Patent Application
20050112277
Microarrays have become widely applied in proteomic and genomic analysis, as they permit multiplexed analysis of multiple analytes. See, e.g., Ramsay, Nat. Biotechnol. 16, 40-44 (1998); P. Brown, D. Botstein, Nat. Genet. 21, 33-37 (1999); D. Duggan, M. Bittner, Y. Chen, P. Meltzer, J. M. Trent, Nat. Genet. 21, 10-14 (1999); R. Lipshutz, S. P. A. Fodor, T. R. Gingeras, D. J. Lockhart, Nat. Genet. 21, 20-24 (1999). In a microarray, binding agents such as antibodies and/or oligonucleotides are spotted on planar substrates. These binding agents are then contacted with samples including complementary ligands (proteins or complementary oligonucleotides, as applicable) and permitted to bind or hybridize. The binding or hybridization is then detected. Because either the identity of the binding agents or the complementary ligands are known, by tracing their identity in the array, the complementary oligonucleotides or proteins can be determined. This is an effective method for identification or quantification of analytes in a sample.
The principal techniques of oligonucleotide array fabrication include: spotted arrays, and refinements of the original “spotting” in the form of pin transfer or ink jet printing of small aliquots of probe solution onto various substrates, as illustrated in V. G. Cheung, et al., Nat. Genet. 21, 15-19 (1999); sequential electrophoretic deposition of binding agents in individually electrically addressable substrate regions, as illustrated in J. Cheng, et al., Nat. Biotechnol. , 541-546 (1998); and methods facilitating spatially resolved in-situ synthesis of oligonucleotides, as illustrated in U. Maskos, E. M. Southern, Nucleic Acids Res. 20, 1679-1684 (1992); S. P. A. Fodor, et al., Science 251, 767-773 (1991) or copolymerization of oligonucleotides, as illustrated in A. V. Vasiliskov, et al., BioTechniques 27, 592-606 (1999). These techniques produce spatially encoded arrays in which the position within the array indicates the chemical identity of any constituent probe.
The reproducible fabrication of customized arrays by these techniques requires the control of microfluidics and/or photochemical manipulations of considerable complexity to ensure consistent performance in quantitative assays. Microfluidic spotting to produce, in quantitatively reproducible fashion, deposited features of 100 μm diameter involves dispensing of nanoliter aliquots with tight volume control, a task that exceeds the capabilities of currently available fluid handling methodologies. In addition, exposure of binding agents to air during the deposition process, typically several hours' in duration, has uncontrollable impact on the molecular configuration and the accessibility of the binding agents in subsequent binding assays. In-situ array synthesis relies on a sequence of multiple masking and photochemical reaction steps which must be redesigned to accommodate any changes in array composition. Finally, assay performance must be assessed “in-situ” for each array subsequent to immobilization of binding agents, an aspect of array manufacturing which raises difficult quality control and implementation issues.
As an alternative to solve many of the problems associated with spotted arrays, microbead particles bound to oligonucleotide probes have been used. See U.S. application Ser. No. 10/271,602, “Multiplexed Analysis of Polymorphic Loci by Concurrent Interrogation and Enzyme-Mediated Detection” filed Oct. 15, 2002; Ser. No. 10/204,799 “Multianalyte Molecular Analysis Using Application-Specific Random Particle Arrays,” filed on Aug. 23, 2002, both being incorporated by reference. The beads are deposited on a substrate, and preferably affixed thereto, to form an array. Among the principal advantages are that the beads are encoded so that particular probes associated with particular beads can be determined by decoding. This obviates the need, associated with spotted arrays, to form arrays with particular probes in particular positions (spatial encoding).
Affixing the beads to the substrate is desirable because if they move about on the substrate, decoding signals cannot be localized and accurately interpreted. One of the advantages of a bead array is that the signal from the array and the decoding can be accomplished using an ordinary microscope. For example, a microscope can acquire a fluorescent signal from bound ligands in the array or can detect color differences which encode the beads. The array should be sized such that the entire array can be viewed in a single field, i.e., all at once, under the microscope.
