Phototrophic cultivation of Chlorella vulgaris in the BioLector XT microbioreactor


Modern bioprocess engineering techniques have enabled scientists to explore the potential of microalgae for the production of energy and valuable compounds1. The recent rise of interest in algae biotechnology has led to significant advancements in the use of microalgae for biofuel production, carbon dioxide sequestration and environmental bioremediation, and revealed algae’s great potential as a source of biomass, food, nutraceuticals and pharmaceuticals2.

Moreover, the use of algae as microbial cell factories provides answers to some of the most urgent global challenges like the food and energy crisis3, and will boost the transition to a sustainable bioeconomy4. Microalgae value chains are potentially profitable and competitive at industrial scale, but biorefineries need to be adapted according to biological potential, process routes and market needs5, 6.

Improved culture conditions, strain screening and strain engineering are critical steps to commercialization7, for example by maximizing the solar-to-product energy conversion efficiency by truncating the chlorophyll antenna size8. Microwell based culture devices provide a powerful tool for rapid and early-stage screening for microbial and mammalian cells9 and have already been used for heterotrophic microalgae bioprocess development10.

Microphotobioreactor (μPBR) systems are needed to investigate optimal auto- or mixotrophic cultivation conditions, but current concepts are far from series technology and further improvement – especially on adjustable illumination – is essential11, 12.

For this Application Note, the BioLector XT microbioreactor is equipped with a sophisticated illumination module to enable parallel, phototrophic cultivations in up to 48 microwells, and specialized filter modules were designed to allow for the online, non-invasive measurement of important cultivation parameters like biomass, chlorophyll concentration and pH. The illumination module or Light Array Module (LAM) allows for precise and diverse lighting regimes within relevant photosynthetic spectra. The spectral flexibility is achieved by a total of 16 different LED-types, which can each be controlled individually, delivering maximum irradiances near 4000 μmol/m2/s.

biolector microbioreactor with lam module

Figure 1. The BioLector XT microbioreactor with the LAM.

Chlorella vulgaris can grow phototrophic, heterotrophic and mixotrophic13 and is one of the dominant microalgae genera on the market, with about 5000 tons of biomass produced per year14. C. vulgaris shows high growth rates under versatile cultivating conditions and numerous studies have revealed many applications for biochemical components produced by C. vulgaris15. Its high protein content – with an amino acid profile comparing well to values suggested by the World Health Organisation (WHO) for human nutrition – along with the presence of essential nutrients has led to various applications in the food and feed industry15. Moreover, the accumulation of C16 and C18 fatty acids under unfavourable growth conditions16, 17 presents possibilities to produce biofuels in wastewater treatment plants15.

Chlorella vulgaris

Figure 2. Chlorella vulgaris grown photoautotrophically in the BioLector XT microbioreactor.

In this AppNote we show that the BioLector XT microbioreactor – equipped with LAM – is suited for the photoautotrophic cultivation of C. vulgaris. Furthermore, several filter modules were designed and validated to monitor crucial cultivation parameters online.


Development of filter modules

Several filter modules were designed and tested for online monitoring of important phototrophic cultivation parameters.

Biomass: For biomass determination with scattered light18, filter modules were developed outside of the chlorophyll absorbance spectrum (>700 nm) to avoid pigment interference19. These filter modules were calibrated against a dilution series of C. vulgaris.

Chlorophyll content: Chlorophyll fluorescence was used to quantify chlorophyll concentrations online. To that end, chlorophyll a and b standards (Sigma-Aldrich) were dissolved in DMSO and several filter modules were tested against chlorophyll a and b dilution series. Furthermore, a calibration of chlorophyll fluorescence against biomass was performed.

pH: The pH measurement with optodes20 cannot be used under continuous illumination due to the optodes’ susceptibility for photobleaching. As an alternative, the soluble fluorescent pH-indicator 8-hydroxypyrene-1,3,6-trisulfonic acid trisodium salt (HPTS) can be used for optical pH determination21, 22. For this approach, two modules were designed which need to be installed simultaneously due to the ratiometric nature of the pH-determination via HPTS.

At an emission wavelength of 520 nm, HPTS has pH-dependent fluorescence intensities at excitation wavelengths of 405 and 455 nm, respectively. The intensity ratio IR (Eq. 1) is stable in the pH 0 to 14 range21 but pH-values cannot be calculated without prior calibration22. Fitting calibration results to the Boltzmann equation allows the calculation of calibration parameters pH0, dpH, IR,min and IR,max (Eq. 2)23.

