as
a carbon source.[14, 25] As bicarbonate is used up and becomes
a limiting resource, so the rate of pH increase decreases.
N. oculata cells find it more difficult to obtain carbon, and the
rate of photosynthesis decreases consequently
(Figure 4). The pH maximum plateau at the end of
the light cycle (Figure 2 b), therefore, represents the
point at which the carbon-limited rate of photosynthesis matches the input of carbon from gas exchange. The reduced afternoon [O2] terminal corresponds to the equilibrium between the rate at which
carbon is removed from solution by photosynthesis
and the rate at which carbon is added to solution by
gas exchange (bubbling). This equilibrium will
depend on the factors that affect both photosynthesis (light level, cell number, temperature, nutrient
levels) and gas exchange (gas bubbling rate, CO2
concentration, bubble size, gas residence time).[5, 47]
Equations (3)–(5) were fitted to the [O2] measurements
before bubbling was interrupted [Eq. (5)], during the interruption [Eq.( 3)] and after [Eq. (4)] using the least squares fitting
procedure in gnuplot.
A more precise way to calculate net photosynthesis is to
remove the complication of gas exchange by measuring [O2]
in a traditional cuvette-based respirometer setup.[44, 45] By using
this system, a 2 mL culture sample was extracted from the
PBR, dark-adapted for 10 min and the oxygen production rate
was measured by performing a rapid light curve over five irradiances. The use of a sealed cuvette ensures that photosynthesis rate measurements are free of interference from atmospheric gas exchange. However, it is difficult to relate the light field
that cells experience in the PBR to the light field in the respirometer cuvette. Other bulk properties, such as mixing, will also
be different. For these reasons, the rate of photosynthesis
measured in the PBR and cuvette are not compared directly,
and different ordinate scales are used in Figure 4.
A similar diurnal pattern is observed in the PBRs and in the
respirometer setup, which implies that [O2] can be used with
confidence as proxy for net photosynthesis provided that the
gas exchange is controlled and stable[46] (Figure 4). Dark respiration (R) measurements of 20 mmolO2 L1 h1 are consistent
across the diurnal cycle in the PBR and against the cuvette-
Mechanism
Figure 4. A comparison between different types of photosynthesis rate measurements
and calculations over two days of PBR operation: red pluses, calculated using [O2] spikes;
red line, calculated directly from [O2] profile using Fick’s Law &&which one?&& and
assuming constant gas exchange; blue dots (in the light) and blue squares (in the dark),
measured using the cuvette-based respirometer setup.
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The asymptotic diurnal [O2] trend cannot be attributed to photo-inhibition as the light availability in a culture decreases monotonically with age; hence photoinhibition is more likely in dilute cultures at early
stages of growth. Therefore, this afternoon decrease
in photosynthesis is likely caused by a resource limi 0000 Wiley-VCH Verlag GmbH & Co. KGaA, Weinheim
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conversion of CO2 plus hydroxyl ions and bicarbonate in the
culture,[50] as well as internal buffering by N. oculata cells
caused by fluxes of the pH-influencing species across the cell
plasmalemma.[29, 49]
The extracellular carbon pool continues to empty over
a timescale of hours, and the inflection in the pH rise indicates
that bicarbonate ions are starting to become limiting. This limitation results in a reduction in the photosynthesis rate
(phase B).
Finally, near the end of the light period, the extracellular
carbon pool is almost empty of bicarbonate ions and photosynthesis becomes fully carbon limited (phase C). Photosynthesis is maintained at a new equilibrium between carbon
demand and the delivery of additional usable carbon by gas
exchange. Gas exchange, therefore, controls the degree of
carbon limitation experienced by the algal culture as the light
cycle progresses.[51]
At the beginning of the dark cycle, photosynthesis is immediately switched off, and [O2] rapidly returns to its dark minimum (phase D). The pH gradually returns to its minimum
value during the dark cycle as the extracellular carbon pool is
refilled slowly by CO2 delivered by gas exchange and dark respiration (phase E). This process continues as long as the N. oculata culture remains in the exponential growth phase and no
additional nutrient limitation is present.[9]
It has been shown that photo-respiration increases linearly
with [O2] at O2 saturation levels greater than 75 %
(165 mmol L1 at 20 8C and salinity of 33&&unit?&&), which
is within the range of this experiment.[52] The initial (phase A)
increase of [O2] from 218 to 252 mmol L1, therefore, increases
photo-respiration by ~ 16 %. This increase in photo-respiration
likely triggers the initial decrease in [O2] (phase B), which provides another explanation for the quick [O2] response compared to the pH response. Following on from phase A, the
photo-respiration rate stabilises and any further decreases in
[O2] may be attributed directly to carbon limitation.
