Cell Disruption and Hydrolysis of Microchloropsis salina Biomass as a Feedstock for Fermentation
Source abstract
Abstract
Microalgae are a promising biomass source because of their capability to fixate CO2 very efficiently. In this study, the potential of Microchloropsis salina biomass as a feedstock for fermentation was explored, focusing on biomass hydrolysis by employing various mechanical and chemical cell disruption strategies in combination with enzymatic hydrolysis. Among the mechanical cell disruption methods investigated on a lab scale, namely ultrasonication, bead milling, and high-pressure homogenization, the most effective was bead milling using stainless-steel beads with a diameter of 2 mm. In this way, 87–97% of the cells were disrupted in 40 min using a mixer mill. High-pressure homogenization was also effective, achieving 86% disruption efficiency after four passes on a 30–200 L scale using biomass with 15% (w/w) solids content. Enzymatic hydrolysis of the disrupted cells using a mixture of cellulases and mannanases yielded up to 25% saccharification efficiency after 72 h. Acidic hydrolysis of undisrupted cells followed by enzymatic treatment yielded around 30% saccharification efficiency but was coupled with significant dilution of the resulting hydrolysate. Microalgal biomass hydrolysate produced was determined to have ~8.1 g L−1 sugars and 2.5% (w/w) total carbon, as well as sufficient nitrogen and phosphorus content as a fermentation medium.
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Research context
OpenAlex topics: Algal biology and biofuel production · Microbial Metabolic Engineering and Bioproduction
SciVX discovery tags are terminology-based. OpenAlex topics are source-provided classifications.
Affiliations
Chair of Biochemical Engineering, School of Engineering and Design, Technical University of Munich, 85748 Garching, Germany
TUM-AlgaeTec Center, Technical University of Munich, 82024 Taufkirchen, Germany
TUM Pilot Plant for Industrial Biotechnology, Technical University of Munich, 85748 Garching, Germany
Werner Siemens—Chair of Synthetic Biotechnology, School of Natural Sciences, Technical University of Munich, 85748 Garching, Germany
Funding
German Federal Ministry of Education and Research (BMBF, Berlin, Germany)
References (60)
Show source-provided references
1. Mittermeier, F., Fischer, F., Hauke, S., Hirschmann, P., and Weuster-Botz, D. (2024). Valorization of wheat bran by co-cultivation of fungi with integrated hydrolysis to provide sugars and animal feed. BioTech, 13.10.3390/biotech13020015 ↗
2. Knesebeck, M., Schäfer, D., Schmitz, K., Rüllke, M., Benz, J.P., and Weuster-Botz, D. (2023). Enzymatic one-pot hydrolysis of extracted sugar beet press pulp after solid-state fermentation with an engineered Aspergillus niger strain. Fermentation, 9.10.3390/fermentation9070582 ↗
3. Comparative evaluation of Aspergillus niger strains for endogenous pectin-depolymerization capacity and suitability for d-galacturonic acid production10.1007/s00449-020-02347-z ↗
4. Rerop, Z.S., Stellner, N.I., Graban, P., Haack, M., Mehlmer, N., Masri, M., and Brück, T.B. (2023). Bioconversion of a lignocellulosic hydrolysate to single cell oil for biofuel production in a cost-efficient fermentation process. Fermentation, 9.10.3390/fermentation9020189 ↗
5. Koruyucu, A., Blums, K., Peest, T., Schmack-Rauscher, L., Brück, T., and Weuster-Botz, D. (2023). High-cell-density yeast oil production with diluted substrates imitating microalgae hydrolysate using a membrane bioreactor. Energies, 16.10.3390/en16041757 ↗
6. Saccharification of carbohydrates in microalgal biomass by physical, chemical and enzymatic pre-treatments as a previous step for bioethanol production10.1016/j.cej.2014.10.049 ↗