Boltzmann equation biolector 

With the designed filter modules, calibration curves were made to evaluate the potential of pH determination via HPTS in the BioLector XT microbioreactor. Furthermore, the susceptibility of this method against photobleaching was tested under typical phototrophic cultivation conditions.

Chlorella vulgaris

Axenic Chlorella vulgaris was obtained from the Culture Collection of Algae at the University of Göttingen (SAG Strain Number 211-11b).

Culture medium

Cultures were grown in an adapted recipe of the enriched Bold’s Basal Medium (enBBM), at a pH value of 6.524-27.

The medium consisted of 9.76 g/L MES buffer, 1.5 g/L NaNO3, 0.6 g/L K2HPO4, 1.4 g/L KH2PO4, 187.5 mg/L MgSO4 · 7 H2O, 6.25 mg/L NaCl, 125 mg/L CaCl2 · 2 H2O, 9.96 mg/L FeSO4 · 7 H2O, 3.68 H2SO4, 100 mg/L Na2EDTA · 2 H2O, 62 mg/L KOH, 10 mg/L sodium penicillin-G and 20 mL/L trace element solution.

The trace element solution had the following composition: 17,64 mg/L ZnSO4 · 7 H2O, 2.88 mg/L MnCl2 · 4 H2O, 2.4 mg/L Na2MoO4 · 2 H2O, 3.14 mg/L CuSO4 · 5 H2O, 0.94 mg/L CoSO4 · 7 H2O and 22.8 mg/L H3BO3.

For cultivations in the BioLector XT microbioreactor a HPTS stock solution was added to the medium to a final concentration of 0.1 mg/L HPTS.

Cultivation in shake flasks

Precultures were cultivated in shake flasks in an incubator at 25 °C at 180 rpm with a shaking diameter of 50 mm. To allow for phototrophic growth, an LED-module was installed to one of the sides of the incubation chamber and cotton plugs were used to allow the transfer of gases to and from the culture broth. The LED-module held eight sun-like LED-Strips (LUMITRONIX LED-Technik GmbH) in parallel setup. The irradiance was set at 200 μmol/m2/s to match the irradiance during cultivation in the BioLector XT microbioreactor.

Cultivation in the BioLector XT microbioreactor

Phototrophic cultivation was performed in Flowerplate microtiter plates (M2P-MTP-48-B, m2p-labs (now part of Beckman Coulter Life Sciences)28) with an initial cell concentration of 5.5*10^6 cells/mL and 1 mL filling volume. The microtiter plate was sealed with gas permeable sealing foil (MTP-F-GPRS-48-10) to allow the exchange of carbon dioxide and oxygen during photosynthesis. The illumination module was set to deliver a sunlike spectrum from 400 to 700 nm at a photon flux density of circa 200 μmol/m2/s (Figure 3).

Illumination spectrum and irradiance
Figure 3. Illumination spectrum and irradiance set during cultivation.

Cultivation parameters were set at 800 rpm, 25 °C and 85 % relative humidity and gassing was performed at a 10 mL/min flowrate with a mixture of air and 2 % CO2.


Calibration of filter modules

Biomass: The developed biomass filters at 730, 750 and 850 nm showed excellent calibration results in a range 0.3 ≤ OD750 ≤ 25, as demonstrated in Figure 3 for the 730 nm module. Furthermore, no chlorophyll interference was detected against chlorophyll a and b standards.

Calibration of a 730 nm scattered light filter module
Figure 4. Calibration of a 730 nm scattered light filter module against a C. vulgaris dilution series. 

Chlorophyll content: The chlorophyll calibration results revealed that the designed filter modules allowed the separate and simultaneous detection of chlorophyll a and b (Figure 5).

Chlorophyll concentration
Figure 5. Calibration of the chlorophyll fluorescence filter modules against dilution series of chlorophyll a (black) and chlorophyll b (red).

Chlorophyll fluorescence is often used for biomass determination for phototrophic cultures29, 30. Accordingly, a calibration with a diluted biomass series was performed and an excellent resolution at low biomass concentrations was observed when an exponentially decreasing fit was applied (Figure 6).

