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Transcript of How hydrophobically modified chitosans are stabilized by biocompatible lipid aggregates
Accepted Manuscript
How hydrophobically modified chitosans are stabilized by biocompatible lipid
aggregates
N. Ruocco, H. Frielinghaus, G. Vitiello, G. D’Errico, L.G. Leal, D. Richter, O.
Ortona, L. Paduano
PII: S0021-9797(15)00342-2
DOI: http://dx.doi.org/10.1016/j.jcis.2015.03.058
Reference: YJCIS 20369
To appear in: Journal of Colloid and Interface Science
Received Date: 23 January 2015
Accepted Date: 31 March 2015
Please cite this article as: N. Ruocco, H. Frielinghaus, G. Vitiello, G. D’Errico, L.G. Leal, D. Richter, O. Ortona,
L. Paduano, How hydrophobically modified chitosans are stabilized by biocompatible lipid aggregates, Journal of
Colloid and Interface Science (2015), doi: http://dx.doi.org/10.1016/j.jcis.2015.03.058
This is a PDF file of an unedited manuscript that has been accepted for publication. As a service to our customers
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1
How hydrophobically modified chitosans are stabilized by
biocompatible lipid aggregates
N. Ruocco,† H. Frielinghaus,‡ G. Vitiello,ʃ, ΨG. D’Errico,¶,ΨL. G. Leal,†
D. Richter,§,‡ O. Ortona,¶,Ψ and L. Paduano*,¶,Ψ
†Department of Chemical Engineering, University of California Santa Barbara, Santa
Barbara,
California 93106-5080,
‡Jülich Centre for Neutron Science, JCNS at MLZ, Forschungszentrum Jülich GmbH, 85747
Garching, Germany,
ʃ Department of Chemical, Materials and Production Engineering, University of Naples
“Federico II”, Piazzale Tecchio 80, 80125, Naples, Italy
ΨCSGI, Consorzio interuniversitario per lo sviluppo dei Sistemi a Grande Interfase, Florence,
Italy.
¶ Department of Chemical Sciences, University of Naples “Federico II”, Complesso di
Monte S. Angelo, via Cintia, 80126, Naples, Italy.
§Jülich Centre for Neutron Science, JCNS-1, Forschungszentrum Jülich GmbH, 52425 Jülich,
Germany
*E-mail: [email protected]
2
Abstract
Nanostructured hydrogels composed by biocompatible molecules are formulated and
characterized. They are based on a polymer network formed by hydrophobically modified
chitosans (HMCHIT or CnCHIT) in which vesicles of monoolein (MO) and oleic acid or
sodium oleate (NaO), depending on pH, are embedded. The best conditions for gel formation,
in terms of pH, length of the hydrophobic moieties of chitosan, and weight proportion among
the three components were estimated by visual inspection of a large number of samples.
Among all possible combinations, the system C12CHIT-MO-NaO in the weight proportion
(1:1:1) is optimal for the formation of a well-structured gel-like system, which is also
confirmed by rheological experiments. Electron paramagnetic resonance (EPR)
measurements unambiguously show the presence of lipid bilayers in this mixture, indicating
that MO-NaO vesicles are stabilized by C12CHIT even at acid pH.
A wide small angle neutron scattering investigation performed on several ternary systems of
general formula CnCHIT-MO-NaO shows that the length of the hydrophobic tail Cn is a
crucial parameter in stabilizing the polymer network in which lipid vesicles are embedded.
Structural parameters for the vesicles are determined by using a multilamellar model that
admits the possibility of displacement of the center of each shell. The number of shells tends
to be reduced by increasing the polymer content. The thickness and the distance between
consecutive lamellae are not influenced by either the polymer or MO-NaO concentration.
The hydrogel presented in this work, being fully biocompatible and nanostructured, is well-
suited for possible application in drug delivery.
3
I) Introduction
In the past and also presently, mixtures of polymers and surfactants are of major interest to
both technologists and scientists. The former are interested mainly due to the huge number of
combinations that these chemicals form and that can be used in multicomponent formulations
such as cosmetics, paints, food products, as well as drug delivery vehicles. The latter are
interested in understanding the thermodynamic reasons of their stability or instability and in
studying the microscopic structure of their aggregates [1-7]. In recent years, interest has been
mainly focused on systems formed by biocompatible polymers and surfactants [8-11]. In this
field, charged polysaccharides are of special interest due to their ready availability from
renewable sources, their biodegradability, and the absence of toxicity [12, 13]. Among these
biopolymers, chitosan plays a leading role, not only because it can be easily and plentifully
obtained from chitin deacetylation [14] but also for its antinflammatory and antimicotic
properties that are of special interest in pharmaceutical applications [15] Furthermore,
chitosan, being a charged polymer, is able to interact with charged surfactant molecules
[16,17]. Chitosan is a linear polysaccharide composed of randomly distributed D-
glucosamine and N-acetyl-D-glucosamine units. It can be obtained from crustacean shells by
deacetylation of chitin under alkaline conditions. This biopolymer can be easily modified [18,
19], due to the presence of two types of reactive groups onto which they can be grafted: the
free amine group on deacetylated units and the two hydroxyl groups on the gluco ring. The
chemical modification of chitosan can be performed in many different ways, allowing this
natural polymer to be the basis of applications in very different technological fields, such as
drug delivery, tissue engeneering, antimicrobial agents, metal ion absorption, dye removal,
viscosity control, and coating processes [20-23]. In the present report, we are concerned with
chemical modifications of chitosan. This has been obtained by grafting alkyl pendants of
different lengths to the free amine group of the saccharide unit, thus preserving its high
4
biocompatibility [20]. These chemical modifications have the aim of changing the
hydrophilic-lipophilic balance of this bio-polymer, giving rise to the formation of
hydrophobic pools that can interact with bio-compatible surfactant aggregates [24, 25]. In this
work, we investigate the interaction of these modified chitosans with anionic and non-ionic
surfactants, and analyze the microstructure of these mixtures.
Concerning the surfactants, monoolein (MO) is non-toxic, biodegradable, and biocompatible.
It has a polar head group and a non-polar hydrocarbon chain, clearly showing its amphiphilic
properties. This allows monoolein molecules to self-assemble into different liquid crystalline
structures, under varying conditions of temperature and solvent composition [26-28]. On the
basis of these properties, monoolein-based nanostructures represent a suitable strategy to
formulate useful drug delivery carriers, as well shown in literature [29-33].
