- Nano Express
- Open Access
Biofunctionalization of zinc oxide nanowires for DNA sensory applications
Nanoscale Research Letters volume 6, Article number: 511 (2011)
We report on the biofunctionalization of zinc oxide nanowires for the attachment of DNA target molecules on the nanowire surface. With the organosilane glycidyloxypropyltrimethoxysilane acting as a bifunctional linker, amino-modified capture molecule oligonucleotides have been immobilized on the nanowire surface. The dye-marked DNA molecules were detected via fluorescence microscopy, and our results reveal a successful attachment of DNA capture molecules onto the nanowire surface. The electrical field effect induced by the negatively charged attached DNA molecules should be able to control the electrical properties of the nanowires and gives way to a ZnO nanowire-based biosensing device.
Semiconductor nanowires have gained large interest as building blocks for low-cost, highly sensitive biosensors [1, 2]. Due to the quasi-one-dimensional geometry of the nanowires and the large surface-to-volume ratio, surface-induced effects play a significant role on the electrical properties of nanowire-based devices. Even a single molecule attached to the nanowire surface is able to change the electrical properties of the nanowire considerably. Therefore, a functionalization of the nanowire surface gives way to highly sensitive sensors that can be arranged in a very dense assembly, owing to their nano-sized dimension. However, both the surface modification and the nanowire device arrangement have to be taken care of in order to prepare a complete nanowire-based DNA sensor.
During the last decade, there have been several studies concentrating on the development of Si-based nanowire sensors [1–3]. Si nanowires are complementary metal oxide semiconductor (CMOS) compatible and biocompatible, and techniques for the functionalization of Si are well understood. Although it is not CMOS compatible, ZnO is very stable under ambient conditions and compared to silicon especially its surface is stable under oxygen-rich conditions. The stability of ZnO nanostructures under physiological conditions, which is important for biosensing applications, depends on the crystal quality of the nanostructures but can be assumed as sufficient for structures grown by thermal evaporation methods [4–6]. The material is also biocompatible, non-toxic, and easy available. Nanostructures made of ZnO are easy and reliable to produce in a wide manner of different forms and structures [7, 8]. The DNA capture molecule immobilization with organosilanes has been successfully shown by Corso and co-workers on planar ZnO surfaces , where the biomolecule layer was used to act as an acoustic wave sensor. With the use of ZnO nanowires instead of planar films, the metal oxide itself can be used to build an electrically working biosensor. Biosensors based on ZnO nanostructures have been reported, using both electrostatic adsorption as well as organosilane modification with subsequent covalent binding for immobilization [10–13]. Various enzymes have been immobilized using electrostatic adsorption in order to realize highly selective bioassays [11–13]. Recently, the biofunctionalization of ZnO nanowires with biotin for streptavidin detection has been shown using organosilanes with aldehyde functionality that bind the amino group of biotin . The nanowire-based protein sensors could detect streptavidin binding down to a concentration of 2.5 nmol, underlining the capability of ZnO nanowires for the electrical detection of biomolecules. Hereby the nanowire has the character of an active channel in a field effect transistor whose conductivity is governed by the field effect induced by the assembly of charged target molecules on the semiconductor surface.
In this study, we will extend the successful biofunctionalization of ZnO nanowire surfaces to DNA using the organosilane glycidyloxypropyltrimethoxysilane (GOPS) [14–16]. DNA molecules are negatively charged and therefore applicable for the electrical detection with biofunctionalized nanowires. In contrast to the detection of streptavidin in , where the current increases when streptavidin is attached, the current through the intrinsically n-type ZnO nanowire should decrease as the negatively charged DNA target molecules induce a depletion zone inside the nanowire.
The ZnO nanowires have been grown via vapor-liquid-solid mechanism in a horizontal tube furnace  at a pressure of 150 mbar with a growth temperature of 1,050°C. The nanowires evolve in a typical spaghetti-like structure with wire diameters around 100 nm and wire lengths up to some tens of micrometers. To remove adsorbed species from the nanowires and supply a clean and reactive ZnO surface, the samples have been oxygen-plasma-treated for 30 min at 5 Pa oxygen pressure with a plasma energy of 50 W. As this treatment is known to enhance the dissociative adsorption of water on the ZnO surface , the samples have been stored in a cabinet dryer at 100°C for at least 5 min before the silane treatment to remove water residues from the surface.
Subsequent silanization took place in 10 mM GOPS in a water-free toluene solution (for details on chemicals resource, see Additional file 1). The silanization mechanism is displayed in Figure 1a. The samples have been incubated stirring constantly for at least 6 h at 70°C. The samples have been rinsed three times subsequently with pure toluene for 5 min in each case and then dried with compressed air.
