• We are sorry, but NCBI web applications do not support your browser and may not function properly. More information
Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Science. Author manuscript; available in PMC Dec 12, 2008.
Published in final edited form as:
PMCID: PMC2601629
NIHMSID: NIHMS77286

Mussel-Inspired Surface Chemistry for Multifunctional Coatings

Abstract

We report a method to form multifunctional polymer coatings through simple dip-coating of objects in an aqueous solution of dopamine. Inspired by the composition of adhesive proteins in mussels, we used dopamine self-polymerization to form thin, surface-adherent polydopamine films onto a wide range of inorganic and organic materials, including noble metals, oxides, polymers, semiconductors, and ceramics. Secondary reactions can be used to create a variety of ad-layers, including self-assembled monolayers through deposition of long-chain molecular building blocks, metal films by electroless metallization, and bioinert and bioactive surfaces via grafting of macromolecules.

Methods for chemical modification of bulk material surfaces play central roles in modern chemical, biological, and materials sciences, and in applied science, engineering, and technology (14). The existing toolbox for the functional modification of material surfaces includes methods such as self-assembled monolayer (SAM) formation, functionalized silanes, Langmuir-Blodgett deposition, layer-by-layer assembly, and genetically engineered surface-binding peptides (59). Although widely implemented in research, many available methods have limitations for widespread practical use; specific examples include the requirement for chemical specificity between interfacial modifiers and surfaces (e.g., alkanethiols on noble metals and silanes on oxides), the use of complex instrumentation and limitations of substrate size and shape (Langmuir-Blodgett deposition), or the need for multistep procedures for implementation (layer-by-layer assembly and genetically engineered surface-binding peptides).

Development of simple and versatile strategies for surface modification of multiple classes of materials has proven challenging, and few generalized methods for accomplishing this have been previously reported (10). Our approach is inspired by the adhesive proteins secreted by mussels for attachment to wet surfaces (11). Mussels are promiscuous fouling organisms and have been shown to attach to virtually all types of inorganic and organic surfaces (12), including classically adhesion-resistant materials such as poly(tetrafluoroethylene) (PTFE) (Fig. 1A). Clues to mussels’ adhesive versatility may lie in the amino acid composition of proteins found near the plaque-substrate interface (Fig. 1, B to D), which are rich in 3,4-dihydroxy-l-phenylalanine (DOPA) and lysine amino acids (13). In addition to participating in reactions leading to bulk solidification of the adhesive (1416), DOPA forms strong covalent and noncovalent interactions with substrates (17).

Fig. 1
(A) Photograph of a mussel attached to commercial PTFE. (B and C) Schematic illustrations of the interfacial location of Mefp-5 and a simplified molecular representation of characteristic amine and catechol groups. (D) The amino acid sequence of Mefp-5 ...

DOPA and other catechol compounds perform well as binding agents for coating inorganic surfaces (1823), including the electropolymerization of dopamine onto conducting electrodes (24); however, coating of organic surfaces has proven much more elusive. Hypothesizing that the coexistence of catechol (DOPA) and amine (lysine) groups may be crucial for achieving adhesion to a wide spectrum of materials, we identified dopamine as a small-molecule compound that contains both functionalities (Fig. 1E). We show that this simple structural mimic of Mytilus edulis foot protein 5 (Mefp-5) is a powerful building block for spontaneous deposition of thin polymer films on virtually any bulk material surface and that the deposited films are easily adapted for a wide variety of functional uses.

Simple immersion of substrates in a dilute aqueous solution of dopamine, buffered to a pH typical ofmarine environments (2mg of dopamine per milliliter of 10 mM tris, pH 8.5), resulted in spontaneous deposition of a thin adherent polymer film (Fig. 1, F to H). Analysis by atomic force microscopy (AFM) indicated that the polymer film thickness was a function of the immersion time and reached a value of up to 50 nm after 24 hours (Fig. 1G). X-ray photoelectron spectroscopy (XPS) analysis of 25 diverse materials coated for 3 hours or more revealed the absence of signals specific to the substrate (solid red bars in Fig. 1H; see also fig. S1), indicating the formation of a polymer coating of 10 nm or more in thickness. Little variation in the atomic composition of the coating was found (blue circles in Fig. 1H), suggesting that the composition of the polymer coating was independent of the substrate composition. The nitrogen-to-carbon signal ratio (N/C) of 0.1 to 0.13 is similar to that of the theoretical value for dopamine (N/C = 0.125), implying that the coating is derived from dopamine polymerization. Evidence for dopamine polymerization was found through analysis of the modification solution by gel permeation chromatography (fig. S2) and of coated substrates by time-of-flight secondary ion mass spectrometry (TOF-SIMS) (fig. S3). Polymer was found both in solution and on the substrate, with TOF-SIMS clearly revealing signals corresponding to dihydroxyphenyl-containing polymer fragments. Although the exact polymerization mechanism is unknown at this time, it is likely to involve oxidation of the catechol to a quinone, followed by polymerization in a manner reminiscent of melanin formation, which occurs through polymerization of structurally similar compounds (25) (fig. S3).

