- Nano Express
- Open Access
DNA-directed immobilization of horseradish peroxidase onto porous SiO2 optical transducers
Nanoscale Research Lettersvolume 7, Article number: 443 (2012)
Multifunctional porous Si nanostructure is designed to optically monitor enzymatic activity of horseradish peroxidase. First, an oxidized PSi optical nanostructure, a Fabry-Pérot thin film, is synthesized and is used as the optical transducer element. Immobilization of the enzyme onto the nanostructure is performed through DNA-directed immobilization. Preliminary studies demonstrate high enzymatic activity levels of the immobilized horseradish peroxidase, while maintaining its specificity. The catalytic activity of the enzymes immobilized within the porous nanostructure is monitored in real time by reflective interferometric Fourier transform spectroscopy. We show that we can easily regenerate the surface for consecutive biosensing analysis by mild dehybridization conditions.
Nanostructured porous Si (PSi) has emerged as a promising material for optical biosensing applications due to its large internal surface area and tunable optical properties[1–3]. Numerous biosensing applications, including the detection of DNA hybridization, proteins[5, 6], and enzymatic activity[7, 8], have been presented, demonstrating the advantages of these nanosystems in terms of improved detection sensitivity, label-free and real-time rapid analysis. However, the major challenge in designing these biosensors arises from the intrinsic instability of the recognition element during the immobilization procedures onto the transducer’s surface[9–11].
The present work describes a highly versatile approach for reversible enzyme conjugation to a porous SiO2 (PSiO2) surface via DNA-directed immobilization (DDI). This approach has been successfully used for the immobilization of different classes of enzymes onto a range of solid supports, without affecting their biological activity[9, 12]. DDI strategy utilizes the site-selectivity and the high affinity of Watson-Crick base pairing between two complimentary strands. Taking into account that DNA hybridization is a reversible process, the anchored enzyme as well as the biosensor surface can be regenerated and reused for multiple reaction cycles. Herein, we demonstrate this concept for a model enzyme, horseradish peroxidase (HRP), which is one of the most active peroxidases and often used as a powerful tool in biotechnology (e.g., organic synthesis, immune-detection, and wastewater treatment)[13, 14].
Preparation of porous SiO2 nanostructures
Single side polished on the <100 > face oriented and heavily doped p-type Si wafers (0.8 to 1.0 mΩ·cm resistivity, B-doped, from Siltronix Corp., Archamps, France) are electrochemically etched in a 3:1 (v/v) solution of aqueous HF (48%, Merck, Whitehouse Station, NJ, USA) and ethanol (99.9%, Merck) at a constant current density of 385 mA cm−2 for 30 s. Si wafers with an exposed area of 1.33 cm2 are contacted on the backside with a strip of aluminum foil and mounted in a Teflon etching cell; a platinum mesh is used as the counterelectrode. After etching, the surface of the wafer is rinsed with ethanol several times and dried under a dry nitrogen gas. The freshly-etched PSi samples are thermally oxidized in a tube furnace (Thermolyne) at 800°C for 1 h in ambient air, resulting in a PSiO2 layer.
All materials were purchased from Sigma Aldrich Chemicals (St. Louis, MO, USA) unless mentioned otherwise.
Preparation of enzyme-DNA conjugates
To prepare the enzyme-DNA conjugate, 100 μL of a 100-μM solution of 5′-thiol-modified single-stranded oligonucleotide (cD1 sequence) in TE buffer (10-mM Tris and 1-mM EDTA) is mixed with 60 μL 1,4-dithiothreitol (1 M) and incubated overnight at 37°C. HRP type VI (0.92 mg) is dissolved in 200 μL of 50-mM phosphate buffered saline (PBS, pH 7.4) and incubated for 1 h at 37°C with sulfo-succinimidyl-4-(N-maleimido-methyl)cyclohexane-1-carboxylate (sulfo-SMCC) obtained from Thermo Scientific Pierce Protein Biology Products, Rockford, IL USA (2 mg in 60 μL of N,N-dimethylformamide). Both the DNA and the protein reaction mixtures are purified by two consecutive gel-filtration chromatography steps using NAP5 and NAP10 columns (Pharmacia LKB Biotechnology AB, Uppsala, Sweden). The purified DNA and protein solutions are combined and incubated in the dark at room temperature for 3 h. The reaction mixture is concentrated to approximately 500 μL by ultrafiltration (Centricon 30, Millipore Co., Billerica, MA, USA), and the buffer is changed to Tris (20-mM, pH 8.3) during this step. The conjugate is purified by anion exchange chromatography on a MonoQ HR 5/5 column (Pharmacia) using linear gradient over 25 min (AKTATM purifier, Amersham Biosciences, Piscataway, NJ, USA; buffer A 20-mM Tris, pH 8.3 and buffer B 20-mM Tris and 1.5-M NaCl, pH 8.3). The final concentration is determined spectrophotometrically.
