J. Zhanga,
S. Dua,
A. Kafia,
B. Foxa,
J. L. Lia,
X. Y. Liub,
R. Rajkhowaa and
X. G. Wang*ac
aAustralian Future Fibres Research and Innovation Centre, Institute for Frontier Materials, Deakin University, VIC 3217, Australia. E-mail: xwang@deakin.edu.au
bBiophysics and Micro/Nanostructures Lab, Department of Physics, Faculty of Science, National University of Singapore, 117542, Singapore
cSchool of Textile Science and Engineering, Wuhan Textile University, Wuhan 430073, China
First published on 28th November 2014
Silkworm cocoons are biological composite structures protecting the silkworms against environmental damage and physical attack by natural predators. In particular, some outdoor reared silk cocoons exhibit outstanding mechanical properties that are relevant to the higher level protection required to enhance the survival chance of silkworms while supporting their metabolic activity. The performance of composite materials strongly depends on the adhesion between the fiber reinforcement and matrix, with the surface properties of the fibers playing a key role in determining the level of adhesion achieved. For this reason it is important to study the surface properties of silk fibroin to further understand the composite properties of the cocoons. In this work, both the mechanical properties of the silk cocoons and silk fibroin were studied. The surface topography was examined using scanning probe microscopy (SPM), which revealed distinct longitudinal ridges and striations along the fiber axis of the four silk fiber types. The fibers were found to exhibit heterogeneity in surface energy as evidenced from inverse gas chromatography (IGC) measurements. The combination of excellent mechanical properties and the more energetically heterogeneous surface nature of the wild A. pernyi silk fibroin fibers correlates well with the excellent mechanical properties of the A. pernyi cocoons.
A cocoon is a multilayer porous composite structure formed by continuous twin silk filaments (bave) bonded by silk gum (sericin). The compact cocoon structure is formed when a silkworm, along with spinning, wraps the twin silk filaments around its body through a gyrating motion of its head and cyclically bending and stretching of its body with different shapes in a programmed manner.11,12 The mechanical performance of composites depends on the properties of individual component as well as on the interfacial compatibility between the constituting materials. The performance of composites strongly depends on the strength of the fiber/matrix interfacial zone, which controls the stress transfer process between the reinforcement and the matrix. However, it is difficult to evaluate the interface when the boundary between fiber and matrix is not clear. Composite interfaces can be characterized by analysing the surfaces of the fibers before they are impregnated with matrix.13 In the case of natural silk filaments, the interfacial properties can be examined through analysing the surface of the degummed fibers. Because the fiber/matrix interfacial region is closely related to the surface properties (e.g., surface energy, acid–base interactions, etc.) of both the fibers and matrix, characterization of the surface properties would be necessary to understand the adhesion, including the topography study and the IGC tests of degummed silk fibers for this work. Despite of the importance of surface energy parameters in preparation and properties in silk/polymer composites, the surface characteristics of silkworm silks are scarcely reported in literature.
Our previous work on interlaminar peel tests has shown that the wild silkworm cocoons are uniquely tough composite structures; the maximum work-of-fracture of the wild cocoons (A. pernyi and Antheraea mylitta, i.e. A. mylitta) was approximately 1000 J m−2, which was almost 10 times the value for the domesticated cocoon (B. mori) and 3–4 times the value for the semi-domesticated cocoon (A. assamensis).14,15 For some applications, natural fibers offer advantages over conventional synthetic fibers such as carbon and glass fibers as the reinforcement for composites, i.e. low cost, renewability, acceptable specific strength properties and biodegradability.16,17 As one of the animal-based fibers, silk has received far less attention than plant-based fibers such as flax, jute, kenaf for the use as reinforcement in biocomposites.18,19 As a result, further study of various silkworm silks and more particularly wild silkworm silks and their naturally built composite structures, i.e. cocoons, have important practical implications for the development of new biodegradable and renewable composite materials.
This work employs a range of techniques to characterize both the physical and chemical properties, including surface energy and surface energy heterogeneity, of both domestic and wild silkworm silk fibroin. In particular, inverse gas chromatography (IGC) was used in the present study to characterize the surface properties (surface area, surface energy, heterogeneity and acid–base properties) of several silk fibres.