One method of immobilizing beads involves confining them to wells in the substrate, where the wells are size-matched in diameter to the beads (i.e., only slightly larger than the beads). The height of the wells is preferably also about the same as that of the beads.
By way of background, it is noted that the magnitude of the adhesion force between two solid surfaces depends on a number of factors, including surface chemistry, relative humidity, temperature, surface roughness, time of contact, nature of the material, and others. However, for two surfaces to establish adhesive contact, they must first approach each other closely. A number of colloidal forces control and modulate the approach of two surfaces.
Capillary forces also can be very effective in bringing two surfaces close to each other. For example, the capillary force (Fc) between a rigid sphere of radius R and a flat surface has the functional form Fc˜4πRσ cos θ, where θ is the local contact angle, and σ the interfacial tension of the liquid forming the capillary film. See Israelachvili, J. N. Intermolecular and Surface Forces, Academic Press, New York, 1985. For a wetting film, the large interfacial tension of the liquid leads to a correspondingly large value of Fc.
Once in contact, whether two surfaces will adhere is not solely determined by the net attraction between molecules. Bodies deform macroscopically in response to being placed in contact and hence the bulk contact geometry as well as material properties, such as elastic modulus and hardness, all affect the conformity and adhesion of one surface to another. According to JKR theory (Johnson, K. L, Kendall, K., Roberts, A. D. Surface Energy and the Contact of Elastic Solids. Proc. R. Soc. London A 1971, 324, 301) the variation of the radius of contact ‘a’ under applied load ‘P’ has the form
where K denotes an elastic constant, W ˜{square root}{square root over (γ1γ2)}, denotes the work of adhesion (where γ1 and γ2 are the surface energies of the two surfaces in contact) and R denotes the radius of curvature. In the absence of any applied load (P), the equilibrium contact radius is:
The theory also predicts an adhesive contact force (Fadh):
A large area of contact enhances adhesion, however it alone is not sufficient. For example, a wetting liquid achieves an excellent contact, but does not generate significant adhering force, because it does not resist shear deformation.
In reality, material surfaces are rough and hence are never in intimate contact. If the real area of contact is small, adhesion is weak. For rough surfaces, surface phenomena alone cannot account for the adhesion and many other macroscopic phenomena come into play, including, the degree of surface roughness, the maximal normal force applied to the contact, time for which the surfaces are in contact, bulk molecular structure and dynamics, and others. One of the early studies by Greenwood and Tripp (Greenwood, J. A., Tripp, J. H. The Elastic Contact of Rough Spheres. J. Appl. Mech. 1967 (March) 153-159) concluded that the effective initial contact area between rough surfaces is given by:
a={square root}{square root over (2Rσroughness)}
where σroughness is the root mean square of the surface asperities and R the bulk radius of curvature of the system (radius of the sphere for a sphere and flat system). A recent study by Quon et al. (Quon, R. A., Knarr, R. F., and Vanderlick, T. K. Measurement of the Deformation and Adhesion of Rough Solids in Contact. J. Phys. Chem. B 1999, 103, 5320-5327) concluded that systems that are in initial contact over an area with a radius greater than that predicted above are strongly adherent and ones with a smaller radius of contact are either weakly adherent or non-adherent. Thus, for rough solids, the adhesion improves with increasing initial loads. Under the influence of an increased initial load, asperities deform, permitting the surfaces to approach more closely and thereby permitting van der Waals attractions to contribute to adhesion.
In immobilizing bead arrays on silicon substrates (chips) for multiplexed analysis of multiple analytes, the immobilization must take place after completion of the array assembly process. Also, the immobilization protocol should not in any substantial manner affect the on-chip bioassays, i.e., it should, instead, preserve receptor moieties displayed on bead surfaces, leave binding kinetics unaffected and minimize non-specific binding.