Sodium oleate (NaO) is one of the main components (39% as oleic acid) of palm oil and is
the principal unsatured fat present in this natural material. As in the case of MO, NaO
aggregates in water giving rise to different structures depending on composition and
temperature [34]. In summary, both amphiphilic compounds show the tendency to aggregate
and are ecologically benign and mild. Taking into account that all compounds are
biocompatible, largely available, and affordable in the fields of food preparation and drug
delivery, we address the final goal of this paper, which is to determine the composition and
ratios among components that give rise to the formation of nanostructured gel-like systems.
In the context of their possible utilization as drug delivery systems, a quantitative analysis of
the microstructural characteristics of the CnCHIT-MO-NaO system deals with the aim to
obtain a deeper insight on the type of aggregates.
5
II) Experimental section
A. Materials
Chitosan (CHIT), classified by the supplier as medium molecular weight, batch 08028CD,
was purchased from Aldrich. Its acetylation degree was determined by NMR with a Varian
300 spectrometer to be 5%, which is in agreement with the value reported by the
manufacturer. Pentanal (97%), hexanal (98%), octanal (98%), decanal (99%), dodecanal
(92%), sodium cyanoborohydride NaCNBH3 (≥ 95%) and glacial acetic acid (~99.8%),
which were used for the alkylation procedure on the amine group, were all purchased from
Aldrich and used as received. We synthesized HMCHIT’s alkylating chitosan under mild
conditions following a reductive amination procedure suggested by Yalpani [18], and
successively modified by Rinaudo [35, 36]. The substitution degree of these alkylated
chitosans, from here on indicated as CnCHIT, is 10% as determined by nuclear magnetic
resonance (NMR), while their molecularweight is ~260kgmol-1. Monoolein (MO) and sodium
oleate (NaO) were provided by Danisco and BioChemica (Fluka), respectively, and were
used as received. For simplicity, from here on we will use the acronym NaO also in the case
of acidic solutions of sodium oleate in which only oleic acid is present. The EPR probes, 5-
doxylstearate (5-DSA) and 16-doxylstearate (16-DSA), were purchased from Sigma-Aldrich.
All solutions were prepared by weight using water obtained by inverse osmosis from an Elix
Millipore apparatus. Na2HPO4, citric acid, NaHCO3, and Na2CO3 components were used to
prepare buffer solutions with 3≤pH≤9. For SANS measurements all solutions were prepared
in heavy water (D2O) and, if necessary, in deuterated acetic acid (AcD), purchased from
Sigma-Aldrich.
B. Methods
Our aim is to study of the structures formed by CnCHIT, MO-NaO, and CnCHIT-MO-NaO
aqueous systems. The experimental approach follows three lines: i) visual inspection of
6
binary and ternary mixtures combined with a rheological analysis on the most successful
sample, ii) analysis of the structure of the aggregates by electron paramagnetic resonance
(EPR), and iii) determination of the aggregates structural parameters by small angle neutron
scattering (SANS).
1) Visual and Rheological Inspection
Several mixtures formed by CnCHIT and MO and NaO in different proportions and at
different pH conditions, were prepared by weight, left to rest overnight, and then visually
analysed.
The rheological experiments were performed with a rheometer AR-G2, which is an advanced
controlled stress instrument. The rheological flow and oscillatory experiments were made
with parallel plate geometry (diameter of 20mm). All the experiments were performed under
constant temperature, i.e. 25oC unless otherwise specified. Both frequency and flow sweeping
tests were rapidly performed after the hydrogel formation. The frequency sweeping tests were
used to obtain the viscoelastic behavior of the hydrogel in the linear regime. The experiment
was conducted isothermally in the frequency range 0.1<w<100rad/s. The stress strain was
kept constant at 1%.
The flow sweep experiments were made isothermally in the shear rate range 0.0001< <1s-1.
This range of shear rates allowed to determine the zero-shear viscosity (h0) and shear
thinning regime. The data points were collected once every 100s.
2) Electron paramagnetic resonance (EPR)
The EPR spectra were recorded using a 9 GHz Bruker Elexys E-500 spectrometer. Samples
were located in 25μL glass capillaries and flame sealed. Afterwards, the capillaries were
inserted in a quartz sample tube containing light silicone oil to provide thermal stability. The
7
experiments were carried out at 25°C. The instrumental setting for the spectra can be reported
as follows: sweep width, 120 G; resolution, 1024 points; time constant, 20.48 ms; modulation
frequency, 100 kHz; modulation amplitude, 1.0 G; incident power, 6.37 mW. The signal-to-
noise ratio was improved by collecting several scans (usually 32). The systems considered in
the present work are not paramagnetic and consequently, they are EPR silent. The EPR
analysis of the lipid aggregates microstructure was achieved by using suitable spin-probes,
such as 5-DSA and 16-DSA. The concentration of these probes in the mixtures was 5.2.10-6
mol L-1, i.e., less the 0.1 mol % of the total lipid concentration. This ratio is low enough to
avoid peak broadening due to spin exchange interaction. A semi-quantitative analysis of the
5-DSA spectra was done by measuring the outer hyperfine splitting, 2Amax, defined as the
difference (in Gauss) between the low-field maximum and the high-field minimum. 2Amax is
dependent upon both the amplitude (i.e., order) and rate of chain rotational motion, and is
therefore a useful parameter for characterizing chain dynamics in lipid aggregates [37, 38].
3) Small angle neutron scattering (SANS)
Small angle neutron scattering measurements were performed at the KWS1-FRM2-Garching
instrument with the wavelength λ=7Å and the corresponding spread Δλ/λ≤ 0.1 and at 25°C.
The two-dimensional (2D) scattering intensities in 128 by 128 channels were corrected
pixelwise for empty cell scattering, detector efficency, radial average and transformation to
absolute scattering cross sections were made with a secondary plexiglass standard [39, 40]
using QtiKWS software of the host institute. The experimental data were normalized to
absolute scale (cm-1) via calibration with the incoherent scattering [41, 42]. Two instrumental
configurations including two different collimation (C) and detecting (D) distances were used
(λ7ÅC8D8 and λ7ÅC8D2), underscripts are length in meters) to measure the scattering of the
neutrons by the samples. These configurations allowed data to be collected in the q-scattering
8
vector range: 2·10-3 Å-1<q<0.25 Å-1. In a general form, the scattering vector is defined as:
q = 4 n sin( / 2 ) , where n=1 for neutron scattering and θ is the scattering angle.