The 5'-amino-modified oligonucleotides were dissolved in 5 × PBS buffer (pH 7.4) with a concentration of 10 μmol for the biofunctionalization. The single-stranded DNA sequences of the applied oligonucleotides consisting of 27 bases are shown in Table 1. The fluorescence markers that are linked to the 3'-end and enable the detection of the molecules with fluorescence microscopy are also listed in Table 1. The DNA solution was pipetted onto the nanowire samples and incubated overnight under wet conditions to immobilize the nucleotides on the GOPS surface via the 5'-amino linker (see Figure 1b). Afterward, the samples were rinsed for 10 min in 15 mmol Tris-HCl buffer (pH 8) in order to get rid of unbound DNA and then dried with compressed air.
To ensure covalent binding following the scheme in Figure 1 takes place, control samples have been prepared both leaving out the GOPS silanization step and with DNA that does not have an amino linker. The biofunctionalized nanowires were mechanically transferred to silicon or glass substrates by a gentle pressure imprint of the growth substrate.
The as-grown nanowires have been characterized with a JEOL JSM-6490 scanning electron microscope. Subsequently to the biofunctionalization, the samples were investigated with a Zeiss Axio Imager 2 fluorescence microscopy setup. Fluorescence microscopy is known as an adequate tool for the analysis of DNA monolayers on thin film surfaces as well as on nanowires [9, 19]. The microscope makes use of a filter cube to detect marker-specific fluorescence. The samples marked with cyanine 3 (Cy3) dyes turned out to be more photo stable than the fluorescein isothiocyanate (FITC)-marked samples. Thus, we will present here mainly Cy3-marked samples.
Results and discussion
Dark field and fluorescence images of biofunctionalized ZnO nanowires are shown in Figure 2a,b,c,d. One can clearly see that every nanowire that can be identified in the dark field image is showing a fluorescence signal. However, the luminescence intensities differ extremely for the investigated wires. This can be explained by the fact of different diameters of the nanowires and thus different nanowire surface areas. The intensity of the emitted light is also appearing non-uniformly along the nanowire axis, as clearly visible on the wire highlighted in Figure 2d. These intensity fluctuations might be owing to only fragmentary DNA coverage or variations of the nanowire thickness. In Figure 3b, the fluorescence intensity along the nanowire axis (dotted line) in Figure 3a is shown. It is clearly visible that the fluorescence intensity is not only fluctuating but even disappearing in some regions of the wire. This leads to the assumption that the functionalized nanowire might not be completely covered with DNA.
In Figure 3c,d, detailed scanning electron microscope (SEM) pictures of a typical ZnO wire used in this study are shown. One can see that the wire itself has a non-uniform thickness, varying up to a factor of 2. The detailed surface morphology of the functionalized wires is not clearly resolvable within an SEM; however, a uniform coverage of the nanowire is noticed. A respective SEM image can be found in the supplementary information (Additional file 1). Thus, we can also trace back a major distribution to the nanowire intensity fluctuations to the thickness variations along the wire axis. To confirm this estimation, we also functionalized a single crystalline ZnO bulk sample and investigated the DNA surface coverage. The sample is showing a homogeneous fluorescence of the functionalized area (not shown here, see Additional file 1), underlining that the GOPS treatment is applicable for the successful accumulation of DNA monolayer to ZnO surfaces.
The observed thickness variations might result from furnace-related instabilities of the growth conditions. With a scaled-up and improved setup, it is possible to overcome this issue easily .
However, it is possible that due to the uneven nanowire surface of the samples, a uniform coverage of the nanowire with DNA molecules might be hampered. Nanowires sticking together during the silanization process could also lead to a non-uniform DNA coverage. Additionally, damages of the DNA layer during the imprint could result in the same layer inhomogeneity. Nanowires grown from a seed array  could be used to avoid non-uniform coverage due to shadowing effects and facilitate a non-destructive nanowire imprint process. Therefore, the intensity fluctuations of the biofunctionalized nanowires can be explained by the interplay of nanowire thickness variations and non-homogeneous surface coverage. Recourse to either can be solved using a more advanced nanowire growth setup than the one utilized here.
As ZnO nanostructures are known to show a green defect luminescence that can be dramatically enhanced when the nanowires are coated , one has to check if the wires themselves might cause a significant luminescence signal that could be interpreted falsely as fluorescence. Therefore, all samples have been examined with different band pass fluorescence filters. All samples only showed fluorescence at wavelengths referable to the specific dye used for the biofunctionalization; a broader defect luminescence was not detected.
Additionally, necessary reference experiments have been performed with untreated ZnO wires as well as nanowires, which were silanized but not biofunctionalized (with DNA). Figure 4 confirms the absence of autofluorescence or luminescence of the nanowires.