Disclosed are two different approaches for immobilization of beads on a substrate, one of which involves forming a bead-nanoparticle composite by cross-linking of the bead mixture with nanoparticles, and the other involving surface modification, using multi-layered polyelectrolytes.
In the first approach, an array of functionalized beads is assembled in a designated location (preferably in a depression or at another type of bead localization site, as described in Ser. No. 10/192,352, “Arrays of Microparticles and Methods of Preparation Thereof,” filed Jul. 9, 2002) on a chip. Next, a droplet of nanoparticle suspension is introduced over the chip. The suspending solution is then allowed to evaporate for a pre-determined length of time, during which time the nanoparticles undergo extensive self-aggregation and adhere to beads as well as to the substrate surface. During incubation, care is taken to avoid complete evaporation of water, which will form a dry sintered film. After the incubation, the excess nanoparticle suspension is aspirated off and the surface of the chip cleaned by thorough scrubbing and washing. This removes the adhering nanoparticles from the exposed portions of the chip and the beads, but leaves behind the nanoparticles which are trapped between the bead and the substrate. The aggregated nanoparticles trapped between the beads and the substrate surface act to immobilize the beads in the wells. See
While this method is effective in immobilizing beads, a possible disadvantage is that there is an increase in nonspecific binding of analytes (e.g., oligonucleotides) to the nanoparticles. The nanoparticles accumulate around the beads in the wells, trapped between the beads and the well-wall, and this non-specific binding leads to a non-specific signal. The non-specific binding can be decreased by pre-treatment of the substrate with a polymer like polyethylene glycol (“PEG”), which coats the substrate and the nanoparticles, and thereby reduces nonspecific binding of the analytes. See Example 2.
Ultrathin surface films are routinely used to modify and/or add functionality to solid phase supports. Traditional chemisorption techniques usually require a reaction yield of 100% or extensive lateral crosslinking to establish and maintain a uniform film. A relatively new technique for growing ultrathin surface films is by successive deposition of alternating layers of cationic and anionic polyelectrolytes (Iler, R. K. J. Colloid Interface Sci. 1966,21,569; Decher, G., Hong, J. D. European patent number 0472 990 A2, 1992; Decher, G. Fuzzy “Nanoassemblies: toward layered polymeric multicomposites.” Science 277, 1232, 1997). In this approach, electrostatic attraction adheres successive layers. Recently, there have been a few reports of use of oppositely charged polymer-nanoparticle systems for growing such multilayered films. See Sennerfors, T et al. Journal of Colloid and Interface Science, 254, 222-226 (2002); Serizawa, T. et al. Langmuir, 1998, 14, 4088-4094; Lvov, Y, et al. Langmuir 1997, 13, 6195-6203; Kotov, N. A. J. Phys. Chem. 1995, 99, 13065-13069.
This type of multilayer assembly is depicted schematically in
Different designs of depressions are also disclosed, some of which are suitable for holding beads in place without any deposition of nanoparticles or polyelectrolytes.
A description of the drawing figures, and examples, along with a more detailed description, follow.
Turning first to
With any of the design of holes described herein, one can use additional techniques, including deposition of polyelectrolyte layers or a nanoparticle suspension, to hold beads in place in the holes. Examples of such techniques are set forth below. Alternatively, for depressions into which beads are wedged or squeezed, additional steps may not be required to hold the beads in place.
An experiment was designed to estimate the critical concentration of nanoparticles needed for particle immobilization in traps. For this experiment, an array of hexagonal traps of size 3.5 micron (side-to-side diameter) and a depth of 3.5 micron were made in a silicon substrate. 3.2 micron diameter latex particles coated with neutravidin protein were stained with a green fluorescent dye. The nanobead stock suspension was 80 nm silica particles at 34% by wt. (Snowtex-ZL, Nissan Chemicals, Houston, Tex.). Aliquots were taken from the nanoparticle stock and diluted with 10 mM Tris buffer (pH 8.0) containing 3%(v/v) glycerol to make desired concentrations. These diluted suspensions were then used to perform the experiments.
