Skip to main content
Applied Physics Letters logoLink to Applied Physics Letters
. 2009 Mar 23;94(12):122104. doi: 10.1063/1.3103616

Solid state nanogaps for differential measurements of molecular properties

Benjamin Moody 1,a), Gregory S McCarty 1,b)
PMCID: PMC3645910  PMID: 23696694

Abstract

This paper demonstrates the production and probing of solid state nanogaps. These nanogaps can be inexpensively and controllably produced using a combination of molecular and standard photolithography. These nanogaps are implemented for chemical monitoring by using surface enhanced Raman spectroscopy to collect molecular information at the nanogap and current-voltage traces to probe the charge transport of the nanogap. These data show that the oligonucleotides used as the molecular resist are degraded, that some of the degraded oligonucleotides are removed, and then new oligonucleotides are adsorbed.


Solid state nanogaps are scientifically interesting due to their small size, robustness, and versatility. Many insights in physics at the nanometer scale have been made using these types of structures and more are expected in the future. Practically, solid state nanogaps have the potential of detecting chemical species on the near single-molecule scale. This capability is beginning to be studied due to the importance of inexpensive chemical sensing.

Coincidentally, surface enhanced Raman spectroscopy (SERS) is an analytical technique of growing importance that also stands to benefit from the maturation of nanogap technologies. SERS is a variant of Raman spectroscopy that uses roughened metallic substrates to enhance, amplify, and otherwise refine its output signal. However, the difficulty that frequently arises with SERS is creating substrates that have large and very uniform enhancement factors. Ideally SERS substrates should be efficiently and inexpensively fabricated on the wafer scale and will consist of small metallic structures with uniform spacing from a few hundred nanometers to just a few nanometers. More routinely, however, SERS substrates are subject to local unpredictable “hot spots” of enhancement and require advanced nanolithographic patterning to prepare.1, 2, 3

Fortunately, the commingling of solid state nanogaps and SERS has increased recently and research is beginning to show that the closely spaced metal features at the nanogap are capable of enhancing the Raman effect.4, 5, 6 Such discoveries lead to the possibility of using nanogaps for dual function applications—to serve as an electronic detection device and as a SERS platform for chemical characterization.

In the past, nanogap structures have been fabricated with mechanically controlled break junctions,7, 8 nanowire lithography,9 and electron beam lithography with electromigration4, 10 among others.11 Each method has its own individual advantages and disadvantages though very few offer both the promise of nanoscopic gap-size control and the likelihood of inexpensive and efficient fabrication. In this project, emphasis will be placed on using a hybrid molecular technique to create planar electrodes with separations of about 20 nm. In the future, these structures will be invaluable for investigating molecular electronic candidates, for researching biological systems, and as a substrate for SERS studies. Here, as a proof of concept experiment, the local molecular environment of the nanogap is monitored using SERS and current-voltage traces immediately after fabrication, then again after an alkanethiol substitution, and finally after a subsequent oligo substitution.

Solid state nanogaps are generated using a variation in previously developed molecular resist strategies.12 These strategies have demonstrated the ability to use multilayer resists to create structures from just a few nanometers to 40 nm.13 The structures presented here are different in several ways from previous alkanethiol-based solid state nanogaps in that these structures are created with thicker single layer molecular resists and they maintained the capping metallic layer often sacrificed in other papers.

The fabrication methodology for these structures will be briefly explained. In this report, the initial electrode in the electrode pair that composes the nanogap is fabricated on a silicon wafer with 200 nm of silicon oxide (University Wafer) using a conventional photolithography lift-off process with SPR3012 (Rohm&Haas) and LOR5A (MicroChem) resists and then 3 nm of chrome and 40 nm of gold are deposited using electron beam evaporation. The photoresist and unwanted metal are removed with sonication in acetone and an immersion in CD-26 (MicroChem). Next, the electrode is submerged in 5μM solution of thiolated oligonucleotide (IDT) for 24 h. Finally, a second photolithographic lift-off process, metallic evaporation, and resist removal are used to pattern the second electrode in the electrode pair. These processes were similar to those used to pattern the initial electrode except 3 nm of chrome and 25 nm of gold were deposited. The oligo resist had the sequence 5-T10-GC AGC TTA GAA TCA AAT AGC GCG ATA TGC ATC GAT GAC TA-3 and a thiol modification at the 5 terminus. Research suggests an oligo this size should be about 20 nm in length.14 Scanning electron microscope (SEM) images were collected to characterize the electrode fabrication process (data not shown) and image analysis confirms that the size of the nanogap is within the expected range of 20±5 nm.