The polydopamine coating is able to form on virtually all types of material surfaces (Fig. 1H): noble metals (Au, Ag, Pt, and Pd), metals with native oxide surfaces (Cu, stainless steel, and NiTi shape-memory alloy), oxides [TiO2, non-crystalline SiO2, crystalline SiO2 (quartz) Al2O3, and Nb2O5], semiconductors (GaAs and Si3N4), ceramics [glass and hydroxyapatite (HAp)], and synthetic polymers {polystyrene (PS), polyethylene (PE), polycarbonate (PC), polyethylene terephthalate (PET), PTFE, polydimethylsiloxane (PDMS), polyetheretherketone (PEEK), and polyurethanes [Carbothane (PU1) and Tecoflex (PU2)]}.

The polydopamine coating was found to be an extremely versatile platform for secondary reactions, leading to tailoring of the coatings for diverse functional uses. For example, the metal-binding ability of catechols (26) present in the polydopamine coating was exploited to deposit adherent and uniform metal coatings onto substrates by electroless metallization. This was demonstrated through deposition of silver and copper metal films via dip-coating of polydopamine-coated objects into silver nitrate and copper(II) chloride solutions, respectively (Fig. 2). Metal film deposition was confirmed by XPS and TOF-SIMS analysis, which demonstrated successful metal film deposition on several ceramic, polymer, and metal substrates: nitrocellulose, coinage metals, commercial plastics, Si3N4, glass, Au, TiO2, SiO2 PC, PS, PEEK, Nb2O5, Al2O3, and NiTi (figs. S4 and S5). Metal coatings were successfully applied in this manner to flexible polymer substrates and bulk objects with complex shapes (Fig. 2, A to C), as well as to flat surfaces in which the polydopamine coating had been patterned by means of standard photolithography techniques (Fig. 2, D to F). Unlike many other approaches to electroless metallization (27), the use of (immobilized) colloidal metal seed particles was unnecessary for spontaneous formation of adherent metal films. In the case of silver film deposition, the apparent reductive capacity of the polydopamine sublayer was sufficient to eliminate the need for addition of an exogenous reducing agent in the metal salt solution, implying oxidation of the underlying polydopamine layer.

Fig. 2
Polydopamine-assisted electroless metallization of substrates. (A to C) Electroless copper deposition on polydopamine-coated nitrocellulose film (A), coin (B), and three-dimensional plastic object (C). (D) Schematic representation of electroless metallization ...

Polydopamine coatings also support a variety of reactions with organic species for the creation of functional organic ad-layers. For example, under oxidizing conditions, catechols react with thiols and amines via Michael addition or Schiff base reactions (14, 28) (fig. S3B). Thus, immersion of polydopamine-coated surfaces into a thiol- or amine-containing solution provided a convenient route to organic ad-layer deposition through thiol- and amine-catechol adduct formation (Fig. 3A). We demonstrated this approach for deposition of organic ad-layers in the form of alkanethiol monolayer, synthetic polymer, and biopolymer coatings.

Fig. 3
Polydopamine-assisted grafting of various organic molecules. (A) Schematic illustration of alkanethiol monolayer (top right) and PEG polymer (bottom right) grafting on polydopamine-coated surfaces. (B) Pictures of water droplets on several unmodified ...

A monolayer of alkanethiol was spontaneously formed through simple immersion of polydopamine-coated substrates (Fig. 3B). Monolayer formation on the polydopamine sublayer is believed to involve reaction between terminal thiol groups and the catechol/quinone groups of the polydopamine coating, in a manner analogous to the reaction between thiols and noble metal films in the formation of conventional SAMs. Alkanethiol monolayers formed by this approach are likely to contain defects but nevertheless appear to be functionally similar to conventionally formed SAMs. We therefore refer to these monolayers of alkanethiols as “pseudo-SAMs” (pSAMs). For example, spontaneous formation of pSAMs with the use of methylterminated alkanethiol (C12-SH) was suggested by water contact angles of greater than 100° (Fig. 3B and table S1) (29) and XPS spectra revealing the presence of sulfur in the modified surfaces (fig. S6). pSAMs were formed in this way on at least seven different materials, including several ceramics and polymers.