Biofunctionalization of PSiO2
The PSiO2 films are first immersed in a solution of 3-glycidoxypropyl(trimethoxy)silane (GPTS) dissolved in toluene (90 mM) for 2 h. The samples are then extensively rinsed with toluene, ethanol, and acetone and dried under a nitrogen gas. The sequence of the capture strand is 5′-amino TCCTGTGTGAAATTGTTATACGCC-3′ (aD1). A solution of the amino-modified probe (100 μM) is applied onto the silanized PSiO2 surface and incubated for 2 h in a humidity chamber, followed by a post-cleaning process. Afterwards, 2.6-μM of the complimentary strand (cD1)-modifiedHRP conjugates are incubated onto the PSiO2 for 30 min. Finally, the PSiO2 samples are rinsed with 50-mM PBS, soaked in the buffer for 20 min, and vigorously rinsed again with PBS to remove any unbounded species from the surface. All processes are carried out at a room temperature (RT), below the melting temperature of the DNA (65.6°C). Mild basic conditions are used for dissociation of the hybridized complex (0.1-M NaOH for 5 min) to allow surface regeneration.
Fluorescent labeling and fluorescence microscopy
Fluorescently labeled (5′-TAMRA-modified) complimentary strand (TAMRA-cD1, 1 μM) is used to confirm DNA hybridization onto the modified PSiO2 surface Following the introduction the fluorescently tagged strand, the PSiO2 samples are characterized using TIRF iMIC microscope, and images are taken using interline transfer CCD (Andor Clara E, Till Photonics, Munich, Germany) and fast filter-based illumination system with 488 nm TIRF laser beam or the oligochrome light. Data are analyzed by LA live acquisition software.
Interferometric reflectance spectra of PSiO2 samples are collected using an Ocean Optics CCD USB 4000 spectrometer (Dunedin, FL, USA) fitted with a microscope objective lens coupled to a bifurcated fiber optic cable. A tungsten light source was focused onto the center of the sample surface with a spot size approximately 1 to 2 mm. Reflectivity data are recorded in the wavelength range of 400 to 1,000 nm, with a spectral acquisition time of 100 ms. Both illumination of the surface and detection of the reflected light are performed along an axis coincident with the surface normal. All the optical experiments are conducted in a fixed cell in order to assure that the sample’s reflectivity is measured at the same spot during all the measurements. All optical measurements are collected in aqueous surrounding. Spectra are collected using a CCD spectrometer and analyzed by applying fast Fourier transform, as previously described[15, 16].
Enzymatic activity of HRP
Ampliflu Red stock solutions are prepared according to the manufacturer’s instructions using 50-mM PBS buffer (pH 7.4). Final concentrations of 1-mM H2O2 and 0.1-mM Ampliflu Red are used to characterize the HRP activity levels. Solutions of 200 μL are placed on the HRP-modified PSiO2 samples, and the reaction progress is monitored for 8 min at RT. The fluorescence values of the reaction product resorufin are recorded at 590 nm, using an excitation wavelength of 530 nm.
The relative activity is calculated by the following relationship:
Optical sensing of HRP activity
The PSiO2 is washed with 50-mM PBS buffer solution (pH 7.4) for 30 min. Then, 0.8-mM of 4-chloro-1-naphthol in PBS buffer is introduced and continually cycled through the flow cell for 20 min. Finally, 0.16-M H2O2 is added to the cycled solution for HRP surface activation. The reflectivity spectra of the sample are recorded throughout the experiment.