III) Results
A) Visualand Rheological Inspection
The effect of CnCHIT on the MO-NaO aqueous system was checked by visual inspection. In
Table 1, results are shown for several MO-NaO mixtures in the presence or absence of
CnCHIT’s with different lengths of the alkyl chain on the chitosan backbone. An
alphanumeric code is introduced to specify the composition of each mixture and what kind of
CnCHIT was used for each preparation. The general formula of the alphanumeric "Sample
Code" is CnCHIT(g1:g2:g3): Cn indicates the presence and the number of carbon atoms in
the chitosan alkyl chain; g1, g2, and g3 indicate the weight percentage of CnCHIT, MO, and
NaO, respectively. For example, the Sample Code C6CHIT(2:3:4) represents a ternary
mixture composed of C6CHIT at 2% w, MO at 3% w, and NaO at 4% w. HMCHIT or
CnCHIT polymers are soluble only if their amine functions are protonated, namely for pH≤ 5.
Thus, acetic acid at 1% by volume was used as the solvent for all the samples. If this is not
the case, it is indicated explicitly (see Samples 3-5 in Table 1).
Here, it is necessary to stress that, while the MO-NaO aqueous system is rather stable in
water at pH≥7, it is unstable for lower pH values (see Samples 1-5); the protonation of the
carboxyl group of the OA at low pH decreases the surface charge density of the membrane,
and also decreases the polarity of the membrane interface as widely discussed in the literature
[43]. Furthermore, the addition of hydrophobically modified chitosans to MO-NaO system
(Samples 12-28) shows different effects depending on the length of the aliphatic chain used
9
to modify CHIT. In fact, for unmodified chitosan or for short hydrophobic chains on the
polysaccharide backbone (see Samples 12-16), a precipitate is observed as a consequence of
the cited instability of MO-NaO aqueous systems at low pH values. The comparison among
samples 17 [C8CHIT(1:1:1)], 19 [C10CHIT(1:1:1)], and 23 [C12CHIT(1:1:1)] shows that by
increasing the aliphatic chain length of HMCHIT, the systems become increasingly stiff with
a gelatinous texture. In the case of Sample 23, a "wall-to-wall" gel is observed. The different
behavior of the samples: 3, 11, and 23 is shown in Fig. 1.
Figure 1: From left to right, MO-NaO (pH 9), C12CHIT and C12CHIT-MO-NaO systems(pH 4) are presented. The picture shows the increase of stiffness from (MO-NaO) or
(C12CHIT) solutions to the C12CHIT-MO-NaOgel.
This is an indication that, in spite of the instability of MO-NaO system in an acidic medium,
the presence of the CnCHIT with long aliphatic chains is able to avoid precipitation.
Furthermore, if we compare samples at increasing (MO+NaO)/C12CHIT ratios (Samples 23
and 24) or (MO+NaO)/C10CHIT ratios (Samples 19 and 20), it becomes evident that the
10
optimum weight proportion among components to get a well-structured gel is (1:1:1). The
visual analysis strongly indicates the presence of a gel-like system only at specific
compositions of CnCHIT and MO-NaO as reported in Table 1.
Therefore, the system C12CHIT(1:1:1) was selected for a detailed rheological analysis. In
Fig. 2, the oscillatory frequency experiment highlights the viscoelastic properties of the
material.
Figure 2: Dynamic oscillatory rheological characterization of C12CHIT(1:1:1). Frequency-sweep measurements provide viscoelastic insights in the linear regime
Generally, gels show G' (storage modulus) higher than G'' (loss modulus) all over the
investigated frequency range (0.1<w<100rad/s). From the mechanical spectrum, we can
distinguish between strong and weak gels [44]. A strong gel consists of moduli that are
"almost" parallel to each other and frequency independent. However, G' has a slope of zero
and G'' shows a minimum at intermediate frequencies [44, 45]. Furthermore, the storage
modulus is commonly 1-2 orders of magnitude bigger than the loss one. In soft gels, the
moduli can still be almost parallel but show a certain frequency dependence and the ratio
11
G''/G' exceeds 0.1, which is typical in soft tissues and biological gels [44, 46]. In the
C12CHIT(1:1:1) system, the averaged ratio is G''/G'~0.06 and moduli are rather low for a
well-structured gel (G’~130Pa and G’’~8Pa), thus a strict classification of the material as
weak or strong gel cannot be easily made, due to the hybrid characteristics.
In order to investigate the effect under flow of the material, a steady-state shear viscosity
analysis as function of the shear rate was performed and shown in Fig. 3.
Figure 3: Steady-state shear viscosity as function of shear rate of C12CHIT(1:1:1). Themeasurements determine the mechanical strength of the network-like system.
The shear rate dependence highlights a complex profile, which is characterized by a
Newtonian plateau, followed by intensive shear-thinning effects (~3orders of magnitude)
[47]. Here, the zero-shear viscosity is about 40600Pa.s and at intermediate shear rates the
viscosity profile shows ~ , these are characteristic values of densely organized structure.
The combination of the Newtonian plateau (low shear rates) and shear thinning effect
(intermediate and high shear rates) seems to be common to biological gels such as protein or
polysaccharide based networks [41].
12
Table 1: Visual analysis of the samples. If not expressly indicated the samples are preparedin acetic acid at 1% w.Systems prepared in water (*) and at pH 9 (**).
B) Electron paramagnetic resonance (EPR)
EPR investigation allows the morphology of the lipid aggregates (e.g., micelles vs. vesicles)
to be unambiguously identified both in aqueous solutions and in polymer hydrogels. The spin
Samplenumber
HMCHITw% MO %wt NaO
%wt Sample code Appearance
1 0.00 1.00 1.00 (0:1:1) Precipitate2 0.00 2.02 2.02 (0:2:2) Precipitate
3* 0.00 0.99 0.98 (0:1:1) Bluish fluid4** 0.00 0.52 0.50 (0:0.5:0.5) Bluish fluid5** 0.00 1.02 1.03 (0:1:1) Bluish fluid
6 1 0 0 C0 (1:0:0) Clear oil7 1.00 0.00 0.00 C5 (1:0:0) Clear oil8 1.00 0.00 0.00 C6 (1:0:0) Clear oil9 1.01 0.00 0.00 C8 (1:0:0) Clear oil
10 1 0 0 C10 (1:0:0) Clear oil11 1.01 0.00 0.00 C12 (1:0:0) Opalescent oil12 0.98 1.00 1.00 C0 (1:1:1) Precipitate13 1.01 1.00 1.01 C5 (1:1:1) Precipitate14 1.01 2.00 2.01 C5 (1:2:2) Precipitate15 0.99 1.00 1.00 C6 (1:1:1) Precipitate16 1.00 1.99 2.00 C6 (1:2:2) Precipitate17 1.00 1.00 1.00 C8 (1:1:1) Viscous oil and precipitate18 1.00 2.01 2.01 C8 (1:2:2) Viscous oil and precipitate19 1.01 1.00 1.01 C10 (1:1:1) Opaque weak gel20 1.01 2.02 2.02 C10 (1:2:2) Opaque viscous oil21 1.00 0.25 0.26 C12 (1:0.25:0.25) Opalescent viscous oil22 1.00 0.51 0.49 C12 (1:0.5:0.5) Opaque weak gel23 0.99 1.00 0.99 C12 (1:1:1) Opaque weak/strong gel24 1.02 2.01 2.00 C12 (1:2:2) Opaque weak gel25 0.13 1.02 1.04 C12 (0.1:1:1) Opaque fluid26 0.34 1.01 1.02 C12 (0.3:1:1) Opaque fluid27 0.51 1.02 1.03 C12 (0.5:1:1) Opaque viscous oil28 0.72 1.03 1.03 C12 (0.7:1:1) Opaque weak gel
13
probe 5-DSA is well-suited to this aim. 5-DSA is an amphiphilic molecule bearing a radical
nitroxide group close to the hydrophilic headgroup. Whenever inserted in supramolecular
aggregates formed by other amphiphiles, it monitors the structure and dynamics of the
aggregate/aqueous medium interphase. Particularly, 5-DSA shows an almost isotropic three-
line spectrum when embedded in micelles [48], while a well-resolved anisotropic line shape
is observed for vesicles [49].