Through proper choice of secondary reactants, polydopamine coatings can be transformed into surfaces that have specific chemical properties, such as the suppression of nonspecific biological interactions or the promotion of specific ones (23, 24). We first demonstrated this by formation of pSAMs from heterobifunctional molecular precursors on polydopamine-coated surfaces as described above. pSAMs terminated by oligo(ethylene glycol) (OEG6) were found to be largely resistant toward fibroblast cell attachment (Fig. 3C), behaving in a qualitatively similar fashion to nonfouling SAMs formed on gold (30).

Grafting of polymer ad-layers onto polydopamine coatings was accomplished through the use of thiol- or amine-functionalized polymers in the secondary reaction step, giving rise to bioresistant and/or biointeractive surfaces. For example, fouling-resistant surfaces were made by covalently grafting amine- or thiol-terminated methoxy-poly(ethylene glycol) [(mPEG-NH2 or mPEG-SH) in 10 mM tris, pH 8.5, 50°C] to the polydopamine-coated surface (fig. S7). mPEG-NH2–modified polydopamine-coated glass exhibited substantial reduction in nonspecific protein adsorption as compared with uncoated glass and also outperformed glass surfaces modified by a silane-terminated PEG in terms of fouling resistance after 2 days of continuous exposure to protein solution (Fig. 3, D to F). Similarly, mPEG-SH grafting onto a variety of polydopamine-coated substrates led to dramatic reduction of fibroblast cell attachment as compared with the unmodified substrates (Fig. 3G and table S3). The polydopamine coating itself was supportive of fibroblast cell adhesion at a level similar to that of bare substrates {for example, the total area of attached cells on 1.08 mm2 of polydopamine-modified SiO2 [(46 ± 1.4) × 103 µm2] was similar to that of unmodified SiO2 [(55 ± 8.6) × 103 µm2]}, leading us to conclude that the observed decrease in cell adhesion was due to the grafted mPEG-SH.

Finally, we engineered polydopamine surfaces for specific biomolecular interactions by forming an ad-layer of the glycosaminoglycan hyaluronic acid (HA). HA/receptor interactions are important for physiological and pathophysiological processes, including angiogenesis, hematopoietic stem cell commitment and homing, and tumor metastasis (31, 32). Partially thiolated HA (33) was grafted onto a variety of polydopamine-coated substrates (Fig. 4), and HA ad-layer bioactivity was measured via adhesion of the human megakaryocytic M07e cell line. Unlike fibroblasts, M07e cells did not adhere to polydopamine but did adhere to HA-grafted polydopamine surfaces in a dose-dependent manner (Fig. 4B). Together with decreased binding in the presence of soluble HA (Fig. 4C), these findings are consistent with expression of the HA receptor CD44 by M07e cells (fig. S8). Polydopamine and HA-grafted polydopamine surfaces were biocompatible, as evidenced by similar levels of M07e cell expansion as compared with cell expansion on tissue-culture PS surfaces, although only the HA-grafted polydopamine surfaces supported cell adhesion (Fig. 4, D to F, and fig. S9).

Fig. 4
Polydopamine-assisted grafting of a biomacromolecule for biospecific cell interaction. (A) Representative scheme for HA conjugation to polydopamine-coated surfaces. (B) Adhesion of M07e cells on polydopamine-coated PS increases with the HA solution concentration ...

We introduced a facile approach to surface modification in which self-polymerization of dopamine produced an adherent polydopamine coating on a wide variety of materials. Polydopamine coatings can, in turn, serve as a versatile platform for secondary surface-mediated reactions, leading ultimately to metal, SAM, and grafted polymer coatings. This two-step method of surface modification is distinctive in its ease of application, use of simple ingredients and mild reaction conditions, applicability to many types of materials of complex shape, and capacity for multiple end-uses.