All Raman spectra presented in this paper were collected with a custom-built Raman microscope. Raman scattering was excited using a 12 mW, 632.8 nm HeNe laser (Thorlabs) coupled to an inverted microscope (Nikon, Diaphot) with a 100× (Nikon) dry objective. The reflected Raman signal was analyzed through an imaging spectrograph (PI Acton, SpectraPro SP-2156) and detected with a liquid nitrogen cooled charge-coupled device (CCD) camera (PI Acton, Spec-10:100BR/LN). The laser power at the sample measured 3 mW and the laser spot was 2μm in diameter. Collection times were 20 s. GRAMS/AI 8.0 software (Thermo) was used for analysis and correction.

The electronic properties of the nanogap were also collected as they provide a quick, qualitative measure of variation in the nanogap. While electronic property measurements are fast and inexpensive, they provide little molecular information. For this reason, SERS was also performed. The electronic properties and Raman spectra for these structures were recorded at three time points during the experiment: (1) immediately after fabrication, (2) after substitution of dodecanethiol (DDT) into the gap, and (3) after immersion in a 50-mer thiol terminated oligonucleotide. Note that the Raman information was collected in a confocal format at the nanogap enabling the data to be collected from nominally the same position during each step of the experiment.

Figure 1 shows portions of the Raman spectra from a representative solid state nanogap and Fig. 2 shows the current voltage traces for the same solid state nanogap at the same time points. The dark blue trace in Fig. 1 shows the as fabricated condition. Note that while spectra recorded away from the nanogap show little signal or perhaps small contributions from the Si substrate (data not shown), the portion of the spectrum from the nanogap shown in Fig. 1 has two strong peaks at 1342 and 1585 relative cm1. These peaks are very similar to those observed in pyrolized photoresist or for glassy carbon with two strong bands around 1360 relative cm1 [disordered (D) band] and 1600 relative cm1 [graphitic (G) band].15, 16 These features alone are typical of sp2 bonding within a graphitic carbon matrix whereas oligo systems typically have several additional characteristic peaks present.17, 18 This suggests that some of the oligonucleotide being used as a molecular resist degraded during the fabrication process. The dark blue trace in Fig. 2 shows the electronic properties of the as fabricated nanogap. Through SEM imaging, the separation of the nanogap was observed to be 20 nm with a roughness on the order of 5 nm. At this length scale, no charge transport is expected from ballistic tunneling12 but as can be seen in the current voltage trace, significant charge transport was observed for this system. It is expected that this charge transport was through the oligos or through the degraded oligos, which appear graphitic from the molecular information collected by Raman spectroscopy. Note that oligonucleotides and DNA once thought to be insulators have since been shown to enable long range charge transfer when dry, though the exact mechanism is still debated.19, 20

Figure 1.

Figure 1

Raman signal from a nanogap created using single-stranded oligonucleotides as a molecular resist in the structure’s fabrication. (a) shows a portion of the Raman spectra collected at the electrode interface as fabricated, after a DDT substitution, and then after thiol functionalized oligonucleotides (Oligos) were added to the solid state nanogap. (b) and (c) are the spectra that result from subtracting the as fabricated trace from the DDT trace and from subtracting the DDT trace from the oligonucleotide trace, respectively. These latter spectra are used to highlight the change in condition between two states.

Figure 2.

Figure 2

Current-voltage characteristics for the electrode as fabricated, after the DDT substitution, and then again after the final oligonucleotide addition. The electrode conducted 350 nA as fabricated, 18 nA after the alkane substitution, and 130 nA after the oligo substitution, all at +0.5 V of applied bias.

