Back to Journals » International Journal of Nanomedicine » Volume 10 » Special Issue on diverse applications in Nano-Theranostics

Ultrafast sonochemical synthesis of protein-inorganic nanoflowers

Authors Batule BS , Park KS, Kim MI , Park HG, An SSA 

Received 10 June 2015

Accepted for publication 28 July 2015

Published 25 August 2015 Volume 2015:10(Special Issue on diverse applications in Nano-Theranostics) Pages 137—142


Checked for plagiarism Yes

Review by Single anonymous peer review

Peer reviewer comments 3

Editor who approved publication: Dr Thomas J Webster

Bhagwan S Batule,1 Ki Soo Park,1 Moon Il Kim,2 Hyun Gyu Park1

1Department of Chemical and Biomolecular Engineering (BK21+ Program), Korea Advanced Institute of Science and Technology (KAIST), Daejeon, 2Department of BioNano Technology, Gachon University, Seongnam, Republic of Korea

Abstract: We developed a simple but efficient method to synthesize protein-inorganic hybrid nanostructures with a flower-like shape (nanoflowers), which relies on sonication to facilitate the synthesis of the nanoflowers. With this technique, we synthesized nanoflowers containing laccase as a model protein and copper phosphate within 5 minutes at room temperature. The resulting laccase nanoflowers yielded greatly enhanced activity, stability, and reusability, and their usefulness was successfully demonstrated by applying them in the colorimetric detection of epinephrine. The strategy developed could be used to rapidly synthesize nanoflowers for various applications in biosensor and enzyme catalysis and would expand the utilization of nanoflowers in diverse fields of biotechnology.

Keywords: copper phosphate, laccase, epinephrine, hybrid nanomaterials


Nanobiocatalysis, which utilizes enzymes incorporated within nanostructured materials for improving the performance of natural enzymes, has created new opportunities in enzymatic applications including biosensors and biocatalysis.16 To achieve an efficient nanobiocatalysis system, enzymes have been generally immobilized within various nanostructured materials by employing approaches such as physical adsorption, covalent attachment, and entrapment.79 Physical adsorption is very simple to perform and effective at retaining enzyme activity during adsorption, but stability is poor due to the leaching of adsorbed enzymes during the operation. On the other hand, covalent attachment can achieve fairly good stabilization of enzyme activity, but requires tedious procedures to covalently attach the enzyme molecules to the surface of the materials.7 Entrapment of enzyme molecules within a polymeric network could efficiently retain and stabilize enzymes, however, its practical use is generally restricted by mass transfer limitation through the solid support.1 Therefore, there has been a continuous need to develop a novel immobilization method that effectively retains and stabilizes enzyme activity by overcoming the mentioned limitations.10

Along this line, several groups have reported different innovative strategies to synthesize enzyme-inorganic hybrid nanostructures having flower-like shapes (nanoflowers) from enzyme and copper or calcium phosphate,1113 which are more stable and active than the conventionally immobilized enzymes. The nanoflowers made from laccase and copper phosphate were also successfully applied to detect phenol in an aqueous solution with the enhanced activity and stability.14 Furthermore, several groups have utilized enzyme-inorganic hybrid nanoflowers for different applications such as detection of hydrogen peroxide,15 glucose,16 and protein digestion.17 Although the enzyme-inorganic hybrid nanoflowers resulted in greatly enhanced activity and stability, their synthesis was so slow that they had to be incubated in the reaction mixture for up to 3 days at room temperature (RT), which critically limited their widespread use in real applications. Therefore, there is a significant incentive to develop an innovative method to rapidly synthesize protein-inorganic nanoflowers by effectively reducing the reaction time, which could establish the large-scale production of enzyme-incorporated nanoflowers within relatively short period of time.