Figure 5. Carbonate chemistry of seawater shows a predominance of bicarbonate at the equilibrium pH of 8.2. Consumption of bicarbonate and influx
of protons and/or efflux of hydroxyl ions by photosynthesis is faster than inorganic carbon is resupplied as CO2 from the gas stream, which causes a decrease in total inorganic carbon; CO2 and bicarbonate decrease, whereas carbonate and pH increase. The inorganic carbon pool is refilled during the
night as part of the diurnal cycle. Phases A–E correspond to the classification
in Figure 2.
tation. In these batch cultures, the total concentration of inorganic nutrients, such as phosphorous and nitrogen, also decreases monotonically and could not be responsible for the diurnal pattern. This leaves DIC as the most likely candidate for
resource limitation. The concentration of DIC and O2 in a culture vessel are determined by gas exchange. It is now possible
to propose a mechanism for the carbon limitation of N. oculata
in PBRs (Figure 6).
At the end of the dark cycle, [O2] and pH are both at their
minimum levels (phase E). Dissolved O2 and CO2 are in equilibrium with the air supply, and the gas exchange system is in
a steady state. The extracellular DIC pool, which contains carbonate and bicarbonate ions, is at its highest level in the light/
dark cycle and the proton concentration is high. A small
amount of O2 is used up by dark respiration at a constant rate.
Once the light is turned on, photosynthesis is activated rapidly and the steady-state [O2] maximum is attained (phase A).
At this point, net photosynthesis is limited only by photon
availability.[38] Some O2 is used up by dark respiration and
photo-respiration, but the majority of O2 departs the system
by gas exchange as the O2 concentration is now significantly
higher than that under air equilibrium. The carbon pool begins
to decrease slowly as N. oculata cells take up bicarbonate ions,
the conversion of which to CO2 supplies photosynthesis and
limits photo-respiration.[16] As the carbon pool is large relative
to the oxygen pool, the pH response is significantly slower
than the [O2] response. The slow pH response also reflects the
buffering capacity of seawater and the slow uncatalysed interChemSusChem 0000, 00, 0 – 0
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Confirmation
To further verify whether carbon really limits N. oculata growth,
additional CO2 was introduced into the PBR and the [O2] and
pH profiles were measured. The results are shown in Figures 7
and 8.
The initial proof-of-concept experiment involved a single
CO2 injection (Figure 7). The control PBR displays the typical diurnal [O2] and pH variation over a four-day cycle (Figure 7 a).
The second PBR follows the same pattern until CO2 is injected
at the presumed carbon-limited period (before the end of
phase C) on day 8 of the experiment, and the light cycle
changed from a diel pattern to continuous illumination. If the
N. oculata cells are carbon limited, the addition of more carbon
should increase the rate of photosynthesis. Alternatively, if the
cells are photo-inhibited, additional CO2 should have a negligible effect.[16]
This large CO2 injection, 12 min in duration, saturated the
extracellular carbon pool rapidly back to its pre-dawn maximum, as evidenced by a rapid decrease in the pH (Figure 7 b).
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Figure 6. Mechanism for carbon limitation of N. oculata in a PBR. Changes in arrow thickness indicate changes in the rate of photosynthesis, respiration and
gas exchange. Changes in the red and white ovals indicate changes in extracellular DIC and proton (H+) pool sizes respectively.
At the same time, [O2] returned to its maximum value, which
indicates that steady-state photosynthesis is possible in
a carbon-replete system at any point during the light cycle.
Following CO2 addition, the light cycle was extended for an additional 10 h (Figure 7 b). Over this time, the [O2] reduction corresponded directly to carbon pool depletion (increased pH)
with no evidence of photo-inhibition, circadian cycles or any
other light-related effects.
A second experiment was performed to determine whether
[O2] could be maintained at its carbon-replete maximum by
periodic CO2 injection (Figure 8). In the control PBR, the typical
diurnal carbon limitation pattern was observed over a period
of five days (Figure 8 a). In the second PBR, a brief CO2 injection
of 10 s in duration was applied whenever [O2] began to fall beneath the light-limited maximum (Figure 8 b). The maximum
daily [O2] was maintained across five consecutive light cycles
by applying a set of 5–8 such CO2 injections to maintain
a carbon-replete environment.