MO-NaO (0:1:1) pH 9
C12CHIT-MO-NaO (1:1:1)
2Amax
= 50.5 ± 0.2 G
pH 4 2Amax
= 45.3 0.4 G
5-DSA
16-DSA
MO-NaO (0:1:1) pH 9
C12CHIT-MO-NaO (1:1:1) pH 4
±
2Amax
Figure 4: EPR spectra of 5-DSA and 16-DSA in the aggregates formed by MO-NaO at pH 9and C12CHIT-MO-NaO (1:1:1) at pH 4.
The spectra of 5-DSA in MO-NaO, registered both in water and in a buffer solution at pH 9,
show the anisotropic line shape typical of liposomes, see Fig. 4. No measure could be done at
acidic pH because of lipid precipitation. The presence of bilayered structure at pH 7 is in
qualitative agreement with the literature [26], in which the strong propensity of this mixture
to form a cubic phase in excess of water is shown evolving in reversed phases by increasing
14
monoolein content [50]. Nevertheless, the NaO and MO w% explored in this work is low
enough to exclude the formation of the cubic phase.
Interestingly, in the C12CHIT-MO-NaO gel, prepared at pH 4, 5-DSA also shows an
anisotropic line shape, as reported in Fig. 4. This is clear evidence that in these systems the
polymer inhibits lipid precipitation, and the bilayered structure of MO-NaO aggregates is
preserved. The significant reduction of the 2Amax value, indicated in the figure, is connected
to the different protonation state of the spin probe (i.e., protonated at pH 4 and deprotonated
at pH 9) [51] and consequently is scarcely informative on changes in bilayer fluidity.
To investigate the microstructure of lipid self-aggregates both in MO-NaO and C12CHIT-
MO-NaO systems, spectra of 16-DSA were also registered. 16-DSA bears the nitroxide group
close to the terminus of the hydrophobic tail, and thus monitors the deep interior of the lipid
aggregate. In all cases considered here, almost isotropic three-line spectra were observed,
indicating a fluid-like interior of the bilayers. A gradient in lipid ordering and dynamics in
going from the aggregate surface (monitored by 5-DSA) to its interior (monitored by 16-
DSA) is a hallmark of lipid bilayers in the liquid-crystalline phase [52, 53]. Thus, the EPR
results conclusively point to the presence of lipid bilayers, presumably in the vesicular form.
C) Small angle neutron scattering (SANS)
A SANS analysis was performed on several of the systems in Table 1 to detect the main
structural characteristics of the aggregates present in solution. SANS was used to highlight
some details at a mesoscopic level both for the binary and ternary chitosans as well as MO-
NaO aggregates.
15
1) Aggregates of hydrophobically modified chitosans
In Fig. 5, the scattering profiles of four hydrophobically modified chitosans are reported. A
quantitative analysis of the SANS data excludes the presence of compact micellar aggregates,
as for classical surfactants, thus indicating the presence of a more complex aggregation
system. The aggregation ability of these polymers has been highlighted in the past by
fluorescence studies [25]. According to the analysis of Esquenet [54] based on the work of
Semenov [55], these systems were interpreted as a network of intermolecularly bridged
flower-like aggregates.
10-4
10-2
100
102
104
106
0.001 0.01 0.1
x100
x101
x102
x103q-2.6
q-2.6
q-2.7
q-3.6
q-0.3»q-0.9:
q-1.2:
q-3.6
····
C12CHIT (1:0:0)C8CHIT (1:0:0)C6CHIT (1:0:0)C5CHIT (1:0:0)
(d/d
cm-1
1-q/Å
Figure 5: Scattering cross sections of hydrophobically modified chitosans with differentlength of the aliphatic chains at pH 4 and 25°C. Cross sections have been multiplied with ascale factor to allow a direct comparison. Error bars result inside the plotted points
On the basis of this interpretation and due to the lack of a quantitative theory, the discussion
will be limited to some qualitative aspects. Owing to the lack of very low q-region (the
Guinier region) for all samples, we can only state that the size of the network is above
experimental 2 /qmin, which is of the order of hundreds of Å. In the low q-range, the power
16
law of the scattering profile evolves from a ~q-2.6for the short chained polymers to a ~q-3.6in
the case of C12CHIT, suggesting a transition of the aggregate morphology.
The latter law corresponds to the presence of aggregates that are more compact. Furthermore,
in the intermediate q-range, 0.01Å-1<q<0.04 Å-1, the variation of the scattered intensity with q
shows a transition from a ~q-1observed for C6CHIT to a ~q-3.6dependence in the case of the
more hydrophobic C12CHIT. It may be recalled that a q-1dependence corresponds to the
characteristic rod-like behavior of the semi-rigid chitosan chains, whenever we look at length
scales that are smaller than the persistence length [56]. The crossover, at which the transition
between a ~q-3and ~q-1regime is observed, provides a qualitative evaluation of the length
scale at which the polymer begins to fold. Interestingly, the q-1 behavior is present only in the
case of chitosan polymers with a hydrophobic pendant of intermediate length, namely C6 and
C8CHIT. The absence of the q-1power law for the polymer with the longest pendant,
C12CHIT, is an indication that a more compact network dominates over a rod-like scattering
profile. In contrast with this observation, in the case of the polymer with the shorter aliphatic
chain (C5CHIT), this behavior is probably due to the high flexibility of the backbone in the
absence of well-structured hydrophobic pools that are able to stiff the chain.