Toward this goal, we developed a novel and ultrafast sonochemical method to synthesize protein-inorganic nanoflowers. Although sonication treatment has been employed to facilitate the synthesis of several kinds of nanostructures for many years, there has been no report, as far as we are aware, of its use for the synthesis of protein-inorganic nanoflowers.18 By using this technique, we synthesized nanoflowers containing protein and copper phosphate in a significantly shortened reaction time – within 5 minutes at RT – presumably because the sonication approach may allow the building blocks (copper phosphate) to quickly complete the self-assembly process by uniformly providing high energy to the structure.1921 Importantly, this rapid process enables efficient scale-up production of the nanoflowers for practical applications in various fields of biotechnology.

Materials and methods


Bovine serum albumin (BSA) (lyophilized powder), laccase from Trametes versicolor, copper(II) sulfate pentahydrate, syringaldazine, and (−)-epinephrine were purchased from Sigma-Aldrich Co (St Louis, MO, USA). Phosphate-buffered saline (PBS; 1×, pH 7.4) was obtained from Thermo Fisher Scientific (Waltham, MA, USA). All other chemicals were of analytical grade and used without further purification. Aqueous solutions were prepared using UltraPure™ DNase/RNase-Free Distilled Water (Thermo Fisher Scientific).

Synthesis of nanoflowers

The conventional method used to prepare nanoflowers involves 20 μL of aqueous CuSO4 solution (120 mM) being added to 3 mL of PBS (pH 7.4) at 25°C containing proteins at different concentrations, followed by incubation at RT for 3 days. In the study reported here, we synthesized nanoflowers following the same procedure but sonicated the solution for different time intervals instead of incubating at RT. For sonication, we utilized a Branson (1510) bath sonicator (length 15.2 cm, breadth 14 cm, height 10.2 cm, operating capacity 1.9 L) at a frequency of 40 kHz and power of 70 W.

Characterization of nanoflowers

Scanning electron microscopy (SEM) images were obtained by using a Magellan™ 400 Field Emission Scanning Electron Microscope. For the analyses, the suspension of prepared nanoflowers was filtered and dried on a membrane (pore size: 0.1 μm). For X-ray diffraction (XRD) analysis (D/MAX-2500, Rigaku Corporation, Tokyo, Japan), 100 mL of reaction mixture was prepared by dissolving bovine serum albumin (BSA; 10 mg) in PBS (pH 7.4) followed by the subsequent addition of CuSO4 solution (120 mM, 0.665 mL). Finally, the reaction mixture was sonicated for 5 minutes at RT, then the precipitate was collected, washed with deionized water, and dried at 80°C for 1 day before XRD measurement. The encapsulation yield of protein in the nanoflowers was calculated by measuring the protein amount in the supernatant using a Novagen® bicinchoninic acid (BCA) protein assay kit (EMD Millipore, Billerica, MA, USA) using BSA as a standard.22 The weight percentage of protein in nanoflowers was calculated based on the encapsulation yield and the weight of the powder.

Measurement of enzyme activity using syringaldazine or epinephrine

The enzymatic activities of sonicated laccase nanoflowers (0.1 mg·mL−1), sonicated laccase (0.1 mg·mL−1), and free laccase (0.1 mg·mL−1) were determined by measuring the absorbance intensity using syringaldazine (40 μM) as a substrate in PBS buffer (pH 7.4) at 25°C for 30 minutes. Absorbance intensity was measured using a Tecan Infinite® M200 PRO microplate reader (Männedorf, Switzerland) with a transparent 96-well plate. The enzymatic activities of sonicated laccase nanoflowers (30 μg·mL−1) and free laccase (30 μg·mL−1) were determined by using epinephrine as a substrate at different concentrations (25.0, 12.5, 5.0, 2.5, and 1.0 μg·mL−1) in PBS (pH 7.4) for 20 minutes. After the reaction, the reaction mixture was used to obtain images showing the progress of the reaction.