In an effort to remove some of the degraded oligonucleotide, the sample was immersed in a solution of 1 mM DDT in ethanol and heated at 60°C for 1 h. The sample was then slowly returned to room temperature over several hours. Then the Raman spectrum and electronic properties of the same nanogap were collected again. The results are shown in the brown trace of Fig. 1 for Raman spectroscopy and the brown current voltage traces in Fig. 2. Experiments in our laboratory have not shown significant characteristic SERS scattering from DDT. This is expected since Raman activity is enhanced in molecules with some π-bonding or with large cross-sectional areas.21, 22 Thus, because DDT is a straight chain, sp3 hybridized system, a great reduction in Raman activity is expected when it is used to replace the more complex and aromatic, π-bonded environment of the oligonucleotide system. From Fig. 1 it can be seen that Raman activity indeed dropped significantly after the alkanethiol substitution, including activity from the graphitic peaks. This point is highlighted specifically by subtracting the “as fabricated” trace from the “DDT” trace. The resulting Fig. 1b shows large negative peaks at 1342 and 1585cm1 that have been attributed to the D and G bands of carbon.15, 16 In Fig. 2 a significant reduction in the charge transfer through the nanogap is also shown. It can be deduced from this information that some (though not all) of the degraded oligonucleotide has been removed from the solid state nanogap. Repeated aggressive sonication in strong solvents like dimethylformamide can be used to remove more of the molecular species at the nanogaps, resulting in a Raman spectrum that is featureless except for a small peak at 530cm1 that represents the silicon substrate. Unfortunately, this process is time consuming and its adverse effects to the electrodes limit overall device yield.

Finally, the alkanethiol-substituted oligo sample was immersed in a 5μM aqueous solution of thiol modified 50-mer oligonucleotide and heated to 60°C for 1 h. The sample was removed, rinsed, and the electronic and Raman spectrum were again recorded and are shown as green traces in Figs. 12. The conductivity of the sample increased while still remaining nonlinear with respect to applied voltage (see Fig. 2). Figure 1c shows the Raman spectrum created by subtracting the “oligonucleotide” spectrum from the DDT spectrum. The resultant spectrum shows characteristic nucleic acid peaks for cytosine (at 619 and 1023cm1),23 adenine (at 1332cm1),24 thymine (at 992cm1),23 and guanine (at 1315 and 1602cm1).24 This information verifies that some oligonucleotide was added to the solid state nanogap. It is expected that this corresponds to a significant Raman enhancement factor. Unfortunately, to date Raman spectra for single stranded oligonucleotide is notoriously difficult to obtain25 and by our hands none have been collected on other substrates for comparison. Notice also that while all conditions share similar peaks in the range of the sp2 bands, besides the additional peaks below 1200 relative wavenumbers, the oligo sample exhibits a significant shift in the 1342cm1 peak to lower wavenumbers and a shift in the 1585cm1 peak to higher wavenumbers. This can be observed easily in Fig. 1c. It is hypothesized that these features are due to the convolution of peaks from the remaining degraded oligonucleotide from the fabrication process and some overlapping peaks from the added oligonucleotide. It is expected that the shifts predominantly indicate the presence of C–N stretching and NH2 deformations, respectively.18

In conclusion, the probing of electronic and optical properties for nanogaps created using a combination of oligo-based molecular lithography and conventional photolithography has been shown. Because of the advanced state of common oligonucleotide preparation techniques, theoretically the oligonucleotide length and thus a single layer molecular resist thickness can be easily tailored to size specifications from just a few nanometers up to realistically tens of nanometers. These nanogaps are not only capable of sensitive electronic detection for quickly and inexpensively probing charge transfer at the nanogap, but may also be analyzed for molecular information using SERS.

Acknowledgments

G.S.M. and B.M. would like to thank the NIH (DA023586) and North Carolina State University, College of Engineering and Department of Biomedical Engineering for funding.