It is also known that ZnO nanostructures act fluorescence enhancing themselves through affecting the self-quenching properties of fluorophores . This could lead to fluorescent wires on top of a dye-covered substrate. As mentioned already above, the wires in our study were first functionalized and then subsequently transferred to a clean and dye-free substrate. Thus, fluorescence enhancement of substrate-bonded fluorescence markers can also be excluded as the origin of the observed fluorescence.
Upon having clarified that the observed fluorescence is caused by DNA attached to the ZnO nanowires, the question regarding the character and stability of this attachment still remains. To investigate these issues, several control samples have been prepared. In Figure 5, a typical fluorescence image of a silanized and biofunctionalized nanowire (a) is compared to an image of a nanowire that was treated the same way, but leaving out the silanization step and using DNA without a 5'-amino linker (b). One can see that the observed luminescence appears to be orders of magnitude weaker in the latter case. In Figure 5c, the fluorescence intensities of various control samples are compared. To quantify the intensities of different fluorescent samples, all signals have been integrated for different lengths of time and the resulting apparent magnitudes have been classified into six levels of fluorescence intensity between no fluorescence at all and fluorescence saturation. It turns out that the fluorescence is most pronounced in the case of GOPS treatment and DNA with amino linker. All the other control samples show significant less fluorescence, indicating that the strongest binding of the DNA to the nanowire is only achieved with both coupling groups present (epoxy group at GOPS and amino group at DNA) in order to form a covalent binding.
In Figure 5d, a comparison of a sample with GOPS and a sample without GOPS is presented. Both samples were biofunctionalized with DNA with amino linker. The samples have been rinsed in Tris-HCl buffer solution for 10 min and then measured. As expected, the silanized sample is showing the stronger fluorescence. However, after rinsing both samples for another 12 h, the fluorescence of the sample silanized with GOPS and then functionalized has not dropped, whereas the fluorescence of the control sample is less present than before. This also indicates a comparatively stable, presumably covalent bond between the DNA and the nanowire following the reaction scheme in Figure 1. In conclusion, the stable biofunctionalization of ZnO nanowires has been clearly demonstrated. The bifunctional linker GOPS was used to immobilize a monolayer of DNA capture molecules on the ZnO nanowires. The successful functionalization could be verified with fluorescence microscopy. Variations of the nanowire thickness result in fluorescence variations along the nanowire axes. The functionalized wires may be used as building blocks for electrically driven DNA target molecule detection.
Cui Y, Wei Q, Park H, Lieber CM: Nanowire nanosensors for highly sensitive and selective detection of biological and chemical species. Science 2001, 293: 1289–1292. 10.1126/science.1062711
Patolsky F, Timko BP, Zheng G, Lieber CM: Nanowire-based nanoelectronic devices in the life sciences. MRS Bull 2007, 32: 142–149. 10.1557/mrs2007.47
Cattani-Scholz A, Pedone D, Dubey M, Neppl S, Nickel B, Feulner P, Schwartz J, Abstreiter G, Tornow M: Organophosphonate-based PNA-functionalization of silicon nanowires for label-free DNA detection. ACS Nano 2008, 2: 1653–1660. 10.1021/nn800136e
Zhou J, Xhu NS, Wang ZL: Dissolving behavior and stability of ZnO wires in biofluids: a study on biodegradability and biocompatibility of ZnO nanostructures. Adv Mater 2006, 18: 2432–2435. 10.1002/adma.200600200
Cheng C, Xin R, Leng Y, Yu D, Wang N: Chemical stability of ZnO nanostructures in simulated physiological environments and its application in determining polar directions. Inorg Chem 2008, 47: 7868–7873. 10.1021/ic8005234
Israr MQ, Sadaf JR, Nur O, Willander M, Salman S, Danielsson B: Chemically fashioned ZnO nanowalls and their potential application for potentiometric cholesterol biosensor. Appl Phys Lett 2011, 98: 253705. 10.1063/1.3599583
Wang ZL: Zinc oxide nanostructures: growth, properties and applications. J Phys Condens Matter 2004, 16: R829-R858. 10.1088/0953-8984/16/25/R01