In IGC, the adsorbent under investigation is placed into a column while a known adsorptive is used in the gas phase. As in analytical gas chromatography, the retention time is obtained as the fundamental parameter measured. The retention time can be converted into a retention volume, which is directly related to several physico-chemical properties of the solid (absorbent). Surface energetic heterogeneity profile can be represented by an energy distribution with surface coverage, which can provide more comprehensive understanding on the nature and population of different surface sites. IGC experiments with finite concentrations were conducted in pulse mode, by injecting a desired amount of probe molecule into the column via inert helium carrier gas. A series of n-alkanes (n-heptane, n-octane and n-nonane) and polar probes (chloroform, ethyl acetate, acetone, acetonitrile and 1,4-dioxane) were injected at a specific fractional surface coverage and their retention times measured for a broad range of fractional surface coverage. The retention times were then converted into retention volumes and the dispersive surface energy (γDs) on a solid sample was determined in accordance with standard methodology as described by Jones.20
Determination of the dispersive surface energy (γDs) and specific free energy of desorption (ΔG0SP), as well as the acidic and basic properties of a solid sample are well documented.21 The net retention volume (VN), a fundamental surface thermodynamic property of the solid–vapor interaction, can be computed from eqn (1):
![]() | (1) |
Total surface energy (γTs) was defined as the sum of the dispersive energy and the specific (γABs) energy contributions and the surface polarity was calculated as γABs/γTs. On the other hand, the specific (acid–base) surface energy (γABs) can be obtained by first measuring the ΔG0SP for different polar probe molecules (i.e. acetonitrile, acetone, ethanol, ethyl acetate and dichloromethane) on the materials. Employing the polarisation approach, the ΔG0SP values are determined from a plot of RTln(VN) versus the molecular polarisabilities of the probes (PD). The values obtained for a series of non-polar n-alkanes follow a linear relationship and ΔG0SP for each polar probe is determined relative to this reference line.23 The acid and base numbers, Ka and Kb, and hence the acid/base ratios (Ka/Kb) were determined according to the method of Gutmann.24
Cocoon wall type | Thickness (μm) | Nominal density (kg m−3) | Young's modulus (MPa) | Maximum load (N) | Breaking stress (MPa) | Breaking strain (%) | Absorbed energy (J) |
---|---|---|---|---|---|---|---|
B. mori | 393 ± 21 | 377 ± 15 | 365 ± 102 | 49 ± 8 | 30 ± 7 | 16 ± 1 | 0.09 ± 0.02 |
S. cynthia | 243 ± 31 | 449 ± 56 | 238 ± 39 | 42 ± 9 | 20 ± 2 | 21 ± 5 | 0.17 ± 0.06 |
A. assamensis | 277 ± 29 | 516 ± 28 | 342 ± 72 | 19 ± 1 | 23 ± 6 | 19 ± 7 | 0.05 ± 0.009 |
A. pernyi | 387 ± 31 | 711 ± 44 | 872 ± 142 | 140 ± 13 | 56 ± 5 | 41 ± 6 | 0.6 ± 0.1 |
As a multilayer composite structure, the cocoon wall was tested not only along the in-plane direction but also along the interlaminar direction. Therefore, in addition to the tensile properties, the interlaminar peel resistance was also examined. The 180 degree peel tests showed that the maximum peeling load was 0.74 N and the average peeling load was 0.35 N for the B. mori cocoon. By comparison, the A. pernyi cocoon had a maximum peeling load of 4.45 N and an average peeling load of 2.51 N. The maximum work of fracture (WOF) of all tested cocoon layers was 981 J m−2 from the A. pernyi outer layer, suggesting the highest interlaminar adhesion and bonding energy between the cocoon layers (Table 2). The toughness for the wild A. pernyi cocoon was approximately 10 times of the B. mori cocoon and twice the values of the S. cynthia and A. assamensis cocoon walls. The results are comparable