Measurement of stability and reusability

The storage stability of the epinephrine sensing system was checked in aqueous buffer (PBS, pH 7.4) under static conditions at 25°C. First, the initial activity was determined by measuring the fluorescence emission intensity at 506 nm with the excitation at 375 nm during the typical reaction that involved sonicated laccase nanoflowers (30 μg·mL−1) or free laccase (30 μg·mL−1) with epinephrine as a substrate (50 μg·mL−1) in PBS (pH 7.4) at 25°C for 20 minutes. The residual activity of each sample was then determined at predetermined time. Reusability was assessed after repeated cycles involving the typical reaction using sonicated laccase nanoflowers (0.1 mg·mL−1) and epinephrine (50 μg·mL−1) in PBS (pH 7.4) at 25°C for 20 minutes, separation by centrifugation at 11,000 rpm for 2 minutes, and excessive washing (three times) with PBS. The excessively washed sample was reused for the measurement of the residual activity. The relative activity (%) was determined by calculating the ratio of the residual activity to the initial activity. Fluorescence intensities were measured using the Tecan Infinite M200 PRO microplate reader with a black 384-well plate.

Results and discussion

The overall scheme for the sonochemical synthesis of protein-inorganic nanoflowers is described in Figure 1. To synthesize the sonicated nanoflowers, aqueous PBS solution containing copper(II) sulfate and protein (BSA or laccase) was simply sonicated for 5 minutes, which resulted in the formation of protein-inorganic nanoflowers with flower-like nanostructures, as obtained using the conventional method.11 We expected that the nanoflowers rapidly prepared by using this simple sonication treatment would exhibit enhanced catalytic activity and stability like those prepared by the conventional method, and thus, this method could be employed to very conveniently synthesize protein-inorganic nanoflowers.

Figure 1 Sonication-mediated synthesis of protein-inorganic nanoflowers.

The effect of sonication time on the synthesis of the nanoflowers was first investigated by sonicating the solution containing model protein BSA and copper(II) sulfate in an ordinary ultrasonic bath under a 40 kHz operating frequency for 1 minute, 5, and 7 minutes at RT (Figure 2A). After 1 minute’s sonication, small sized microspheres (average size of ~2 μm) with relatively smooth surfaces were observed, indicating that 1 minute’s sonication was not long enough to bloom flowers, which is required for the formation of nanoflowers. On the other hand, after 5 minutes’ sonication, BSA-copper nanoflowers having average size of ~8 μm were clearly formed and no further blooming of the flowers or growth of flower-like structures was observed during prolonged sonication, as evidenced by comparing the nanoflowers with those synthesized from 7 minutes’ sonication. On the basis of encapsulation yield for the nanoflowers prepared by three different sonication times, 5 minutes was selected as an optimal sonication time showing the highest encapsulation yield, 82% (Figure 2B).

Figure 2 Sonication-mediated synthesis of bovine serum albumin (BSA) nanoflowers. (A) Effect of sonication times on the formation of nanoflowers. (B) Encapsulation yield (%) corresponding to (A). (C) Effect of BSA concentration on the formation of nanoflowers. (D) Encapsulation yield (%) corresponding to (C). Bold text (B, D) indicates the optimal sonication time or BSA concentration showing the highest encapsulation yield.
Note: Scale bar is 10 μm.

We also investigated the effect of BSA concentration on the morphology of sonicated nanoflowers and encapsulation yield. The investigation proved that the flower-like morphology of sonicated nanoflowers was not significantly affected by the concentration of BSA, whereas a negative control sample without any protein molecules did not result in flower-like structures (Figure 2C). When we used 0.02 mg·mL−1 BSA in the sonochemical synthesis of nanoflowers, the encapsulation yield and weight percentage of BSA in the nanoflowers were determined to be the highest ones, 82% and 7%, respectively (Figure 2D).