2) Aggregates of Monoolein-Sodium oleate in solution
In Fig. 6, the binary system MO-NaO (0:1:1) is represented at two different pH conditions.
It can be observed that the different pH values deeply modify the scattering profiles. At pH 7
and low q-values, the Guinier region seems to be detected. In the case of MO-NaO system at
pH 9, the Guinier region is not observable, leading to the conclusion that we are in the
presence of large aggregates with complex morphology.
17
10-2
10-1
100
101
102
103
104
0.01 0.11-q/Å
(d/d
cm-1
x100
x101
q-3
q-0.7MO-NaO (0:1:1) pH 7
MO-NaO (0:1:1) pH 9·
:
:
Lamellarinterference
Figure 6: Scattering cross section of MO-NaO aggregates at pH 7 and 9. Solid linescorrespond to the values of the fitting model applied. Error bars result inside the plottedpoints
The scattering profile decay suggests that unilamellar vesicles dominate at pH 7, although
some multilamellar vesiscles (with a small number of layers) may be present . Whereas, at pH
9, the system is dominated by large and multilamellar vesicles as suggested by the power law,
~q-3, and confirmed by the presence of a lamellar interference peak at higher q-values [57].
On the basis of such evidence, the system at pH 7 was modeled as a collection of unilamellar
vesicles [58] while at pH 9 a multilamellar model [59] was preferred. The fitting parameters
are collected in Table 2. As a general comment we specify that in no one of the data analysis
by theoretical models of this paper we took into account the instrumental resolution.
In the case of the unilamellar vesicle model, a dilute system is considered, in which the
structure factor S(q) is 1 and the form factor P(q) provides the main contribution to the
scattering cross section. P(q) for a sphere with one shell can be written as:
18
( ) ( ) ( ) ( )1 1 2 1 1 2 2 1 2
1 2
23 - 3 -
( ) solv
shell
V J qR V J qRkP qV qR qR
é ù= +ê ú
ë û (1)
where k is a scale factor, Vshell is the volume of the shell, V1and V2 are the volume of the core
and the total volume, respectively. R1and R2 are the radii of the core and of the whole vesicle.
The values of ρsolv, ρ1, and ρ2are the scattering length densities of the solvent, of the shell and
of the core, respectively. 1( )J x is the Bessel spherical function of the 1storder:
( ) 2
sin - cosi
x x xJ xx
= (2)
The modeling approach assumes a Schulz-Zimm distribution function and a polydisperse
inner radius, while the thickness of the bilayer has negligible polydispersity in comparison
with R2. On the other hand, the oligolamellar system at pH 9 was interpreted by using the
Kotlarchyk-Ritzau model for the scattering of lamellar stacks with a paracrystalline distortion
[59]. For this model the form factor is represented by:
( ) ( )( )
22 2
22
sin / 21( ) 2/ 2
qP q S
q q= (3)
In Eq. 3, is the scattering length density difference between sheet and the solvent, S is the
area of the sheet per unit sample volume and the bilayer thickness. According to this
model, the structure factor is also able to extract parameters such as: the number of layers, N,
and their mean separation, l, as explained in references [59, 60]. As noted above, the low q-
regime in the Guinier region is missing, so the overall size of the vesicles cannot be obtained.
However, the scattering profile provides crucial information on the bilayer length scale
(middle q-region). The model for the pH 9 system considers that the thickness of the bilayer
and the distance l between consecutive lamellae can be polydisperse. The thickness is a
Gaussian function, which is described by the average value < > and the standard
19
deviation, , while l is a Schulz distribution characterized by the average value <l>. It can
be noted from the thickness of the bilayer that the amphiphiles are interdigitated, i.e. the
aliphatic chains are partially interpenetrated. In fact, the length of the 17 carbon hydrophobic
chain of the pendant is roughly 22Å, so that in the absence of interdigitation the bilayer
thickness would be at least 44Å, i.e. larger that the 30±2Å fitting value. This interdigitation is
also confirmed by the data on bilayer monoolein thickness in a cubic lattice [61] present in
literature.
Code pH R2/[Å] < > /[Å] N l< > /[Å]
(0:1:1) 7 290±20 28±2 1 -
(0:1:1) 9 N/A 30±2 2 135±3
Table 2: Structural parameters for MO-NaO aggregatesat pH 7and 9 at 25 °C.
3) Aggregates of hydrophobically modified chitosans and monoolein-sodium oleate in
solution
In Fig. 7, the profiles of the systems CnCHIT-NaO-MO (1:1:1) in AcD with different lengths
of the aliphatic chains are reported. It must be stressed here that in the absence of any HM-
chitosan and in acidic conditions, the system containing only MO and NaO is instable due to
oleate protonation. If HMCHIT is present, partial precipitation is still observed for systems
with the shorter aliphatic tails, namely C6-MO-NaO and C8-MO-NaO while a stiff gel is
obtained with C10-MO-NaO and C12-MO-NaO, confirming once more that the MO-NaO
aggregates are stabilized at low pH by the presence of only long-tailed HM-chitosan
molecules. The scattering data of C6 and C8CHIT ternary systems refer to the acidic
20
surnatant solutions. Nevertheless, all systems are strongly characterized by the presence of a
broad correlation peak at a high q-values.
10-2
100
102
104
106
108
10-3 10-2 10-11-q/Å
(d/d
cm-1
x100
x101
x102
x103
· C12CHIT-MO-NaO (1:1:1)
···
C10CHIT-MO-NaO (1:1:1)C8CHIT-MO-NaO (1:1:1)C6CHIT-MO-NaO (1:1:1)
q-2.94
q-2.74
Figure 7: Scattering cross section for CnCHIT-NaO-MO (1:1:1) aggregates for differentlengths of the aliphatic chain at pH 4 and 25 °C. Solid lines correspond to the values of theapplied fitting model. The systems C6CHIT-NaO-MO and C8CHIT-NaO-MO show aprecipitate, i.e. phase separation. Error bars result inside the plotted points
It will be noted that these SANS results are very different from the systems shown in Fig. 6,
which only contain oleine and sodium oleate at pH 7 and 9, respectively. Those were
interpreted just using a simple unilamellar vesicle model at pH 7 and a concentric multi-
lamellar model for the system at pH 9. In the case of the ternary system, we require a more
complex multilamellar model, proposed in the past [61, 62]. We will refer to this as the
Frielinghaus model. It is the only model that, to the best of our knowledge, can give an
explanation for the presence of the correlation peak at high q-values. This is attributed to the
fact that the center of each shell of the vesicle is allowed to shift with respect to its
21
predecessor. In this way, the hydrophobic pendants of the chitosan backbone in the ternary
systems may have full access to the bilayer of the MO-NaO vesicular shells, producing a
displacement of their center. The longer and more hydrophobic the pendant of the chitosan,
the more efficent its access to the bilayer and the stronger is this displacement. Due to the
complexity of the Frielinghaus model, we refer to the original paper for a more detailed
discussion [63]. In Fig. 7, the solid lines represent the results of this model, which is valid
only in the case of the more hydrophobic modified chitosans. In fact, short aliphatic pendants
allow precipitation.
