Enzymatic hydrolysis of quinizarin diester by lipase in silica nanoparticles investigated by fluorescence microscopy
Source abstract
Abstract
The enzymatic hydrolysis of quinizarin diester in silica nanoparticle (NP) of 200 nm diameter is investigated by confocal fluorescence microscopy. The quinizarin diester substrate and the intermediate quinizarin monoester are non-fluorescent species and only the end product—quinizarin formed by enzymatic hydrolysis produces intense fluorescence of the silica NP. The enzyme activity of lipase adsorbed into silica NP was similar to that observed for lipase chemically bound to silica surface. In both situations, partial aggregation of the silica NP dispersed in thin film of polyvinylpyrrolidone was observed from fluorescence and scanning electron microscopy images. The fluorescence decay of the end product—quinizarin in silica NP was biexponential with decay times of 0.49 and 2.17 ns. These two decay times found are ascribed to quinizarin adsorbed in silica NP and dispersed in the surrounding medium, respectively.
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Research context
OpenAlex topics: Enzyme Catalysis and Immobilization · Analytical Chemistry and Chromatography · Enzyme-mediated dye degradation
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References (21)
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1. Ahn K-D, Yoo K-W, Soh J-H, Kang J-H (2009) Fluorescent photoimaging with polymers having protected quinizarin dye precursors by a dry process based on chemical amplification. React Funct Polym 69:111–11610.1016/j.reactfunctpolym.2008.10.012 ↗
2. Al-Suhair S (2005) Production of biodiesel by lipase-catalyzed transesterification of vegetable oils: a kinetics study. Biotechnol Prog 21:1442–144810.1021/bp050195k ↗
3. Bernede JC, Ben Nasrallah T, Jamali M, Mevellec JY, Rabiller C, Proutiere A (1995) Is a hydrogen bound responsible for the optical properties of some dihydroxyanthraquinones: quinizarin and anthraflavic? J Phys Chem Sol 56:1239–125110.1016/0022-3697(95)00055-0 ↗
4. Canton G, Riccò R, Marinello F, Carmignato S, Enrichi F (2011) Modified Stöber synthesis of highly luminescent dye-doped silica nanoparticles. J Nanopart Res 13:4349–435610.1007/s11051-011-0382-3 ↗
5. Duque M, Graupner M, Stutz H, Wicher I, Zechner R, Paltauf F, Hermetter A (1996) New fluorogenic triacylglycerol analogs as substrates for the determination and chiral discrimination of lipase activities. J Lipid Res 37:868–87610.1016/S0022-2275(20)37584-2 ↗
6. Ferreira APG, Frederice R, Janssen KPF, Gehlen MH (2011) Dually fluorescent silica nanoparticles. J Lumin 131:888–89310.1016/j.jlumin.2010.12.019 ↗
7. Gamba M, Lapis AAM, Dupont J (2008) Supported ionic liquid enzymatic catalysis for the production of biodiesel. Adv Synth Catal 350:160–16410.1002/adsc.200700303 ↗
8. Haugland RP, Johnson ID (1993) Detecting enzymes in living cells using fluorogenic substrates. J Fluoresc 3:119–12710.1007/BF00862728 ↗
9. Kim J-M, Kang J-H, Han D-K, Lee C-W, Ahn K-D (1998) A novel precursor for color and fluorescence imaging. Chem Mater 10:2332–233410.1021/cm980395+ ↗
10. Liu Q, DeShong P, Zachariah MR (2012) One-sep synthesis of dye-incorporated porous silica particles. J Nanopart Res 14:92310.1007/s11051-012-0923-4 ↗
11. Mateo C, Palomo JM, Fernndez-Lorente G, Guisan JM, Fernandez-Lafuente R (2007) Improvement of enzyme activity, stability and selectivity via immoblization techniques. Enzyme Microb Technol 40:1451–146310.1016/j.enzmictec.2007.01.018 ↗
12. Pal H, Palit DK, Mukherjee T, Mittal JP (1990) Interaction of the excited singlet state of disubstituted anthraquinones with aromatic hydrocarbons: a fluorescence-quenching study. Chem Phys Lett 173:354–35910.1016/0009-2614(90)85283-I ↗
13. Palit DK, Pal H, Mukherjee T, Mittal JPJ (1990) Photodynamics of the S1 state of some hydroxy- and amino-substituted naphthoquinones and anthraquinones. J Chem Soc Faraday Trans 86:3861–386910.1039/ft9908603861 ↗
14. Pavlidis IV, Vorhaben T, Gournis D, Papadopoulos GK, Bornscheuer UT, Stamatis H (2012) Regulation of catalytic behaviour of hydrolases through interaction with functionalized carbon-based nanomaterials. J Nanopart Res 14:84210.1007/s11051-012-0842-4 ↗
15. Popat A, Hartono SB, Stahr F, Liu J, Qiao SZ, Lu GQ (2011) Mesoporous silica nanoparticles for bioadsorption, enzyme immobilisation, and delivery carries. Nanoscale 3:2801–281810.1039/c1nr10224a ↗
16. Samuel J, Raccurt O, Poncelet O, Auge A, Ling WL, Cherns P, Grunwald D, Tillement O (2010) Surface characterization of fluorescent-functionalized silica nanoparticles: from the macroscatle to the nanoscale. J Nanopart Res 12:2255–226510.1007/s11051-009-9792-x ↗
17. Shi Q, Yang D, Su Y, Li J, Jiang Z, Jiang Y, Yuan W (2007) Covalent functionalization of multi-walled carbon nanotubes by lipase. J Nanopart Res 9:1205–121010.1007/s11051-006-9200-8 ↗
18. Stöber W, Fink A (1968) Controlled growth of monodisperse silica spheres in the micron size range. J Colloid Interface Sci 26:62–6910.1016/0021-9797(68)90272-5 ↗
19. Villeneuve P, Muderhwa JM, Graille J, Haas MJ (2000) Customizing lipases for biocatalysis: a survey of chemical, physical and molecular biological approaches. J Mol Catal B 9:113–14810.1016/S1381-1177(99)00107-1 ↗
20. Yang Y, Babiak P, Reymond J-L (2006) New monofunctionalized fluorescein derivatives for the efficient high-throughput screening of lipases and esterases in aqueous media. Helv Chim Acta 89:404–41510.1002/hlca.200690041 ↗
21. Yo H, Pak J (2013) Synthesis of highly fluorescent silica nanoparticles in a reverse microemulsion through double-layered doping of organic fluorophores. J Nanopart Res 15:160910.1007/s11051-013-1609-2 ↗