Next, we employed laccase, one of the important enzymes in biosensing applications to detect diverse kinds of catecholamines, in the sonochemical synthesis of nanoflowers to demonstrate the real applicability of this method in biosensing fields. As illustrated in Figure 3, sonochemical treatment for 5 minutes successfully synthesized flower-like nanostructures similar to the BSA-based nanoflowers. Among the tested concentrations of laccase, 0.1 mg·mL−1 was chosen as the optimal one because it resulted in highly elaborate flower-like morphology as well as the highest enzyme encapsulation yield (Figure 3A, B). High-magnification SEM images of the sonicated laccase nanoflowers clearly revealed their hierarchical structures with high surface-to-volume ratios (Figure 3C). Also, XRD patterns obtained from the sonicated laccase nanoflowers synthesized under the optimal reaction condition fit well with those of Cu3(PO4)2·3H2O (JCPDS 00-022-0548), indicating copper was incorporated in the nanoflowers (Figure 4).11

Figure 3 Sonication-mediated synthesis of laccase nanoflowers. (A) Effect of laccase concentration on the formation of nanoflowers. (B) Encapsulation yield (%) corresponding to (A). (C) High-magnification scanning electron microscopy images of the sonicated laccase nanoflowers prepared from 0.1 mg·mL−1 laccase. (B) Bold text indicates the optimal laccase concentration showing the highest encapsulation yield.
Note: Scale bar in (A) is 5 μm.

Figure 4 X-ray diffraction patterns of sonicated laccase nanoflowers representing peaks for the Cu3(PO4)2·3H2O (JCPDS 00-022-0548) and some NaCl crystals (JCPDS 01-088-2300), which confirms that the product originated from phosphate-buffered saline.
Abbreviation: JCPDS, Joint Committee on Powder Diffraction Standards.

The catalytic activity of the sonicated laccase nanoflowers synthesized under the optimal condition was then evaluated. In a typical activity assay using syringaldazine as a substrate, the sonicated laccase nanoflowers showed ~150% activity compared to the free laccase (Figure 5A), confirming that the synthesizing of laccase nanoflowers by simple sonication also effectively enhanced their catalytic activity like the conventional method.11 The enhanced catalytic activity of sonicated laccase nanoflowers could be a very distinctive advantage considering that the immobilization of enzymes generally leads to lowered activity.23 We also confirmed that the sonication treatment of free laccase for 5 minutes did not deteriorate the enzyme activity (Figure 5A).

Figure 5 Enhanced performance of laccase nanoflowers synthesized by sonication-based method. (A) Measurement of laccase activity by employing 40 μM syringaldazine as a substrate in phosphate-buffered saline (PBS) buffer (pH 7.4) at 25°C. (B) Visual detection of epinephrine by using sonicated laccase nanoflowers and free laccase. (C) Stability of sonicated laccase nanoflowers and free laccase for detecting epinephrine in PBS (pH 7.4) at 25°C. (D) Reusability of the sonicated laccase nanoflowers for detecting epinephrine.
Note: In (B), 25.0, 12.5, 5.0, 2.5, and 1.0 μg·mL−1 of epinephrine in PBS (pH 7.4) are denoted by 1, 2, 3, 4, and 5, respectively.
Abbreviations: F, free laccase (30 μg·mL−1); N, sonicated laccase nanoflowers.

Finally, we demonstrated the applicability of rapidly synthesized, sonicated laccase nanoflowers for the detection of epinephrine, which should be monitored for the appropriate treatment of anaphylactic shock, bronchial asthma, and organic heart disease.24,25 In a typical colorimetric reaction to employ epinephrine as a substrate, the laccase nanoflowers yielded much denser and greater color changes than those yielded by free laccase, confirming their higher activity in detecting epinephrine (Figure 5B). Weak reddish color intensities were produced by the laccase nanoflowers at a low substrate concentration of epinephrine (below 5 μg mL−1); these can be attributed to the fact that the green-colored nanoflowers may have critically attenuated the reddish color because the photograph was obtained without removing the nanoflower pellet from the reaction tube. Next, we investigated the stability and reusability of our sonicated laccase nanoflowers – two very important factors to evaluate in determining the performance of the enzymatic system. As presented in Figure 5C, the laccase nanoflowers showed remarkable stability, preserving their initial activity over 95% for 1 month, whereas free laccase lost ~50% of initial activity within 10 days during the incubation at RT (Figure 5C). Moreover, when the laccase nanoflowers were recycled and reused after simple centrifugation for 2 minutes, there was no significant loss of activity observed in detecting epinephrine for up to four cycles (Figure 5D). These vividly enhanced stability and reusability characteristics could enable the nanoflowers to be widely employed in various applications for biosensor and enzyme catalysis.