Results and discussion
Biofunctionalization of PSiO2 with DNA-enzyme conjugates
The PSiO2 surfaces are prepared from a highly doped p-type single-crystal Si wafer, polished on the <100 > face using an anodic electrochemical etch. The resulting nanostructure is then thermally oxidized to generate a stable and a more hydrophilic scaffold. The structural properties are as previously described by Massad-Ivanir et al.. Briefly, the porous layer is 7,880 ± 60 nm thick with interconnecting cylindrical pores ranging in diameter from 60 to 100 nm, and the calculated porosity is approximately 80%. The semisynthetic approach for anchoring DNA-protein conjugates onto the PSiO2 surface is based on a well-established methodology of DNA-directed immobilization to solid surfaces, e.g., gold, glass, and polymers[9, 12]. The detailed synthesis is schematically outlined in Figure1a. First, the thermally oxidized nanostructure is epoxy-silanized with GPTS to obtain an activated surface for grafting of amine-modified single-stranded capture DNA (aD1). The complimentary thiolated oligonucleotide strand (cD1) is cross-linked to the HRP using sulfo-SMCC bi-functional linker containing NHS and maleimide moieties. In the final step, the resulting DNA-enzyme (HRP-cD1) conjugates are hybridized with the capture probe to enable their immobilization onto the PSiO2 surface. Hybridization is confirmed by studying the annealing of a fluorescently labeled complimentary DNA strand to the aD1-modified PSiO2. Figure1b depicts a fluorescence microscope image of aD1-modified PSiO2 surface following exposure to the TAMRA-cD1, revealing a large number of small fluorescent regions on the PSiO2 surface. In a control experiment, the silanization step is omitted from the conjugation scheme, and the PSiO2 is exposed to TAMRA-cD1 only. In this case, no florescence signal is observed (Figure1c), confirming that there is no or negligible interaction of the TAMRA-cD1 with PSiO2 surface in the absence of the immobilized aD1. Thus, these experiments demonstrate that the presence of the complementary capture strand is necessary for the immobilization of the TAMRA-cD1 onto the biosensing platform.
Reflective interferometric Fourier transform spectroscopy
Reflective interferometric Fourier transform spectroscopy (RIFTS) is used as a complimentary tool to monitor the optical changes occurring during the biofunctionalization steps onto of the PSiO2 surface. This method presents high sensitivity to small changes in the average refractive index of the porous thin film, allowing for direct and real-time monitoring the binding of different species to the pore walls[1, 3, 5, 7, 8]. The reflectivity spectrum of the thin PSiO2 film consists of a series of interference fringes that result from a Fabry-Pérot interference. This fringe pattern arises from reflections at the top and at the bottom of the film so that the measurement is made over the entire volume of the system. The effective optical thickness (EOT) refers to the 2 nL term in the Fabry-Pérot formula (where n is the average refractive index; L, the thickness of the film; and λ, the wavelength of the incident light). A change in the average refractive index leads to a shift in the observed reflectivity spectrum that correlates with EOT changes. It is expected that the chemical modification of the porous nanostructure (as previously outlined in Figure1a) will result in a redshift of the EOT due to the increase in the average refractive index upon attachment of different species to the pore walls. It should be noted that the nanostructure is designed to allow proper infiltration of the DNA conjugates (approximate size of 10 nm) into the pores, characterized by an average diameter of 80 nm. Indeed, significant EOT changes are observed after each of the described immobilization steps, see Figure2a. Following the grafting of aD1 to the epoxy-functionalized PSiO2, an EOT increase of 49 ± 1 nm is detected. DDI of the HRP-cD1 conjugates (230 ng in 2 μL volume) causes an additional EOT increase of 85 ± 17 nm. Additionally, the specificity of the hybridization is validated by addition of non-modified HRP to the aD1-modified PSiO2, resulting in insignificant EOT changes (Figure2b). Thus, the RIFTS results further confirm that the enzyme immobilization onto the PSiO2 surface occurs through Watson-Crick base pairing.