Calibration of the chlorophyll filter module
Figure 6.
Calibration of the chlorophyll filter module (λex = 450 nm; λem = 700 nm) against biomass up to OD750 = 2. 

The calibration results confirm the applicability of chlorophyll fluorescence filters to accurately determine biomass concentrations, especially at low biomass concentrations.

pH: The pH filter modules were calibrated at 25, 30, 35 and 40 °C with buffer solutions from pH 5 to 10 (Merck, Darmstadt, DE), containing 0.1 mg/L HPTS. The excellent calibration results (Figure 7) confirm that the proposed setup can be used for accurate, online pH determination.

Calibration of intensity ratio
Figure 7.
Calibration of intensity ratio IR against pH, fitted to the Boltzmann equation. 

To ensure the insensitivity of the proposed method towards photobleaching, an experiment was run in the BioLector XT microbioreactor under typical cultivation conditions at 200 μmol/m2/s in enBBM without inoculum (Figure 8).

Optical pH determination with HPTS
Figure 8.
Optical pH determination with HPTS in triplicate wells under cultivation conditions. 

The increased CO2-concentration quickly acidifies the medium (~0.05 pH) at the start of the experiment, but afterwards the measured values remain constant for at least 130 hours (Figure 8). This proves that a multiple-day, accurate and stable pH determination under cultivation conditions and especially under continuous illumination is possible with HPTS.

Parallel phototrophic cultivation in the BioLector XT microbioreactor

Next, a long-term cultivation was started and online monitored with four of the presented filter modules: the scattered light module at 730 nm, the chlorophyll fluorescence filter module (λex = 450 nm; λem = 700 nm) and both HPTS filter modules for the ratiometric pH determination (Figure 9).

Scattered light chlorophyll and pH
Figure 9.
Scattered light, chlorophyll, and pH during a 16-day cultivation in the BioLector XT microbioreactor in combination with an
illumination module. 

Figure 9 shows a continuously increasing biomass concentration for approximately 16 days until the CO2 supply was shut off. Five distinct growth phases are seen: starting with a lag and exponential growth phase (I.), followed by three distinctive linear growth rates (II. to IV.) and a death phase (V.) after CO2 depletion. The course of the pH and chlorophyll signal correlate to the observed growth phases. The scattered light signal’s mean coefficient of variation throughout the experiment is 5.2 %, allowing for parallel phototrophic cultivations in the proposed setup. Offline samples confirmed the accuracy of the online signals. Sampling after 235 hours – where an increased pH is seen due to a brief exposure to the atmospheric CO2-concentration – resulted in offline OD750 values of 40 and an offline pH of 7.3, correlating well to the online determined pH of 7.2. At the end of the experiment, offline OD750 values were around 60, indicating a strong growth during the experiment, leading to high biomass concentrations.


The addition of the Light Array Module has broken new ground for the BioLector instruments. This application note presents several filter modules that can accurately monitor the crucial phototrophic cultivation parameters biomass concentration, chlorophyll content and pH.

The excellent resolution for biomass determination at low concentrations seen with the chlorophyll fluorescence filter module complements the scattered light measurement which are most accurate at sufficiently high cell densities18. Moreover, the HPTS-based pH determination has shown to be an excellent alternative for optode measurements, even under continuous illumination.

The long-term cultivation with Chlorella vulgaris confirmed the system’s potential as a parallel, high-throughput photobioreactor in microliter scale. Furthermore, the developed filter modules delivered online information about the cultures’ growth and revealed several distinct growth phases. These results provide a platform that can be used to optimize phototrophic cultivations in several ways and for many applications. The design of the illumination module allows for a wide spectral and irradiance range to be set under different illumination regimes, which could be used to find optimal illumination conditions. These illumination characteristics have widely been reported to influence algae growth12, 31-35.

Gassing flow rates and gas composition can be used to change the experiment’s atmosphere in the BioLector XT microbioreactor, which is an important parameter in phototrophic cultivations as, e.g., enrichment with CO2 leads to higher biomass concentrations15, 33. Other important factors influencing microalgae cultivations are temperature36, 37, pH15, 34, salinity38, carbon source39-41, nitrogen source33, 39 and medium composition42. The BioLector XT system allows for the optimization of all these parameters.

Furthermore, fed-batch cultivation has been proposed to improve lipid productivity43. The potential of genetically engineering algae strains has only been researched and applied scarcely due to regulatory restrictions, but could result in higher growth rates and cell densities, increased production rate or titer, enhanced robustness or higher solar-to-biomass conversion efficiency and photosynthetic productivity1, 8, 44, 45.