Huang MH, Wu Y, Feick H, Tran N, Weber E, Yang P: Catalytic growth of zinc oxide nanowires by vapor transport. Adv Mater 2001, 13: 113–116. 10.1002/1521-4095(200101)13:2<113::AID-ADMA113>3.0.CO;2-H
Corso CD, Dickherber A, Hunt WD: An investigation of antibody immobilization methods employing organosilanes on planar ZnO surfaces for biosensor applications. Biosens Bioelectron 2008, 24: 805–811. 10.1016/j.bios.2008.07.011
Choi A, Kim K, Jung HI, Lee SY: ZnO nanowire biosensors for detection of biomolecular interactions in enhancement mode. Sens Actuators B 2010, 148: 577–582. 10.1016/j.snb.2010.04.049
Fulati A, Ali SMU, Asif MH, Alvi NH, Willander M, Brännmark C, Stralfors P, Börjesson SI, Elinder F, Danielsson B: An intracellular glucose biosensor based on nanoflake ZnO. Sens Actuators B 2010, 150: 673–680. 10.1016/j.snb.2010.08.021
Ali SMU, Alvi NH, Ibupoto Z, Nur O, Willander M, Danielsson B: Selective potentiometric determination of uric acid with uricase immobilized on ZnO nanowires. Sens Actuators B 2011, 152: 241–247. 10.1016/j.snb.2010.12.015
Lin SS, Chen IC, Yang J, Hsueh TJ, Hsu CL, Lee HE, Shieh TY: A study on one-step immobilization of horse immunoglobulin with vertically grown ZnO nanorods substrates. J Electrochem Soc 2011, 158: K107-K111. 10.1149/1.3559465
Festag G, Steinbrück A, Wolff A, Csaki A, Möller R, Fritzsche W: Optimization of gold nanoparticle-based DNA detection for microarrays. J Fluoresc 2005, 15: 161–170. 10.1007/s10895-005-2524-4
Southern EM, Case-Green SC, Elder JK, Johnson M, Mir KU, Wang L, Williams JC: Arrays of complementary oligonucleotides for analysing the hybridisation behaviour of nucleic acids. Nucl Acids Res 1994, 22: 1368–1373. 10.1093/nar/22.8.1368
Lamture JB, Beattie KL, Burke BE, Eggers MD, Ehrlich DJ, Fowler R, Hollis MA, Kosicki BB, Reich RK, Smith SR: Direct detection of nucleic acid hybridization on the surface of a charge coupled device. Nucl Acids Res 1994, 22: 2121–2125. 10.1093/nar/22.11.2121
Borchers C, Müller S, Stichtenoth D, Schwen D, Ronning C: Catalyst-nanostructure interaction in the growth of 1-D ZnO nanostructures. J Phys Chem B 2006, 110: 1656–1660. 10.1021/jp054476m
Ra HW, Khan R, Kim JT, Kang BR, Bai KH, Im YH: Effects of surface modification of the individual ZnO nanowire with oxygen plasma treatment. Mater Lett 2009, 63: 2516–2519. 10.1016/j.matlet.2009.08.054
Byun KE, Heo K, Shim S, Choi HJ, Hong S: Functionalization of silicon nanowires with actomyrosin motor protein for bioinspired nanomechanical applications. Small 2009, 5: 2659–2664. 10.1002/smll.200900964
Fan HJ, Werner P, Zacharias M: Semiconductor nanowires: from self-organization to patterned growth. Small 2006, 20(6):700–717.
Richters JP, Dev A, Müller S, Niepelt R, Borschel C, Ronning C, Voss T: Influence of metallic coatings on the photoluminescence properties of ZnO nanowires. Phys Status Solidi RRL 2009, 3: 166–168. 10.1002/pssr.200903176
Hu W, Liu Y, Zhu Z, Yang H, Li CM: Randomly oriented ZnO nanorods as advanced substrate for high-performance protein microarrays. ACS Appl Mater Interfaces 2010, 2: 1569–1572. 10.1021/am100314w
We thank Marc Brötzmann, University of Göttingen, for advice and discussion. We thank Christian Leiterer, IPHT Jena, for assistance with both fluorescence microscopy and immobilization protocols. Funding by BMBF (16SV5386K, "NAWION") and EU (Marie Curie ITN 265073, "Nanowiring") is acknowledged.
The authors declare that they have no competing interests.
US and IS synthesized and characterized the nanowires and conducted the fluorescence microscopy measurements. RN assisted with the nanowire synthesis and drafted the manuscript. JS participated in the fluorescence microscopy measurements and helped to draft the manuscript. BR and BS carried out the biofunctionalization and assisted with the fluorescence microscopy measurements. RM and AC participated in the design of the study and its coordination. CR and WF participated in the design of the study and helped to draft the manuscript. All authors read and approved the final manuscript.
Raphael Niepelt, Ulrich C Schröder, Jana Sommerfeld contributed equally to this work.
About this article
Cite this article
Niepelt, R., Schröder, U.C., Sommerfeld, J. et al. Biofunctionalization of zinc oxide nanowires for DNA sensory applications. Nanoscale Res Lett 6, 511 (2011). https://doi.org/10.1186/1556-276X-6-511
- zinc oxide
- fluorescence microscopy
- sensor technology