Supplementary Material

Supplementary

Supporting Online Material:

www.sciencemag.org/cgi/content/full/318/5849/426/DC1

Materials and Methods

Figs. S1 to S10

Tables S1 to S3

References

References and Notes

1. Ratner BD, Hoffman AS, editors. Biomaterials Science: An Introduction to Materials in Medicine. ed. 2. San Diego, CA: Elsevier Academic; 2004.
2. Ahn J-H, et al. Science. 2006;314:1754. [PubMed]
3. Alivisatos P. Nat. Biotechnol. 2004;22:47. [PubMed]
4. Langer R. Science. 2001;293:58. [PubMed]
5. Love JC, Estroff LA, Kriebel JK, Nuzzo RG, Whitesides GM. Chem. Rev. 2005;105:1103. [PubMed]
6. Decher G. Science. 1997;277:1232.
7. Roberts G, editor. Langmuir-Blodgett Films. New York: Plenum; 1990.
8. Whaley SR, English DS, Hu EL, Barbara PF, Belcher AM. Nature. 2000;405:665. [PubMed]
9. Tamerler C, Sarikaya M. Acta Biomater. 2007;3:289. [PubMed]
10. Ryu DY, Shin K, Drockenmuller E, Hawker CJ, Russell TP. Science. 2005;308:236. [PubMed]
11. Waite JH, Tanzer ML. Science. 1981;212:1038. [PubMed]
12. Young GA, Crisp DJ. In: Adhesion. Allen KW, editor. vol. 6. London: Applied Science; 1982.
13. Waite JH, Qin XX. Biochemistry. 2001;40:2887. [PubMed]
14. Burzio LA, Waite JH. Biochemistry. 2000;39:11147. [PubMed]
15. Sever MJ, Weisser JT, Monahan J, Srinivasan S, Wilker JJ. Angew. Chem. Int. Ed. 2004;43:448. [PubMed]
16. Yu M, Hwang J, Deming TJ. J. Am. Chem. Soc. 1999;121:5825.
17. Lee H, Scherer NF, Messersmith PB. Proc. Natl. Acad. Sci. U.S.A. 2006;103:12999. [PMC free article] [PubMed]
18. Yu M, Deming TJ. Macromolecules. 1998;31:4739. [PubMed]
19. Dalsin JL, Hu B-H, Lee BP, Messersmith PB. J. Am. Chem. Soc. 2003;125:4253. [PubMed]
20. Statz AR, Meagher RJ, Barron AE, Messersmith PB. J. Am. Chem. Soc. 2005;127:7972. [PubMed]
21. Paunesku T, et al. Nat. Mater. 2003;2:343. [PubMed]
22. Xu C, et al. J. Am. Chem. Soc. 2004;126:9938. [PubMed]
23. Zürcher S, et al. J. Am. Chem. Soc. 2006;128:1064. [PubMed]
24. Li Y, Liu M, Xiang C, Xie Q, Yao S. Thin Solid Films. 2006;497:270.
25. Montagna W, Prota G, Kenney JA., Jr . Black Skin: Structure and Function. San Diego, CA: Academic Press; 1993.
26. Pierpont CG, Lange CW. Prog. Inorg. Chem. 1994;41:331.
27. Charbonnier M, Romand M, Stremsdoerfer G, Fares-Karam A. Recent Res. Dev. Macromol. Res. 1999;4:27.
28. LaVoie MJ, Ostaszewski BL, Weihofen A, Scholssmacher MG, Selkoe DJ. Nat. Med. 2005;11:1214. [PubMed]
29. Laibinis PE, et al. J. Am. Chem. Soc. 1991;113:7152.
30. Prime KL, Whitesides GM. J. Am. Chem. Soc. 1993;115:10714.
31. Haylock DN, Nilsson SK. Regenerat. Med. 2006;1:437. [PubMed]
32. Toole BP. Nat. Rev. Cancer. 2004;4:528. [PubMed]
33. Lee H, Choi SH, Park TG. Macromolecules. 2006;39:23.
34. Single-letter abbreviations for the amino acid residues are as follows: A, Ala; C, Cys; D, Asp; E, Glu; F, Phe; G, Gly; H, His; I, Ile; K, Lys; L, Leu; M, Met; N, Asn; P, Pro; Q, Gln; R, Arg; S, Ser; T, Thr; V, Val; W, Trp; and Y, Tyr.
35. This research was supported by NIH grants DE 14193 and HL 74151. The authors thank T. G. Park and H. Lee for donation of thiolated HA, N. F. Scherer and X. Qu for their generous discussion and technical assistance with TIRF microscopy, and K. Healy for photomask donation. This research used the NUANCE characterization facilities (Keck II, EPIC, and NIFTI) at Northwestern University.
PubReader format: click here to try

Formats:

Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...

Links