All these factors could be researched and optimized using the proposed combination of a BioLector XT microbioreactor and the LAM, accelerating research to provide the answers required to help realize algae’s potential.


  1. Hallmann, A., Algae biotechnology–green cell-factories on the rise. Current Biotechnology, 2015. 4(4): p. 389-415.
  2. Tripathi, B.N. and D. Kumar, Prospects and challenges in algal biotechnology. 2017: Springer Singapore.
  3. United Nations, Transforming our World: The 2030 Agenda for Sustainable Development. 2015.
  4. Dos Santos Fernandes de Araujo, R., et al., Brief on algae biomass production. 2019.
  5. Slegers, P.M., et al., Design of Value Chains for Microalgal Biorefinery at Industrial Scale: Process Integration and Techno-Economic Analysis. Frontiers in Bioengineering and Biotechnology, 2020. 8.
  6. Hariskos, I. and C. Posten, Biorefinery of microalgae - opportunities and constraints for different production scenarios. Biotechnology Journal, 2014. 9(6): p. 739-752.
  7. Chisti, Y., Constraints to commercialization of algal fuels. Journal of biotechnology, 2013. 167(3): p. 201-214.
  8. Melis, A., Solar energy conversion efficiencies in photosynthesis: minimizing the chlorophyll antennae to maximize efficiency. Plant science, 2009. 177(4): p. 272-280.
  9. Ojo, E.O., et al., Design and parallelisation of a miniature photobioreactor platform for microalgal culture evaluation and optimisation. Biochemical Engineering Journal, 2015. 103: p. 93-102. 
  10. Hillig, F., et al., Bioprocess Development in Single-Use Systems for Heterotrophic Marine Microalgae. Chemie Ingenieur Technik, 2013. 85(1-2): p. 153-161.
  11. Morschett, H., et al., Laboratory-scale photobiotechnology-current trends and future perspectives. FEMS Microbiol Lett, 2018. 365(1).
  12. Kiss, B. and Á. Németh, High-throughput microalgae cultivation with adjustable LED-module applying different colours for Nannochloropsis and Chlorella microcultures. Acta Alimentaria, 2019. 48(1): p. 115-124.
  13. Safi, C., et al., Morphology, composition, production, processing and applications of Chlorella vulgaris: A review. Renewable and Sustainable Energy Reviews, 2014. 35: p. 265-278.
  14. Levasseur, W., P. Perré, and V. Pozzobon, A review of high value-added molecules production by microalgae in light of the classification. Biotechnology Advances, 2020. 41: p. 107545.
  15. Ru, I.T.K., et al., Chlorella vulgaris: a perspective on its potential for combining high biomass with high value bioproducts. Applied Phycology, 2020. 1(1): p. 2-11.
  16. Yeh, K.-L. and J.-S. Chang, Effects of cultivation conditions and media composition on cell growth and lipid productivity of indigenous microalga Chlorella vulgaris ESP-31. Bioresource technology, 2012. 105: p. 120-127.
  17. Maruyama, I., et al., Application of unicellular algae Chlorella vulgaris for the mass-culture of marine rotifer Brachionus, in Live Food in Aquaculture. 1997, Springer. p. 133-138.
  18. m2p-labs GmbH, Baesweiler Germany, The scattered light signal: Calibration of biomass. 2015.
  19. Griffiths, M.J., et al., Interference by pigment in the estimation of microalgal biomass concentration by optical density. Journal of microbiological methods, 2011. 85(2): p. 119-123.
  20. m2p-labs GmbH, Baesweiler Germany, Mode of operation of optical sensors for dissolved oxygen and pH value. 2013.
  21. Wolfbeis, O.S., et al., Fluorimetric analysis. Fresenius’ Zeitschrift für analytische Chemie, 1983. 314(2): p. 119-124.
  22. Kensy, F., et al., Validation of a high-throughput fermentation system based on online monitoring of biomass and fluorescence in continuously shaken microtiter plates. Microbial Cell Factories, 2009. 8(1): p. 31.
  23. Schulte, A., et al., A novel fluorescent pH probe for expression in plants. Plant Methods, 2006. 2: p. 7.