7. Koruyucu, A., Schädler, T., Gniffke, A., Mundt, K., Krippendorf, S., Urban, P., Blums, K., Halim, B., Brück, T., and Weuster-Botz, D. (2024). Energy-efficient production of Microchloropsis salina biomass with high CO2 fixation yield in open thin-layer cascade photobioreactors. Processes, 12.10.3390/pr12071303 ↗
8. Brenner, A., and Abeliovich, A. (2013). Water purification: Algae in wastewater oxidation ponds. Handbook of Microalgal Culture, John Wiley & Sons, Ltd.10.1002/9781118567166.ch31 ↗
9. Kaplan, D. (2013). Absorption and adsorption of heavy metals by microalgae. Handbook of Microalgal Culture, John Wiley & Sons.10.1002/9781118567166.ch32 ↗
10. Lipid production with Trichosporon oleaginosus in a membrane bioreactor using microalgae hydrolysate10.1016/j.jbiotec.2016.10.021 ↗
11. Microbial lipid production by oleaginous yeasts grown on Scenedesmus obtusiusculus microalgae biomass hydrolysate10.1007/s00449-020-02354-0 ↗
12. Schädler, T., Caballero Cerbon, D., de Oliveira, L., Garbe, D., Brück, T., and Weuster-Botz, D. (2019). Production of lipids with Microchloropsis salina in open thin-layer cascade photobioreactors. Bioresour. Technol., 289.10.1016/j.biortech.2019.121682 ↗
13. Lipid and biomass production by the halotolerant microalga Nannochloropsis salina10.1016/0144-4565(87)90006-0 ↗
14. Borowitzka, M.A., and Moheimani, N.R. (2013). Photobioreactors for microalgal biofuel production. Algae for Biofuels and Energy, Springer.10.1007/978-94-007-5479-9 ↗
15. Andersen, R.A. (2013). The microalgal cell. Handbook of Microalgal Culture, John Wiley & Sons.10.1002/9781118567166.ch1 ↗
16. Quantitative evaluation of the ease of rupture of industrially promising microalgae by high pressure homogenization10.1016/j.biortech.2013.04.074 ↗
17. Ultrastructure and composition of the Nannochloropsis gaditana cell wall10.1128/EC.00183-14 ↗
18. Cell disruption for microalgae biorefineries10.1016/j.biotechadv.2015.01.008 ↗
19. Chmiel, H., Takors, R., and Weuster-Botz, D. (2018). Aufarbeitung (Downstream Processing). Bioprozesstechnik, Springer.10.1007/978-3-662-54042-8 ↗
20. Conversion of cheese whey and whey permeate to oil and single-cell protein10.3168/jds.S0022-0302(78)83762-X ↗
21. A seagrass-based biorefinery for generation of single-cell oils for biofuel and oleochemical production10.1002/ente.201700604 ↗
22. Microbial conversion of olive oil mill wastewaters into lipids suitable for biodiesel production10.1021/jf101282t ↗
23. Oil production by oleaginous yeasts using the hydrolysate from pretreatment of wheat straw with dilute sulfuric acid10.1016/j.biortech.2011.02.081 ↗
24. Chemical phosphorus removal to extremely low levels: Experience of two plants in the Washington, DC area10.2166/wst.2006.402 ↗
25. Fluorescence properties of allophycocyanin and a crosslinked allophycocyanin trimer10.1002/cyto.990080113 ↗
26. Protein measurements of microalgal and cyanobacterial biomass10.1016/j.biortech.2010.04.077 ↗
27. Rapid quantification of microalgal lipids in aqueous medium by a simple colorimetric method10.1016/j.biortech.2013.12.077 ↗
28. Composition of algal oil and its potential as biofuel10.1155/2012/285185 ↗
29. Hydrothermal liquefaction of Spirulina and Nannochloropsis salina under subcritical and supercritical water conditions10.1016/j.biortech.2012.12.144 ↗
30. Quantitative calorimetry and biochemical engineering10.1016/S1573-4374(99)80009-0 ↗
31. The effect of high-intensity ultrasound on cell disruption and lipid extraction from high-solids viscous slurries of Nannochloropsis sp. biomass10.1016/j.algal.2018.09.004 ↗
32. Effect of sonication frequency on the disruption of algae10.1016/j.ultsonch.2015.12.011 ↗
33. Evaluation and comparison of algal cell disruption methods: Microwave, waterbath, blender, ultrasonic and laser treatment10.1016/j.apenergy.2012.09.020 ↗
34. Disruption of microalgal cells using high-frequency focused ultrasound10.1016/j.biortech.2013.11.054 ↗
35. Gonzalez-Fernandez, C., and Muñoz, R. (2017). Cell disruption technologies. Microalgae-Based Biofuels and Bioproducts, Woodhead Publishing.