Enzymatic activity assays
The enzymatic activity of the anchored enzymes onto the porous scaffold is studied by monitoring the oxidation products of HRP (Figure3d). The modified PSiO2 samples are exposed to a substrate solution of Ampliflu Red in PBS, and the collected solution is spectrophotometrically analyzed. Figure3b depicts the high relative activity (74%) of the immobilized conjugates compared to non-modified HRP activity in a solution (Equation 1). Thus, the modified enzymes retain their specificity and activity once anchored and confined on the porous support. An important advantage of the DDI anchoring is the ability to regenerate the surface, as schematically shown in Figure3a, by applying mild dehybridization conditions, e.g., pH change or temperature increase (above the melting temperature of the DNA pair). Indeed, following a mild-base wash, an insignificant relative enzymatic activity value of less than 3% is attained (Figure3c), indicating that the PSiO2 surface can be regenerated. In addition, a consecutive cycle of hybridization/dehybridization is carried out to demonstrate the reversibility of DDI method for the characterization of small aliquots (2 μL) of the recovered enzyme and its reuse. These experiments show the high reversibility and reproducibility of the immobilization strategy as relative activity values of 49% and less than 3% are recorded, followed by DDI and dehybridization processes, respectively (Figure3b,c).
Optical detection of enzymatic activity
Previous sections have demonstrated that the DNA-HRP conjugates remain catalytically active after the DDI onto the PSiO2 nanostructure. Next, we investigated the potential of this platform to act as an optical biosensor for monitoring enzymatic activity through RIFTS experiments. Thus, HRP-modified PSiO2 is fixed in a flow cell setup and is exposed to various substrate/buffer combinations. The reactions are monitored in real time by acquisition of the reflectivity spectra of the porous thin film. The recorded EOT values prove a direct measure of the amount of enzymatic activity products infiltrating the pores, as previously shown by Orosco et al.. Figure4 depicts the EOT change of the HRP-modified nanostructure following the introduction of 4-chloro-1-naphthol, which oxidizes in the presence of peroxidases into insoluble 4-chloro-1-naphton (Figure4, inset). A rapid increase of 90 nm in the EOT value is observed after injection of 0.16-M H2O2 to the cycled solution (Figure4b). The EOT increase is attributed to infiltration and accumulation of the oxidation products in the pores as the enzymatic reaction occurs. Control experiments with bare and only aD1-modified PSiO2 (no immobilized enzyme) exposed to the same conditions exhibit insignificant changes in EOT (data not shown), indicating that the biosensor platform is indeed specific for monitoring the enzymatic activity products.
We demonstrate that DNA-directed protein immobilization is an elegant and facile method for specific and reversible anchoring of a model enzyme, i.e., HRP onto PSiO2 Fabry-Pérot thin films. HRP specific immobilization through Watson-Crick base pairing onto the porous nanostructure is confirmed by both fluorescence microscopy and RIFTS. The surface-immobilized HRP retains relatively high enzymatic activity in comparison to its activity in solution. We show that the catalytic activity of the HRP immobilized within the PSiO2 thin film can be monitored in real time by RIFTS technique. For biosensor design, the DDI method allows the use of small enzyme quantities for monitoring the reaction while allowing both enzyme and surface to be regenerated for subsequent usage. This ‘proof-of-concept’ biosensor scheme can be potentially extended for systematic analysis of the enzyme of interest under unlimited experimental setups.
Jane A, Dronov R, Hodges A, Voelcker NH: Porous silicon biosensors on the advance. Trends Biotechnol 2009, 27(4):230–239. 10.1016/j.tibtech.2008.12.004
DeLouise LA, Kou PM, Miller BL: Cross-correlation of optical microcavity biosensor response with immobilized enzyme activity. Insights into biosensor sensitivity. Anal Chem 2005, 77(10):3222–3230. 10.1021/ac048144+
Sailor MJ, Link JR: “Smart dust”': nanostructured devices in a grain of sand. ChemCommun 2005, 11: 1375–1383.
Rong G, Najmaie A, Sipe JE, Weiss SM: Nanoscale porous silicon waveguide for label-free DNA sensing. BiosensBioelectron 2008, 23(10):1572–1576. 10.1016/j.bios.2008.01.017
Pacholski C, Sartor M, Sailor MJ, Cunin F, Miskelly GM: Biosensing using porous silicon double-layer interferometers: Reflective interferometric Fourier transform spectroscopy. J Am ChemSoc 2005, 127(33):11636–11645. 10.1021/ja0511671
Sweetman MJ, Ronci M, Ghaemi SR, Craig JE, Voelcker NH: Porous silicon films micropatternedwith bioelementsas supports for mammalian cells. AdvFunct Mater 2012, 22: 1158–1166.