The beads were assembled on the substrate using the following protocol.
An example of a processing procedure for forming bead arrays is as follows. Two microliters of 1% microparticles (approximately 3.2 micrometers in diameter) in 100 microliters of phosphate-buffered saline (also known as PBS: 150 mM, NaCl; 100 mM, Sodium phosphate, pH 7.2) were used for assembling microparticle arrays on individual silicon chips (1.75×1.75 mm) with microwells on each chip. The following procedures were used:
Following assembly, the occupancy of the traps was checked by fluorescence microscopy. See
The bead assembly was carried out as described in Example1 using a 1% nanoparticle solution. The polymer blocking solution used for this study was 1% (w/v) PEG 20,000 dissolved in 10 mM Tris with 3% (v/v) glycerol. Following the particle assembly and immobilization using the nanoparticle suspension, 15 μl of the polymer solution was added to each chip, which were stored in a humid chamber at 4° C. overnight. For performing the assay, first the excess polymer solution was removed from the chip surface and the chip was washed with de-ionized water.
A hybridization assay was performed using a 90-nt Cy5 labeled polynucleotide target. Two microliters of a 10 μM solution of a synthetic target (5′-Cy5 dye- coupled to the oligo:TCAGTTTTCCTGGATTATGCCTGGCACCATTAAAGAAAATATCA TCTTTGGTGTTTCCTATGATGAATATAGATACAGAAGCGTCATCAA-3′ (SEQ ID NO. 1)) in de-ionized water was diluted with 18 μl of 1×TMAC (4.5 M tetramethyl ammonium chloride, 75 mM Tris pH 8.0, 3 mM EDTA, 0.15% SDS) to a final volume of 20 μl. Two types of oligonucleotide-functionalized fluorescent microparticles were assembled into planar arrays on silicon chips, using the protocol set forth above. The first microparticle type was functionalized with a matched probe sequence (SEQ ID NO.2) 5′-Amino/(TEGspacer)/CCAAAGATGATATTTTC/-3′ (“TEG” is triethylene glycol). The second microparticle type was functionalized with a mismatched probe sequence (SEQ ID NO. 3): Amino/(TEGspacer)/ATAACCAGGAGGAGTTCG/-3′). Twenty microliters of the synthetic target was added to the substrate surface and the substrate was placed in a 55° C. heater for 20 minutes. The substrate was then removed from the heater and the target solution was aspirated. The substrate was washed three times with 1×TMAC at room temperature. Following this, 10 μl of 1×TMAC was placed on the substrate surface, it was covered with a glass cover-slip and the fluorescence intensity of the array was recorded using fluorescence microscopy.
The control assays were done with chips without any added nanoparticle or polymer. In the unoccupied traps in the control assay, there is some non-specific binding of target in the traps. The results are shown in Table 2 and 3, where CV is the coefficient of variation.
The immobilization protocol along with the polymer blocking step preserved the signal for the matched probes (˜10% drop in the specific assay signal), and decreased the non-specific signal from the chip surface (˜20%), while the signal from binding of the mismatched probes was essentially unaffected.