The main parameters obtained by application of the Frielinghaus multilamellar model are
reported in Table 3, in which is the solutes volume fraction.
Code N < > /Å l< > /Å
C10CHIT(1:1:1) 0.0245 9±1 21±1 39±6
C12CHIT(1:1:1) 0.0269 7±1 24±1 39±6
Table 3: Main parameters for C10CHIT-NaO-MO and C12CHIT-NaO-MO aggregates atpH 4 and 25 °C.
In Fig. 8, the scattering data for C12CHIT (1:1:1) is compared to that of a C12CHIT(1:0:0)
aqueous solution. This comparison highlights that the qualitative “flower micelle” model
cannot be used to give an interpretation of the experimental results for the ternary system,
mainly due to the presence of the broad correlation peak at q~0.16 Å-1.
22
10-3
10-1
101
103
105
10-3 10-2 10-1
(d/d
cm-1
· C12CHIT-MO-NaO (1:1:1)C12CHIT (1:0:0)
q/A-1
Figure 8: Comparison between the scattering cross section of C12CHIT (1:0:0) andC12CHIT-NaO-MO (1:1:1) aggregates at pH 4 and 25 °C. Error bars result inside theplotted points
The characterization of the ternary systems was carried out also analysing scattering data at
fixed C12CHIT composition, but different MO and NaO contents. In Fig. 9, the SANS
profiles are reported. It is shown that the scattering maximum at q~0.16 Å-1 increases with
increasing (MO+NaO)/C12CHIT ratio.
By tuning the (MO-NaO)/C12CHIT ratio, it can be noted that the q-dependency in the
intermediate region, 5.5·10-3 Å-1<q<2.5·10-2 Å-1 for all the systems is almost constant, even
slightly decreasing for low MO-NaO content. This indicates a domain fully dominated by the
contribution of the C12CHIT network.
23
10-3
10-1
101
103
105
107
10-3 10-2 10-1
(d/d
cm-1
qMax
q-3.0
q-3.0
q-3.3
q-3.6
q-3.6
1-q/Å
x100
x101
x102
x103
x100
·····
C12CHIT-MO-NaO (1:2:2)C12CHIT-MO-NaO (1:1:1)C12CHIT-MO-NaO (1:0.5:0.5)C12CHIT-MO-NaO (1:0.25:0.25)C12CHIT (1:0:0)
Figure 9: Scattering cross section for C12CHIT-NaO-MO (1:g2:g3) aggregates at pH 4and 25 °C. Solid lines correspond to the values of the applied fitting model. Error barsresult inside the plotted points
In the case of more diluted vesicles, the peak at high q-values is less pronounced, due to a
low amount of surfactants. Both C12CHIT(1:0.25:0.25) and C12CHIT(1:0.5:0.5) provide
similar values for the number of shells, whereas this value decreases with increasing
surfactants concentration, e.g. the system C12CHIT(1:2:2) results in almost unilamellar
vesicles. This set of experiments shows the importance of the surfactants and C12CHIT
concentrationon the overall stability of the systems.
On the other hand, the fitted distance between bilayers assumes comparable values for all of
them, and it is in line with the values of max2 / q , which provides the periodicity of the
scattering planes. The main structural parameters obtained by the best fit of the applied model
[63] are reported in Table 4.
24
Code N < > /Å l< > /Å
C12CHIT(1:0.25:0.25) 0.00461 10±1 21±1 39±6
C12CHIT(1:0.5:0.5) 0.0106 13±1 20±1 39±6
C12CHIT(1:1:1) 0.0269 7±1 24±1 39±6
C12CHIT(1:2:2) 0.0522 2±1 33±1 41±6
Table 4: Main structural parameters measured for C12CHIT-NaO-MO (1:g2:g3) aggregatesat pH 4 and 25 °C
The whole of these experimental results can be reasonably interpreted to suggest the
existence of two zones for the C12CHIT(1:0.25:0.25) and C12CHIT(1:0.5:0.5) systems: in
the first one the polymer HMCHIT interacts directly with the vesicles, determining a
backbone-bilayer connection and linking consecutive bilayers in the single multilamellar
aggregate; in the secondzone the polymer does not have any connection with the vesicles. By
increasing the MO-NaO contentas for the C12CHIT(1:1:1) and C12CHIT(1:2:2) systems, the
two zones disappear, converging to a single zone whereas vesicles with a lower number of
shells are present. The reason for this behavior could be ascribed to the greater surfactants
concentration, which is large enough to occupy all HMCHIT locations. Thus, the systems
have the tendency to form vesicles with a minor number of shells. Another set of
measurements, which helps to fully understand the matter is reported in Fig. 10, wherein the
system C12CHIT-MO-NaO in AcD for various polymer concentrations (from 0.1%w to
1%w) and fixed MO-NaO composition, were investigated. The results of fitting this data,
shown in Table 5, indicate that the number of shells tends to decrease if the polymer
concentration is is increased. Nevetheless, thickness and inter-distance separation of the
bilayers are comparable with the previous experiments.
25
10-2
100
102
104
106
108
10-3 10-2 10-11-q/Å
(d/d
cm-1
C12CHIT-MO-NaO (1:1:1)C12CHIT-MO-NaO (0.7:1:1)C12CHIT-MO-NaO (0.5:1:1)C12CHIT-MO-NaO (0.3:1:1)C12CHIT-MO-NaO (0.1:1:1)
···
··
x100
x101
x102
x103
x104
Figure 10: Scattering cross section for C12CHIT-NaO-MO (g1:1:1) aggregates at pH 4 and25 °C. Solid lines correspond to the values of the applied fitting model. Error bars resultinside the plotted points
Code N < > /Å l< > /Å
C12CHIT(0.1:1:1) 0.0106 15±2 20±1 37±6
C12CHIT(0.3:1:1) 0.0125 13±1 20±1 38±6
C12CHIT(0.5:1:1) 0.0130 16±2 20±1 38±6
C12CHIT(0.7:1:1) 0.0129 9±1 21±1 39±6
C12CHIT(1:1:1) 0.0269 7±1 34±1 39±6
Table 5: Main parameters of C12CHIT-NaO-MO (g1:1:1) aggregates at pH 4 and 25 °C.