Orosco MM, Pacholski C, Sailor MJ: Real-time monitoring of enzyme activity in a mesoporous silicon double layer. Nat Nanotechnol 2009, 4(4):255–258. 10.1038/nnano.2009.11
Kilian KA, Boecking T, Gaus K, Gal M, Gooding JJ: Peptide-modified optical filters for detecting protease activity. ACS Nano 2007, 1(4):355–361. 10.1021/nn700141n
Fruk L, Mueller J, Weber G, Narvaez A, Dominguez E, Niemeyer CM: DNA-directed immobilization of horseradish peroxidase-DNA conjugates on microelectrode arrays: towards electrochemical screening of enzyme libraries. Chemistry-a, European Journal 2007, 13(18):5223–5231. 10.1002/chem.200601793
Frasconi M, Mazzei F, Ferri T: Protein immobilization at gold-thiol surfaces and potential for biosensing. Anal BioanalChem 2010, 398(4):1545–1564.
Thust M, Schoning MJ, Schroth P, Malkoc U, Dicker CI, Steffen A, Kordos P, Luth H: Enzyme immobilisation on planar and porous silicon substrates for biosensor applications. J MolCatal B: Enzym 1999, 7(1–4):77–83.
Niemeyer CM: Semisynthetic DNA-protein conjugates for biosensingand nanofabrication. AngewChemInt Ed 2010, 49(7):1200–1216.
Azevedo AM, Martins VC, Prazeres DM, Vojinovic V, Cabral JM, Fonseca LP: Horseradish peroxidase: a valuable tool in biotechnology. BiotechnolAnnu Rev 2003, 9: 199–247.
Veitch NC: Horseradish peroxidase: a modern view of a classic enzyme. Phytochemistry 2004, 65(3):249–259. 10.1016/j.phytochem.2003.10.022
Massad-Ivanir N, Shtenberg G, Tzur A, Krepker MA, Segal E: Engineering nanostructured porous SiO(2) surfaces for bacteria detection via “Direct Cell Capture”. Anal Chem 2011, 83(9):3282–3289. 10.1021/ac200407w
Massad-Ivanir N, Shtenberg G, Zeidman T, Segal E: Construction and characterization of porous SiO(2)/hydrogel hybrids as optical biosensors for rapid detection of bacteria. AdvFunct Mater 2010, 20(14):2269–2277.
Segal E, Perelman LA, Cunin F, Di Renzo F, Devoisselle JM, Li YY, Sailor MJ: Confinement of thermoresponsive hydrogels in nanostructured porous silicon dioxide templates. AdvFunct Mater 2007, 17(7):1153–1162.
Loew N, Bogdanoff P, Herrmann I, Wollenberger U, Scheller FW, Katterle M: Influence of modifications on the efficiency of pyrolysedCoTMPP as electrode material for horseradish peroxidase and the reduction of hydrogen peroxide. Electroanalysis 2006, 18(23):2324–2330. 10.1002/elan.200603664
Kumada Y, Maehara M, Tomioka K, Katoh S: Liposome immunoblotting assay using a substrate-forming precipitate inside immunoliposomes. BiotechnolBioeng 2002, 80(4):414–418.
Fortin E, Mailley P, Lacroix L, Szunerits S: Imaging of DNA hybridization on microscopic polypyrrole patterns using scanning electrochemical microscopy (SECM): the HRP bio-catalyzed oxidation of 4-chloro-1-naphthol. Analyst 2006, 131(2):186–193. 10.1039/b504711k
ES acknowledges the financial support of the NEVET program administered by the Russell Berrie Nanotechnology Institute and by the Marie Curie Reintegration Grant (NANOPACK) administered by the European Community. GS acknowledges the Miriam and Aaron Gutwirth Excellence Scholarship Award. This work was also supported by Weizmann-Technion-KIT Start up grant and DFG-CFN Excellence Initiative Project A5.7.
The authors declare that they have no competing interests.
GS carried out PSi synthesis, enzyme immobilization, enzyme activity assays, biosensing experiments, and data analysis. He also wrote the manuscript. NMI contributed to the conception of the experiments and was involved in the synthesis and characterization of PSi. SE synthesized the DNA-enzyme conjugates. MS participated in the design of the study. LF conceived the study and coordinated the synthesis and characterization of DNA-enzyme conjugates. ES conceived and coordinated the study, participated in the design of the study and data analysis, and drafted the manuscript. All authors read and approved the final manuscript.