One way to ensure that the PBR remains carbon replete is to
operate the PBR as a pH-stat at the night cycle minimum pH
ChemSusChem 0000, 00, 0 – 0
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of 8.0. There are two disadvantages to this approach: 1) the
pH response time from the carbonate chemistry is slow, especially in the absence of external carbonic anhydrase in Nannochloropsis spp., and 2) carbonate chemistry is complex and pH
is only a proxy for carbon availability. Salinity and dissolved nutrient concentrations play a significant role to determine the
relationship between carbonate chemistry and pH.[29] In a pHstat system, the control parameter is separated by numerous
chemical and metabolic steps from the desired algal physiological response, that is, maximum photosynthesis rate. pH is one
of many inputs of photosynthesis, which include irradiance,
temperature, inorganic nutrient availability and cell density. A
more precise control system could instead utilise [O2], which is
a direct output of photosynthesis. An example of one such
“[O2]-stat” system in operation is given in Figure 8. As the [O2]
response is more dynamic and faster, it would result in more
efficient CO2 delivery, but it will carry additional challenges in
maintaining a steady equilibrium.
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Figure 7. Effects of a single CO2 injection on diurnal [O2] and pH profiles. a) The control experiment shows consistent [O2] and pH profiles over a four-day period. b) A single, large CO2 injection at terminal [O2] on day 8 of the
experiment fills up the carbon pool and returns [O2] back to its steady-state maximum, which effectively replicates
DIC replenishment during a night cycle.
thesis was limited by the depletion of usable carbon, or more
specifically bicarbonate ions, in
the system. A mechanism that
involves photosynthesis, respiration and carbonate chemistry
can explain this phenomenon.
The addition of CO2 was used to
recover the steady-state maximum photosynthesis rate and,
therefore, prove that N. oculata
cells were carbon limited under
the environmental conditions
provided by the photo-bioreactor. This ability to identify and
analyse carbon limitation is of
critical importance to both experimental design and commercial algal biomass production.
The dissolved oxygen concentration [O2] proved to be an effective proxy for photosynthesis
rate. In future, a feedback loop
will be used to maintain [O2] at
its maximum level by gradually
increasing the CO2 concentration
in the gas bubbling mix across
the light cycle. This approach
would alleviate carbon limitation
and maximise photosynthesis,
which would also maximise
N. oculata biomass production in
the absence of other limiting
factors, such as nitrogen or
phosphorus depletion. As the
CO2 molar fraction of the gas
phase and the gas exchange coefficient are both known, it will
also be possible to calculate the
CO2 sequestration rate by N. oculata cells. Once set up, this
system could be applied to any
photo-bioreactor geometry or
indeed to any algal species.
Experimental Section
Figure 8. The use of periodic CO2 injections to maintain [O2] at its carbon-replete maximum throughout the light
cycle. Algae are increasingly carbon limited across the light cycle in a) the control experiment, whereas a higher
rate of net photosynthesis could be consistently maintained with b) periodic CO2 injection across five consecutive
light cycles.
The microalga Nannochloropsis
oculata (Droop) Green (Australian
National Algae Culture Collection;
strain CS-179) was used. Taxonomically, N. oculata is in the class Eustigmatophyceae of the phylum Heterokontophyta. N. oculata was
grown in f/2 seawater medium: artificial seawater (salinity 33) enriched with 54.7 mg L1 NO3, 4.5 mg L1 PO4 and micronutrients.
Stock cultures were maintained in 200 mL Erlenmeyer flasks at
Conclusions
The green alga N. oculata was cultured in an environmental
photo-bioreactor, and a significant reduction in the rate of
photosynthesis was observed during the light cycle. PhotosynChemSusChem 0000, 00, 0 – 0
www.chemsuschem.org
Algae and stock culture
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20 8C under cool-white fluorescent light with an irradiance of (50
5) &&mmolphoton m2 s1&& and a 12:12 h light/dark cycle in an
incubator (Labec Temperature Cycling Chamber incubator, Labec
Pty Ltd, Australia). Cultures were diluted seven days before the experiment to ensure that N. oculata cells were in the exponential
growth phase. PBRs were inoculated with a 1:10 v/v algal dilution
in f/2 to give a starting concentration of approximately
106 cells mL1.
10 min before the experiment. The temperature was controlled at
20 8C in an optical cuvette holder (ED-101US/MD, Heinz Walz
GmbH, Effeltrich, Germany) with integrated magnetic stirring.
White actinic light was provided by the multi-colour pulse-amplitude-modulated fluorometer (MC PAM; Heinz Walz GmbH, Effeltrich, Germany). A [O2] fixed needle-type minisensor probe with
optical isolation (OXF1100-OI; PyroScience, Aachen, Germany) was
used to measure photosynthesis and respiration rates.