26
The ternary system C12CHIT-MO-NaO is strongly influenced by the polymer concentration.
For low C12CHIT concentrations, the surfactant aggregates are separated from the chitosan
backbone. The reason for this behavior is because the amount of polymer is not high enough
to build up locations able to contain the vesicles. On the other hand, at higher concentration,
the C12CHIT can form a polymeric network, which incorporates the vesicles. This means
that, by tuning the polymer content together with the amount of MO-NaO, we have direct
control of the system, e.g. number of lamellae N and vesicular dimensions.
Conclusions
Finally, we conclude that the visual and rheological analysis allowed to determine the best
conditions for gel formation by varying pH, length of the hydrophobic chain of the CnCHIT,
and the weight ratio between the three components. The optimum condition was obtained for
the system C12CHIT-MO-NaO in acetic acid 1%v, with 1% by weight for each component
(1:1:1). The use of C12CHIT improves the conditions for aggregation of the system, due to
its long hydrophobic pendant; the MO-NaO weight ratio equal to 1 insures the presence of
vesicular aggregates, and the acidic pH provides the conditions necessary to solubilize the
polymer and build up a network-like system. Overall, it appears that by increasing the
aliphatic chain length the system becomes more rigid, adopting a gel texture for C12CHIT.
As regards the MO-NaO content, there is a precise (MO+NaO)/ C12CHIT weight ratio, i.e. 2,
that insures the formation of a gel. In fact, for both higher and lower ratios, namely 0.5 and 4,
the gels become less rigid and stiff. We can speculate that for (MO+NaO)/ C12CHIT< 2 the
number of vesicles is too low with respect to the number of the Cn chains on the polymer
backbone. Therefore, the formation of a three dimensional network due to the insertion of the
aliphatic chains inside the MO-NaO bilayer is less efficient. In contrast, for (MO+NaO)/
C12CHIT>2, the number of vesicles is too high in comparison to the aliphatic chain
27
concentration, so that a large number of vesicles cannot take part to the three dimensional
network.
The frequency and flow sweeping tests have showed the main macrostructural and
mechanical properties of the sample C12CHIT-MO-NaO (1:1:1), resulting in a material with
polyvalent characteristics. Indeed, the sample provided hybrid viscoelastic properties
(soft/strong gel) and common features of well-structured biological systems (Newtonian
plateau and shear thinning).
The EPR results unambiguously show the presence of bilayers in the C12CHIT-MO-NaO
(1:1:1) system, highlighting the stability of these structures even in acidic pH conditions. A
very complete SANS analysis was performed on several ternary systems of the general
formula CnCHIT-MO-NaO. The results highlighted and confirmed that the length of the
hydrophobic tail Cn is a crucial parameter to stabilize the polymer network, probably
organized as a system of flower-like aggregates. In the absence of chitosans the system MO-
NaO is stable only in non-acidic conditions and is organized as bilayer or vesicular structures.
The presence of long tailed chitosans allows the stabilization of the MO-NaO aggregates
even in acidic conditions. Indeed, the tuning of the components in the ternary system leads to
the conclusion that among all possible combinations, the system C12CHIT-MO-NaO in the
weight proportion 1:1:1 is optimal for the formation of a very stiff gel, in which multilamellar
vesicles of MO-NaO are embedded.
For ternary systems, structural parameters for the vesicles were determined using a
multilamellar model that admits the possibility of displacement of the center of each shell.
The thickness and the distance between consecutive lamellae are not influenced by either the
polymer concentration or the MO-NaO composition, while the number of shells and
consequently the vesicle dimensions increase by decreasing the surfactant content at constant
C12CHIT w/w% as well as by decreasing (MO+NaO) w/w% at constant chitosan
28
concentration. A possible explanation could be that the high surfactant content leads to
smaller compartments. This offers more options for polymer anchoring, while high polymer
content tends to smaller compartments too, through stronger binding of surfactants.
Ultimately, the dimensions and the number of vesicle shells can be modulated at will by
varying surfactants and chitosan composition, thus creating a flexible system very suited for
delivery of hydrophobic and hydrophilic drugs.
29
Bibliography
[1] Roscigno, P.; Paduano, L.; D’Errico, G.; Vitagliano, V. Langmuir, 2001, 17, 4510-4518.
[2] Lee, J. H.; Gustin, J. P.; Chen, T.; Payne, G. F.; Raghavan, S. R. Langmuir, 2005, 21, 26-
33.
[3] Chen, Y.; Javvaji, V.; MacIntire, I. C.; Raghavan, S. R. Langmuir, 2013, 29, 15302-
15308.
[4] Huang, W.; Wang, Y.; Zhang, S.; Huang, L.; Hua, D.; Zhu, X. Macromolecules, 2013, 46,
814−818.
[5] Lott, J. R.; McAllister, J. W.; Arvidson, S. A.; Bates, F. S.; Lodge T. P.
Biomacromolecules, 2013, 14, 2484−2488.
[6] Dowling, M. B.; Kumar, R.; Keibler, M. A.; Hess, J. R.; Bochicchio, G. V; Raghavan, S.
R. Biomaterials, 2011, 32, 3351-3357.
[7] Hao, X.; Liu, H.; Xie, Y.; Fang C.; Yang, H. Colloid Polym.Sci., 2013, 291, 1749-1758.
[8] Bao, H.; Li, L.; Gan, L. H.; Zhang, H. Macromolecules, 2008, 41, 9406-9412
[9] Mangiapia, G.; Ricciardi, R.; Auriemma, F.; De Rosa, C.; Lo Celso, F.; Triolo, R.;
Heenan, R. K.; Radulescu, A.; Tedeschi, A. M.; D'Errico, G.; Paduano, L. J. Phys. Chem. B,
2007, 111, 2166–2173.
[10] Lee, J. H.; Agarwal, V.; Bose, A.; Payne, G. F.; Raghavan, S. R. Phys. Rev. Lett., 2006,
96, 048102.
[11] Chiappisi, L.; Prevost, S.; Grillo, I.; Gradzielski, M. Langmuir, 2014, 30, 10608-10616.
[12] Chiappisi, L.; Prevost, S.; Grillo, I.; Gradzielski, M. Langmuir, 2014, 30, 1778-1787.
[13] Alonso-Sande, M.; Cuña, M.; Remuñán-López, C.; Teijeiro-Osorio, D.; Alonso-Lebrero,
J. L.; Alonso, M. J. Macromolecules, 2006, 39, 4152-4158
[14] Tolaimate, A.; Desbrieres, J.; Rhazi ,M.; Alagui ,A.; Vincendon ,M.; Vottero, P.
Polymer, 2000, 41, 2463–2469.