36. Grima, E.M., Acién Fernández, F.G., and Robles Medina, A. (2013). Downstream processing of cell mass and products. Handbook of Microalgal Culture, John Wiley & Sons.10.1002/9781118567166.ch14 ↗
37. Quesada-Salas, M.C., Delfau-Bonnet, G., Willig, G., Préat, N., Allais, F., and Ioannou, I. (2021). Optimization and comparison of three cell disruption processes on lipid extraction from microalgae. Processes, 9.10.3390/pr9020369 ↗
38. Optimization of bead milling parameters for the cell disruption of microalgae: Process modeling and application to Porphyridium cruentum and Nannochloropsis oculata10.1016/j.biortech.2015.07.075 ↗
39. Disintegration of Nannochloropsis sp. cells in an improved turbine bead mill10.1016/j.biortech.2017.08.146 ↗
40. Kröger, M., Klemm, M., and Nelles, M. (2018). Hydrothermal disintegration and extraction of different microalgae species. Energies, 11.10.3390/en11020450 ↗
41. Influence of processing parameters on disintegration of Chlorella cells in various types of homogenizers10.1007/s00253-008-1660-6 ↗
42. Microalgal cell disruption for biofuel development10.1016/j.apenergy.2011.08.048 ↗
43. Rapid method for the determination of lipid from the green alga Botryococcus braunii10.1023/A:1008811716448 ↗
44. Selective extraction from microalgae Nannochloropsis sp. using different methods of cell disruption10.1016/j.biortech.2013.12.011 ↗
45. Energy evaluation of algal cell disruption by high pressure homogenisation10.1016/j.biortech.2014.11.049 ↗
46. Low solvent, low temperature method for extracting biodiesel lipids from concentrated microalgal biomass10.1016/j.biortech.2013.09.022 ↗
47. Emerging techniques for cell disruption and extraction of valuable bio-molecules of microalgae Nannochloropsis sp.10.1007/s00449-018-2038-5 ↗
48. Enhanced lipid recovery from Nannochloropsis microalgae by treatment with optimized cell wall degrading enzyme mixtures10.1016/j.biortech.2016.04.025 ↗
49. Bioethanol production using carbohydrate-rich microalgae biomass as feedstock10.1016/j.biortech.2012.10.015 ↗
50. Enzymatic cell disruption of microalgae biomass in biorefinery processes10.1002/bit.25644 ↗
51. Novel, resistant microalgal polyethers: An important sink of organic carbon in the marine environment?10.1016/0016-7037(96)00038-5 ↗
52. Conversion of lipid-extracted Nannochloropsis salina biomass into fermentable sugars10.1016/j.algal.2015.01.013 ↗
53. Enzymatic cell wall degradation of Chlorella vulgaris and other microalgae for biofuels production10.1007/s00425-012-1765-0 ↗
54. Treatment of Phaeodactylum tricornutum cells with papain facilitates lipid extraction10.1016/j.jbiotec.2012.06.033 ↗
55. Jeong, S.W., Nam, S.W., HwangBo, K., Jeong, W.J., Jeong, B.-r., Chang, Y.K., and Park, Y.-I. (2017). Transcriptional regulation of cellulose biosynthesis during the early phase of nitrogen deprivation in Nannochloropsis salina. Sci. Rep., 7.10.1038/s41598-017-05684-4 ↗
56. A novel one-stage cultivation/fermentation strategy for improved biogas production with microalgal biomass10.1016/j.jbiotec.2015.05.008 ↗
57. Structure, morphology, size and application of iron phosphate10.1515/rams-2020-0039 ↗
58. Influence of nitrogen and iron limitations on lipid production by Cryptococcus curvatus grown in batch and fed-batch culture10.1016/0032-9592(95)00077-1 ↗
59. High cell density cultivation of Escherichia coli at controlled specific growth rate10.1016/0168-1656(91)90032-Q ↗
60. Linking microalgae and cyanobacteria culture conditions and key-enzymes for carbohydrate accumulation10.1016/j.biotechadv.2012.07.003 ↗