Overall, in this study, we discovered that a simple sonication treatment can significantly reduce the synthesis time for organic–inorganic hybrid nanoflowers, potentially enabling scaled-up production within a significantly short period of time of 5 minutes at RT. The resulting nanoflowers yielded highly enhanced activity, stability, and reusability, and thus, this strategy should be a powerful strategy in the preparation of the nanoflowers. Furthermore, the method developed in this study may be applied to rapidly synthesize multi-enzyme co-embedded nanoflowers for potential application in biosensor, biocatalysis, and biofuel cells. Future research will range from the development of new types of organic–inorganic hybrid nanoflowers with certified synthetic mechanism to more diverse applications in theranostics (therapy and diagnosis) and other bio-related devices.


This research was supported by the Basic Science Research Program through the National Research Foundation of Korea (NRF) funded by the Ministry of Education [number 2015R1A2A1A01005393]. This work was also supported by the Center for BioNano Health-Guard funded by the Ministry of Science, ICT and Future Planning (MSIP) of Korea as the Global Frontier Project (H-GUARD-2013M3A6B2078964) and by the Basic Science Research Program through the NRF funded by the MSIP (NRF-2014R1A1A1006016).

In addition, the authors would like to thank the National Institute for International Education (NIIED), Ministry of Education, Science and Technology (MEST), Republic of Korea, for a graduate scholarship to Bhagwan S Batule.


Bhagwan S Batule received a graduate scholarship from the National Institute for International Education (NIIED), Ministry of Education, Science and Technology (MEST), Republic of Korea. The authors report no other conflicts of interest in this work.



Kim J, Grate JW, Wang P. Nanostructures for enzyme stabilization. Chem Eng Sci. 2006;61(3):1017–1026.


Wang P. Nanoscale biocatalyst systems. Curr Opin Biotech. 2006;17(6):574–579.


Kim JB, Grate JW, Wang P. Nanobiocatalysis and its potential applications. Trends Biotechnol. 2008;26(11):639–646.


Ge J, Lu DN, Liu ZX, Liu Z. Recent advances in nanostructured biocatalysts. Biochem Eng J. 2009;44(1):53–59.


Yan M, Ge J, Liu Z, Ouyang PK. Encapsulation of single enzyme in nanogel with enhanced biocatalytic activity and stability. J Am Chem Soc. 2006;128(34):11008–11009.


Kim MI, Shim J, Li T, Lee J, Park HG. Fabrication of nanoporous nanocomposites entrapping Fe3O4 magnetic nanoparticles and oxidases for colorimetric biosensing. Chem Eur J. 2011;17(38):10700–10707.


Luckarift HR, Spain JC, Naik RR, Stone MO. Enzyme immobilization in a biomimetic silica support. Nat Biotechnol. 2004;22(2):211–213.


Kim MI, Shim J, Li T, et al. Colorimetric quantification of galactose using a nanostructured multi-catalyst system entrapping galactose oxidase and magnetic nanoparticles as peroxidase mimetics. Analyst. 2012;137(5):1137–1143.


Kim MI, Shim J, Parab HJ, Shin SC, Lee J, Park HG. A convenient alcohol sensor using one-pot nanocomposite entrapping alcohol oxidase and magnetic nanoparticles as peroxidase mimetics. J Nanosci Nanotechnol. 2012;12(7):5914–5919.