to Chen et al.'s findings for the B. mori cocoon, where they observed similar nonlinear load–displacement relation with an average peeling load of 0.32 N and a WOF of 61 J m−2 and also proved that the delamination of cocoon walls is mainly caused by the brittle fracture of the inter-layer sericin bonds.25 As a result, the significantly higher bonding energy for the A. pernyi cocoon wall suggests the strongest fibroin/sericin bond in this cocoon type. The high toughness of the wild A. pernyi cocoon is presumably related to the higher level of protection against attack from predators and the hazardous outdoor physical environment.14
Cocoon type | Wall thickness (μm) | Average peeling load (N) | Maximum peeling load (N) | Peel strength (N m−1) | Work-of-fracture (J m−2) |
---|---|---|---|---|---|
B. mori | 393 ± 21 | 0.35 ± 0.05 | 0.74 ± 0.17 | 62 ± 6 | 119 ± 19 |
S. cynthia | 480 ± 91 | 1.00 ± 0.45 | 1.58 ± 0.71 | 245 ± 99 | 437 ± 203 |
A. assamensis | 277 ± 29 | 1.21 ± 0.56 | 1.43 ± 0.40 | 240 ± 89 | 322 ± 121 |
A. pernyi | 387 ± 31 | 2.51 ± 0.55 | 4.45 ± 0.63 | 469 ± 75 | 981 ± 211 |
After tensile failure, among all the cocoon walls, only the A. pernyi showed a failed planar structure, all the other types turned completely fibrous due to the weaker bond in the 3D cocoon fibrous assembly (Fig. 3). It can be seen in the pulled B. mori silk fibres that the sericin shell detached from the fibroin core, indicating a weak bond between the fibroin and sericin. The fracture morphology shows the separation of the fibroin and sericin took place by the relative sliding of both surfaces. The S. cynthia silk exhibited a fibre split failure; the A. assamensis and the A. pernyi showed the ductile sericin matrix nature, which is in agreement with the reduced elastic modulus of these silk fibers as compared with B. mori (because of the large volume fraction of matrix which does not contribute to the fiber stiffness). Finally, the large elongation of wild silk fibers correlates well with the non-linear behaviour of composites prior to failure.26,27 In all the three types of silk fibers other than B. mori, the sericin and the fibroin are not distinguishable in the other silk types.
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Fig. 3 Tensile fracture of cocoon walls and enlarged view of broken silk fibers. (a) and (b) are B. mori; (c) and (d) are S. cynthia; (e) and (f) are A. assamensis; (g) and (h) are A. pernyi. |
Silk type | Single fiber cross-section area (μm2) | Young's modulus (GPa) | Maximum load (cN) | Maximum stress (MPa) | Strain at maximum stress (%) | Toughness (J m−3) |
---|---|---|---|---|---|---|
B. mori | 74 ± 2 | 13.3 ± 1.8 | 4.7 ± 0.81 | 635 ± 108 | 22 ± 5 | 1.0 × 108 |
S. cynthia | 196 ± 26 | 4.43 ± 0.60 | 5.6 ± 1.7 | 284 ± 88 | 34 ± 13 | 6.1 × 107 |
A. assamensis | 231 ± 22 | 5.70 ± 0.47 | 11.4 ± 1.1 | 495 ± 48 | 51 ± 6 | 1.4 × 108 |
A. pernyi | 350 ± 37 | 4.98 ± 0.56 | 14.9 ± 1.9 | 426 ± 55 | 51 ± 7 | 1.3 × 108 |
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Fig. 5 SPM topography of degummed silk fiber surfaces. (a) B. mori; (b) S. cynthia; (c) A. assamensis; (d) A. pernyi. The z-color bar on the left ranges from −65 to 65 nm. |
Increasing surface roughness of biomaterials has shown advantageous effects on the cell attachment for healing and bone formation.3 Silk fibroin is a native protein from silkworm fiber and is a remarkably stable and mechanically robust protein biomaterial, as evidenced by the ability to be autoclaved for sterilization and is amendable to ethylene oxide sterilization and gamma irradiation.28 It can be conveniently employed in tissue engineering systems, drug release systems, bio-optics and bioelectronics applications.1,29 The combination of excellent mechanical and surface properties of the wild A. pernyi silk fibroin may pave the way for its broader use for biomedical applications.