A negatively charged chip (a silicon substrate coated with a layer of silicon dioxide) was immersed in a cationic polyelectrolyte solution (a 1% w/v solution of polyallylamine hydrochloride, having Mol. Wt. 15,000, made by Aldrich Chemicals, Milwaukee, Wis., in 1M calcium chloride) for 2 minutes. The chip was then taken out and thoroughly washed with de-ionized ultra filtered water and put back in a 3.4% (w/v) solution of negatively charged (ξ potential 56 mV at 1 mM ionic strength and at pH ˜4.0) 22 nm Ludox silica nanoparticles (Aldrich Chemicals, Milwaukee, Wis.) in PBS (0.1M Sodium Phosphate, 0.15M Sodium Chloride, pH 7.2) and incubated for 2 minutes. Following this, the chip was taken out and again thoroughly washed with de-ionized ultra filtered water. This treatment resulted in the formation of a bilayer structure as shown in
An experiment was devised to investigate the minimum number of bilayers needed for immobilization of beads in the traps. Three different trap sizes were chosen for this study (see Table 4). All experiments were performed with 3.2 μm oligo-functionalized beads. The calculated trap size and the difference between the trap size and the bead size (mismatch) is shown in Table 4.
The bilayer coating was carried out as described above in Example 3. Table 5 shows the results for the various trap sizes. For a larger mismatch between the bead and the trap size, more bilayer-coatings are needed for immobilization.
Several chips were coated with the minimum number of bilayers needed for immobilization as described in Example 3. Following the coating, the beads were assembled into the traps, as in Example I, and the surface of the chip was scrubbed clean with a damp cotton applicator. This step removes the bilayer film from the exposed part of the chip but leaves the film on the trap walls, which helps to retain the beads in the traps (see
DNA hybridization assays were carried out as described in Example 2. Two microliter of a 10 μM solution of a synthetic target (5′-Cy5 labeled TCAGTTTTCCTGGATTATGCCTGGCACCATTAAAGAAAATATCATCTTTGGTGTT TCCTATGATGAATATAGATACAGAAGCGTCATCAA-3′ (SEQ ID NO. 4)) in de-inonized water was diluted with 98 μl of 1×TMAC (4.5 M tetramethyl ammonium chloride, 75 mM Tris pH 8.0, 3 mM EDTA, 0.15% SDS) to a final volume of 20 μl. Two types of oligonucleotide-functionalized fluorescent microparticles were assembled into planar arrays on silicon chips using a protocol as described above. The first microparticle type was functionalized with a matched probe sequence 5′-Amino/(TEGspacer)/CCAAAGATGATATTTTC/-3′ (SEQ ID NO. 5). The second microparticle type was functionalized with a mismatched probe sequence Amino/(TEGspacer)/ATAACCAGGAGGAGTTCG/-3′ (SEQ ID NO. 6). Twenty microliters of the synthetic target was added to the substrate surface and the substrate was placed in a 55° C. oven for 20 minutes. The substrate was then removed from the oven the target solution was aspirated. The substrate was washed three times with 1×TMAC at room temperature. Following this, 10 μl of 1×TMAC was placed on the substrate surface, covered with a glass cover-slip and the fluorescence intensity of the array was recorded. The results are shown in
Polyelectrolyte bilayer coated chips were fabricated as described in Example 5, but after the last exposure to Ludox solution, two additional bilayers were added, using Polyallylamine solution and a solution of 1% (w/v) Polyacrylic acid, sodium salt (Mol. Wt. 8,000, Aldrich Chemicals, Milwaukee, Wis.) in 1M calcium chloride. After the final polyacrylic acid deposition the chip was washed thoroughly with de-ionized ultra-filtered water and incubated at 120° C. for 2 hours. Beads were assembled on these coated chips as described before and hybridization assay was carried out as described in Example 5. In some of the assays, in addition to the two types in Example 5, a third type of functionalized bead with a mismatched probe sequence Amino/(TEGspacer)/CCCCCCCCCCCCCC/-3 (SEQ ID NO. 7), was also used.
It should be understood that the terms, expressions, examples and embodiments depicted above are exemplary only and not limiting, and that the scope of the invention is defined only in the claims which follow, and includes all equivalents of the subject matter of the claims.
This Application claims priority to U.S. Provisional Application No. 60/478,011, filed Jun. 12, 2003.
| Number | Date | Country | |
|---|---|---|---|
| 60478011 | Jun 2003 | US |