Wang R, Zhang YF, Lu DN, Ge J, Liu Z, Zare RN. Functional protein-organic/inorganic hybrid nanomaterials. Wiley Interdiscip Rev Nanomed Nanobiotechnol. 2013;5(4):320–328.


Ge J, Lei JD, Zare RN. Protein-inorganic hybrid nanoflowers. Nat Nanotechnol. 2012;7(7):428–432.


Ghosh K, Balog ER, Sista P, Williams D, Kelly D. Temperature-dependent morphology of hybrid nanoflowers from elastin-like polypeptides. APL Mater. 2014;2(2):021101–021106.


Shi J, Zhang S, Wang X, Yang C, Jiang Z. Preparation and enzymatic application of flowerlike hybrid microcapsules through a biomimetic mineralization approach. J Mater Chem B. 2014;2(27):4289–4296.


Zhu L, Gong L, Zhang YF, et al. Rapid detection of phenol using a membrane containing laccase nanoflowers. Chem Asian J. 2013;8(10):2358–2360.


Lin Z, Xiao Y, Yin YQ, Hu WL, Liu W, Yang HH. Facile synthesis of enzyme-inorganic hybrid nanoflowers and its application as a colorimetric platform for visual detection of hydrogen peroxide and phenol. Acs Appl Mater Interfaces. 2014;6(13):10775–10782.


Sun JY, Ge JC, Liu WM, et al. Multi-enzyme co-embedded organic-inorganic hybrid nanoflowers: synthesis and application as a colorimetric sensor. Nanoscale. 2014;6(1):255–262.


Lin Z, Xiao Y, Wang L, Hu W, Liu W, Yang HH. Facile synthesis of enzyme-inorganic hybrid nanoflowers and their application as an immobilized trypsin reactor for highly efficient protein digestion. RSC Adv. 2014;4(27):13888–13891.


Xu HX, Zeiger BW, Suslick KS. Sonochemical synthesis of nanomaterials. Chem Soc Rev. 2013;42(7):2555–2567.


Gogate PR, Sutkar VS, Pandit AB. Sonochemical reactors: important design and scale up considerations with a special emphasis on hetereogeneous systems. Chem Eng J. 2011;166(3):1066–1082.


Gogate PR. Cavitational reactors for process intensification of chemical processing applications: a critical review. Chem Eng Process. 2008;47(4):515–527.


Sutkar VS, Gogate PR. Design aspects of sonochemical reactors: techniques for understanding cavitational activity distribution and effect of operating parameters. Chem Eng J. 2009;155(1–2):26–36.


Smith PK, Krohn RI, Hermanson GT, et al. Measurement of protein using bicinchoninic acid. Anal Biochem. 1985;150(1):76–85.


Mateo C, Grazu V, Palomo JM, Lopez-Gallego F, Fernandez-Lafuente R, Guisan JM. Immobilization of enzymes on heterofunctional epoxy supports. Nat Protoc. 2007;2(5):1022–1033.


Lu XQ, Li YY, Du J, et al. A novel nanocomposites sensor for epinephrine detection in the presence of uric acids and ascorbic acids. Electrochim Acta. 2011;56(21):7261–7266.


Shankar SS, Swamy BEK. Detection of epinephrine in presence of serotonin and ascorbic acid by TTAB modified carbon paste electrode: a voltammetric study. Int J Electrochem Sci. 2014;9(3):1321–1339.

Creative Commons License © 2015 The Author(s). This work is published and licensed by Dove Medical Press Limited. The full terms of this license are available at and incorporate the Creative Commons Attribution - Non Commercial (unported, v3.0) License. By accessing the work you hereby accept the Terms. Non-commercial uses of the work are permitted without any further permission from Dove Medical Press Limited, provided the work is properly attributed. For permission for commercial use of this work, please see paragraphs 4.2 and 5 of our Terms.