Using IGC at finite concentration conditions generates surface energy (total, dispersive, specific or polar) as a function of surface coverage. Surface heterogeneity of silk fibers has not been sufficiently studied in silk fibers, despite its importance in many applications. There are two types of surface heterogeneity: structural and energetic. The former refers to the distribution of pore size and shape, being mainly a geometrical effect determined by the correlation between probe molecule size and pore diameter, whereas the latter refers to the distribution of surface sites of distinct energetic levels including surface groups, impurities and/or surface irregularities.30 A completely flat line is indicative of an energetically homogeneous surface. The total surface energy traces (γTs) for four types of silk fibers are shown in Fig. 7. All samples are energetically heterogeneous since the surface energy changes as a function of surface coverage. The total surface energy of the A. pernyi fibers varies from a minimum average value of 44 mJ m−2 to a maximum value of 52 mJ m−2 and the total surface energy of the B. mori fibers varies from a minimum average value of 43 mJ m−2 to a maximum value of 52 mJ m−2. The range of the total surface energy for the S. cynthia is from 41 mJ m−2 to 47 mJ m−2 and that for the A. assamensis is from 45 mJ m−2 to 52 mJ m−2.
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Fig. 7 Total surface energy (γTs and dispersive surface energy (γDs for the degummed B. mori, S. cynthia, A. assamensis and A. pernyi silk fibers. |
The total surface energy (γTs) is made up of the dispersive (non-polar) interactions (γDs) and the specific (acid–base or polar) contributions (γABs). The dispersive component arises from London, van der Waals and Lifshitz forces31 and the acid–base component arises from Lewis acid–base interactions and hydrogen bonds.24 It can be seen from Fig. 7 and 8 that all the silk fibers are heterogeneous in both dispersive and acid–base surface energies. Dispersive surface energy (γDs) profiles in Fig. 7 show that all silk fibers are energetically active and heterogeneous. The dispersive surface energy for the four silk samples changes as a function of surface coverage (up to 20% of surface coverage). The A. pernyi and the A. assamensis silk fibers have higher γDs than the other two types. The A. assamensis silk fibers, in particular, also possess wider γDs distribution, ranging from 41 to 47 mJ m−2 compared to the B. mori (40–44 mJ m−2), S. cynthia (38-41 mJ m−2) and A. pernyi silk fibers (42–46 mJ m−2). Similar dispersive surface energy values for jute, silk floss, coir and sisal (41.9, 39.5, 39.1 and 38.4 mJ m−2, respectively) have been reported.32 The higher γDs of the A. pernyi and the A. assamensis silk fibers may be indicative of different surface groups with higher γDs. The wider γDs variation of the A. assamensis silk fibers indicates their surfaces contain more different levels of energetic sites.33 The higher γDs can also be an indication of more hydrophobic active sites. On the other hand, the polar surface energy profiles in Fig. 8 show energetically heterogeneous nature for all types of silks. In particular, the distribution of polar surface energy of the B. mori silk fibers varies from 3.5 to 7.5 mJ m−2, which is higher than other types. This may be due to the presence of more polar surface groups on the B. mori silks. However, all silk fibers were degummed by using the soap-soda method. During the degumming process, sericin is hydrolyzed and solubilized and at least one type of non-covalent interaction such as hydrogen bonds was weakened. Therefore the polar surface energy would be affected by degumming as the result that the acid–base component of the total surface energy arises from Lewis acid–base interactions and hydrogen bonds.
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Fig. 8 Polar surface energy (γABs), Gutmann acid (Ka) and base (Kb) number ratios for the degummed B. mori, S. cynthia, A. assamensis and A. pernyi silk fibers. |
The surface chemistry of the samples was assessed using the Gutmann acid (Ka) and base (Kb) numbers, determined based on the Gutmann approach. Values of the samples were calculated using the Gibbs free energy values of polar probes at that particular surface coverage. It is clearly seen from Fig. 8 that the base numbers (Kb) are consistently higher than the acid numbers (Ka) (Ka/Kb < 1), indicating that the surfaces are generally more basic in nature,34 which may be attributed to higher concentration of electron-donating surface functional groups. Fig. 8 shows that the acid–base ratios are higher for the B. mori and the A. assamensis silks which indicates that these silk samples possess marginally higher concentrations of electron-accepting surface functional groups. The work by Fowkes35,36 has indicated that the acid–base interactions, in which one phase acts as an electron donor (base) and the other acts as an electron acceptor (acid), play a significant role in interfacial adhesion. As a result, surface modification of the fibers and/or the matrix of composites must be performed to modify the acid–base interactions at the matrix–fiber interface in order to improve the mechanical performance of the composites constituted by these fibers.
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