References

  1. Mulvaney S. P., He L., Natan M. J., and Keating C. D., J. Raman Spectrosc. 10.1002/jrs.972 34, 163 (2003). [DOI] [Google Scholar]
  2. Gunnarsson L., Bjerneld J., Xu H., Petronis S., Kasemo B., and Kall M., Appl. Phys. Lett. 10.1063/1.1344225 78, 802 (2001). [DOI] [Google Scholar]
  3. Etchegoin P., Cohen L. F., Hartigan H., Brown R. J. C., Milton M. J. T., and Gallop J. C., J. Chem. Phys. 10.1063/1.1597480 119, 5281 (2003). [DOI] [Google Scholar]
  4. Ward D. R., Grady N. K., Levin C. S., Halas N. J., Wu Y. P., Nordlander P., and Natelson D., Nano Lett. 10.1021/nl070625w 7, 1396 (2007). [DOI] [PubMed] [Google Scholar]
  5. Ward D. R., Halas N. J., Ciszek J. W., Tour J. M., Wu Y., Nordlander P., and Natelson D., Nano Lett. 8, 919 (2008). [DOI] [PubMed] [Google Scholar]
  6. Zheng G., Qin L., and Mirkin C. A., Angew. Chem., Int. Ed. 10.1002/anie.200705312 47, 1938 (2008). [DOI] [PubMed] [Google Scholar]
  7. Muller C. J., van Ruitenbeek J. M., and de Jongh L. J., Phys. Rev. Lett. 10.1103/PhysRevLett.69.140 69, 140 (1992). [DOI] [PubMed] [Google Scholar]
  8. Reed M. A., Zhou C., Muller C. J., Burgin T. P., and Tour J. M., Science 10.1126/science.278.5336.252 278, 252 (1997). [DOI] [Google Scholar]
  9. Qin L., Park S., Huang L., and Mirkin C. A., Science 10.1126/science.1112666 309, 113 (2005). [DOI] [PubMed] [Google Scholar]
  10. Wei D., Liu Y., Cao L., Wang Y., Zhang H., and Yu G., Nano Lett. 8, 1625 (2008). [DOI] [PubMed] [Google Scholar]
  11. Liu B., Xiang J., Zhong C., Tian J. H., Mao B. W., Yang F. Z., Chen Z. B., Wu S. T., and Tian Z. Q., Electrochim. Acta 50, 3041 (2005). [Google Scholar]
  12. McCarty G. S., Nano Lett. 10.1021/nl049375z 4, 1391 (2004). [DOI] [Google Scholar]
  13. Hatzor A. and Weiss P. S., Science 291, 1019 (2001). [DOI] [PubMed] [Google Scholar]
  14. Tinland B., Pluen A., Sturm J., and Weill G., Macromolecules 10.1021/ma970381+ 30, 5763 (1997). [DOI] [Google Scholar]
  15. Ferrari A. C. and Robertson J., Phys. Rev. B 10.1103/PhysRevB.61.14095 61, 14095 (2000). [DOI] [Google Scholar]
  16. Knight D. S. and White W. B., J. Mater. Res. 10.1557/JMR.1989.0385 4, 385 (1989). [DOI] [Google Scholar]
  17. Barhoumi A., Zhang D., Tam F., and Halas N. J., J. Am. Chem. Soc. 130, 5523 (2008). [DOI] [PubMed] [Google Scholar]
  18. Jang N. H., Bull. Korean Chem. Soc. 23, 1790 (2002). [Google Scholar]
  19. Endres R. G., Cox D. L., and Singh R. R. P., Rev. Mod. Phys. 10.1103/RevModPhys.76.195 76, 195 (2004). [DOI] [Google Scholar]
  20. van Zalinge H. Schiffrin D. J., Bates A. D., Haiss W., Ulstrup J. and Nichols R. J., ChemPhysChem 10.1002/cphc.200500413 7, 94 (2006). [DOI] [PubMed] [Google Scholar]
  21. Carey P. R., J. Biol. Chem. 10.1074/jbc.274.38.26625 274, 26625 (1999). [DOI] [PubMed] [Google Scholar]
  22. Carey P. R., J. Raman Spectrosc. 10.1002/(SICI)1097-4555(199810/11)29:10/11<861::AID-JRS323>3.3.CO;2-2 29, 861 (1998). [DOI] [Google Scholar]
  23. Otto C., van den Tweel T. J. J., de Mul F. F. M., and Greve J., J. Raman Spectrosc. 10.1002/jrs.1250170311 17, 289 (1986). [DOI] [Google Scholar]
  24. Anthony T., in Raman Spectroscopy in Biology: Principles and Applications (Wiley, New York, 1982), p. 134. [Google Scholar]
  25. Gearheart L. A., Ploehn H. J., and Murphy C. J., J. Phys. Chem. B 10.1021/jp0106606 105, 12609 (2001). [DOI] [Google Scholar]

Articles from Applied Physics Letters are provided here courtesy of American Institute of Physics

RESOURCES