  24. Bischoff, H.W. and H.C. Bold, Some soil algae from Enchanted Rock and related algal species. 1963, Austin, Tex.: University of Texas.
  25. Bold, H.C., The Morphology of Chlamydomonas chlamydogama, Sp. Nov. Bulletin of the Torrey Botanical Club, 1949. 76(2): p. 101-108.
  26. Andersen, R.A., Algal culturing techniques. 2005, Burlington, Mass.: Elsevier/Academic Press.
  27. Morschett, H., W. Wiechert, and M. Oldiges, Accelerated Development of Phototrophic Bioprocesses: A Conceptual Framework. 2017, RWTH Aachen University.
  28. m2p-labs GmbH, Baesweiler Germany, FlowerPlate® Enlighten your Research with our Flowers 2018.
  29. Wiltshire, K.H., et al., The determination of algal biomass (as chlorophyll) in suspended matter from the Elbe estuary and the German Bight: A comparison of high-performance liquid chromatography, delayed fluorescence and prompt fluorescence methods. Journal of Experimental Marine Biology and Ecology, 1998. 222(1): p. 113-131.
  30. Ramaraj, R., D.D. Tsai, and P.H. Chen, Chlorophyll is not accurate measurement for algal biomass. Chiang Mai Journal of Science, 2013. 40(4): p. 547-555.
  31. Carvalho, A.P., et al., Light requirements in microalgal photobioreactors: an overview of biophotonic aspects. Applied Microbiology and Biotechnology, 2011. 89(5): p. 1275-1288.
  32. Johnson, T.J., et al., Photobioreactor cultivation strategies for microalgae and cyanobacteria. Biotechnology Progress, 2018. 34(4): p. 811-827.
  33. Daliry, S., et al., Investigation of optimal condition for Chlorella vulgaris microalgae growth. Global journal of environmental science and management, 2017. 3(2).
  34. Gong, Q., et al., Effects of Light and pH on Cell Density of Chlorella Vulgaris. Energy Procedia, 2014. 61: p. 2012-2015.
  35. Sforza, E., et al., Adjusted Light and Dark Cycles Can Optimize Photosynthetic Efficiency in Algae Growing in Photobioreactors. PLoS ONE, 2012. 7(6): p. e38975.
  36. Serra-Maia, R., et al., Influence of temperature on Chlorella vulgaris growth and mortality rates in a photobioreactor. Algal Research, 2016. 18: p. 352-359.
  37. Converti, A., et al., Effect of temperature and nitrogen concentration on the growth and lipid content of Nannochloropsis oculata and Chlorella vulgaris for biodiesel production. Chemical Engineering and Processing: Process Intensification, 2009. 48(6): p. 1146-1151.
  38. Minhas, A.K., et al., A Review on the Assessment of Stress Conditions for Simultaneous Production of Microalgal Lipids and Carotenoids. Frontiers in Microbiology, 2016. 7.
  39. Kong, W., et al., The characteristics of biomass production, lipid accumulation and chlorophyll biosynthesis of Chlorella vulgaris under mixotrophic cultivation. African Journal of Biotechnology, 2011. 10(55): p. 11620-11630.
  40. Scarsella, M., et al., Study on the optimal growing conditions of Chlorella vulgaris in bubble column photobioreactors. Chem. Eng, 2010. 20: p. 85-90.
  41. Heredia-Arroyo, T., et al., Mixotrophic cultivation of Chlorella vulgaris and its potential application for the oil accumulation from non-sugar materials. Biomass and Bioenergy, 2011. 35(5): p. 2245-2253.
  42. Blair, M.F., B. Kokabian, and V.G. Gude, Light and growth medium effect on Chlorella vulgaris biomass production. Journal of Environmental Chemical Engineering, 2014. 2(1): p. 665-674.
  43. Keil, T., et al., Polymer-based ammonium-limited fed-batch cultivation in shake flasks improves lipid productivity of the microalga Chlorella vulgaris. Bioresour Technol, 2019. 291: p. 121821.
  44. Fayyaz, M., et al., Genetic engineering of microalgae for enhanced biorefinery capabilities. Biotechnology Advances, 2020. 43: p. 107554.
  45. Ng, I.S., et al., Recent Developments on Genetic Engineering of Microalgae for Biofuels and Bio-Based Chemicals. Biotechnology Journal, 2017. 12(10): p. 1600644.

Interested in the BioLector XT?
Request more information below