PBRs
Oxygen production
Experiments were performed in environmental photo-bioreactors
(ePBR, Phenometrics, Lensing, MI, USA) with an inverted conical
frustum geometry and a working volume of 500 mL.[38] Two simultaneous ePBR experimental replicates were used. The algae were
mixed by magnetic stirring. The temperature was maintained at
20 8C using a Peltier heater-cooler connected to a water jacket.
Cool-white LED illumination was delivered from above; the path
length through the algal culture was 20 cm. The algae were illuminated with a photon flux density of 500 mmolphoton m2 s1 over
a 12:12 h light/dark cycle during a six-day adaptation period. Once
acclimation was complete, that is, once N. oculata cells had
reached the exponential growth phase, irradiance was increased to
2000 mmolphoton m2 s1 (12:12 h light/dark cycle), which corresponds to the day-time maximum irradiance at outdoor culturing
facilities. Air bubbling was also turned on at this time. Oil-free laboratory air was humidified by passing it through distilled water
after which it was filtered through a 0.2 mm filter and then delivered through a 0.45 mm sterile needle placed near the bottom of
the ePBR vessel.
Oxygen production was measured several times per day in the
ePBR. The air supply was turned off for approximately 15 min to
measure the rate of oxygen production (modelled by a linear increase) associated with net photosynthesis. Once the air supply
was turned back on, the oxygen concentration returned to its
baseline as a result of gas exchange (modelled by an exponential
decay). Rapid light curves were used to measure oxygen production in the cuvette. Five consecutive illumination steps were used:
44 mmolphoton m2 s1 for 8 min; 122 mmolphoton m2 s1 for 4 min;
258 mmolphoton m2 s1 for 2 min; 499 mmolphoton m2 s1 for 2 min;
831 mmolphoton m2 s1 for 2 min.
Carbon addition
Two mass flow controllers were used to mix pure CO2 at a flow
rate of 20 mL min1 with air at a flow rate of 70 mL min1 to give
a CO2 molar gas fraction of 22.3 %. This CO2 was delivered into one
of the ePBRs at the end of the light cycle on day 10 of the experiment (Figure 7). It was delivered over a period of 12 min through
an additional humidified gas line with a 0.45 mm sterile needle. In
a second experiment, CO2 was instead delivered periodically at
10 s intervals (Figure 8). A solenoid valve was used to control CO2
injection.
Continuous [O2] and pH measurements
Dissolved oxygen [O2] was measured by using a 3 mm robust [O2]
optical probe with optical isolation (OXROB10-OI-CL4; PyroScience,
Aachen, Germany). A two-point [O2] calibration against air-saturated and nitrogen-saturated seawater was performed. A prototype
pH optical probe with optical isolation (PyroScience, Aachen, Germany) was used to measure pH; it was calibrated by titration with
NaOH and HCl, and the pH response was linear within the pH
region of interest.
Acknowledgements
The authors would like to thank Dr Milan Szab for his scientific
input and PyroScience GmbH for giving us access to their prototype pH optodes.
Automated cell counts
Keywords: biomass · carbon dioxide fixation · kinetics ·
photosynthesis · renewable resources
Samples (1 mL) were extracted daily from each ePBR, fixed with
1 % glutaraldehyde and stored in the dark at 5 8C. A 10 mL aliquot
was pipetted into a haemocytometer (Neubauer, Germany) and
placed under a compound microscope (BX50 with analySIS software, Olympus, Victoria, Australia) at 20 magnification. The cells
were left to settle for 5 min before 15–30 images of different haemocytometer squares were recorded. A custom ImageJ script was
used to scan the resulting JPEG files through format changes to
quantify the cell density and size distribution. The software was
able to distinguish between N. oculata cells, cell detritus, dust and
air bubbles.
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Received: March 5, 2015
Revised: June 22, 2015
Published online on && &&, 0000
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FULL PAPERS
B. Tamburic,* C. R. Evenhuis, D. J. Suggett,
A. W. D. Larkum, J. A. Raven, P. J. Ralph
Just grow it: We present the first indepth analysis of CO2 limitation on biomass productivity of the marine microalga Nannochloropsis oculata. Net photosynthesis decreases by 60 % over a 12 h
light cycle as a direct result of carbon
limitation. Continuous dissolved O2 and
pH measurements are used to develop
a detailed diurnal mechanism for the interaction between photosynthesis, gas
exchange and carbonate chemistry in
the photo-bioreactor.&&ok? text and
graphics were missing.&&Tamburic et
al. study CO2 limitation on #biomass
productivity in a #photobioreactor
ChemSusChem 0000, 00, 0 – 0
www.chemsuschem.org
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&& – &&
Gas Transfer Controls Carbon
Limitation During Biomass Production
by Marine Algae
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