[15] Liu, S.; Maheshwari, R.; Kiick, K. L. Macromolecules, 2009, 42, 3-13.
[16] Zhu, C.; Lee, J. H.; Srinivasa, R.; Raghavan, S. R.; Payne, G. F. Langmuir, 2006, 22,
2951-2955.
[17] Mangiapia, G.; Frielinghaus, H.; D’Errico,G.; Ortona, O.; Sartorio, R.; Paduano, L.
Phys. Chem. Chem. Phys., 2007, 9, 6150–6158.
[18] Yalpani, M.; Hall, L.D. Macromolecules, 1984, 17, 272-281.
30
[19] Marcasuzaa, P.; Reynaud, S.; Ehrenfeld, F.; Khoukh, A.; Desbrieres, J.
Biomacromolecules, 2010, 11, 1684–1691.
[20] Lim, S-H.; Hudson, S.H. J. Macromol. Sci., Part C, Polym. Rev., 2003, 43, 223-269
[21] Ge, Y.; Zhang, Y.; He, S.; Nie, F.; Teng, G.; Gu, N. Nanoscale Res. Lett., 2009, 4, 287-
295.
[22] Rassaei, L.; Sillanpaa, M.; Edler, K. J.; Marken, F. Electroanalysis, 2009, 21, 261-266.
[23] Zemljič, L. F.; Peršin, Z.; Stenius, P. Biomacromolecules, 2009, 10, 1181–1187.
[24] Mangiapia, G.; Frielinghaus, H.; D’Errico, G.; Ortona, O.; Sartorio, R.; Paduano, L.;
Phys. Chem. Chem. Phys., 2007, 9, 6150–6158.
[25] Ortona, O.; D’Errico, G.; Mangiapia, G.; Ciccarelli, D. Carbohydr. Polym., 2008, 74,
16-22.
[26] Borné, J.; Nylander, T.; Khan, A. Langmuir, 2001, 17, 7742-7751.
[27] Ferreira, D. A.; Bentley, M. V. L. B.; Karlsson, G.; Edwards, K. Int. J. Pharm., 2006,
310, 203-212.
[28] Angelova, A.; Angelov, B; Mutafchieva, R.; Lesieur, S.; Couvreur, P. Acc. Chem. Res.,
2011, 44, 147-156.
[29] Angelov, B.; Angelova, A.; Filippov, S.; Drechsler, M.; Stepanek, P.; Lesieur, S. ACS
Nano, 2014, 8, 5216-5226.
[30] Angelov, B.; Angelova, A.; Garamus, V. M.; Drechsler, M.; Willumeit, R.; Mutafchieva,
R.; Stepanek, P.; Lesieur, S., Langmuir, 2012, 28, 16647-16655.
[31] Angelov, B.; Angelova, A.; Papahadjopoulos-Sternberg, B.; Hoffmann, S. V.; Nicolas,
V.; Lesieur, S. J. Phys. Chem. B, 2012, 116, 7676-7686.
[32] Angelov, B.; Angelova, A.; Filippov, S.; Karlsson, G.; Terrill, N.; Lesieur, S.; Stepanek,
P. Soft Matter, 2011, 7, 9714-9720.
[33] Angelov, B.; Angelova, A.; Vainio, U.; Garamus, V. M.; Lesieur, S.; Willumeit, R.;
Couvreur P. Langmuir, 2009, 25, 3734-3742.
[34] Antunes, F.E.; Coppola, L.; Gaudio, D.; Nicotera, I.; Oliviero, C. Colloids and Surfaces
A: Physicochem. Eng. Aspects, 2007, 297, 95–104.
[35] Rinaudo, M.; Auzely, R.; Vallin, C.; Mullagaliev, I. Biomacromolecules, 2005, 6, 2396-
2407.
[36] Desbrieres, J.; Martinez, C.; Rinaudo, M. Int. J. Biol. Macromol., 1996, 19, 21-28.
[37] Lange, A.; Marsh, D.; Wassmer, K. H.; Meier, P.; Kothe, G. Biochemistry, 1985, 24,
4383–4392.
31
[38] Vitiello, G.; Fragneto, G.; Petruk, A. A.; Falanga, A.; Galdiero, S.; D’Ursi, A. M.;
Merlino, A.; D’Errico G. Soft Matter, 2013, 9, 6442–6456.
[39] Russell, T. P.; Lin, J. S.; Spooner, S.; Wignall, G. D. J. Appl. Cryst., 1988, 21, 629-638.
[40] Wignall, G. D.; Bates, F. S. J. Appl. Cryst., 1987, 20, 28-40.
[41] Ruocco, N.; Dahbi, L.; Driva, P.; Hadjichristidis, N.; Allgaier, J. ; Radulescu, A.; Sharp,
M;. Lindner, P.; Straube, E.; Pyckhout-Hintzen, W.; Richter, D. Macromolecules, 2013, 46,
9122-9133.
[42] Frielinghaus, H.; Frielinghaus, X.; Ruocco, N.; Allgaier, J.; Pyckhout-Hintzen, W.;
Richter, D. Soft Matter, 2013, 9, 10484-10492.
[43] Aota-Nakano, Y; Li, S.J.; Yamazaki, M. Biochimica et Biophysica Acta , 1999, 1461,
96-102.
[44] Clark A. H.; Murphy, S. B. Adv. Polym. Sci., 1987, 83, 57-192.
[45] Hua, X.; Tang, Y.; Wang, Q.; Li, Y.; Yang, J.; Du, Y.; Kennedy J. F. Carbohydr.
Polym., 2011, 83, 1128–1133.
[46] Barbucci, R. “Hydrogels: Biological Properties and Applications”, Ed. Springer, 2010,
Milan.
[47] Popescu, M. T.; Mourtas, S.; Pampalakis, G.; Antimisiaris, S. G.; Tsitsilianis; C.
Biomacromolecules, 2011 12, 3023-3030.
[48] Kang, Y. S.; Kevan, L. J. Phys. Chem.,1994, 98, 7624–7627.
[49] McCarney, E. R.; Armstrong, B. D.; Kausik, R.; Han, S. Langmuir, 2008, 24, 10062-
10072.
[50] Angelov, B.; Angelova, A.; Mutafchieva, R.; Lesieur, S.; Vainio, U.; Garamus, V. M.;
Jensena, G. V.; Pedersena, J. S. Phys. Chem. Chem. Phys., 2011, 13, 3073–3081.
[51] Sulkowski, W. W.; Pentak, D.; Nowak, K.; Sulkowska, A. Journal of Molecular
Structure, 2006, 792-793, 257-264.
[52] Vitiello, G.; Falanga, A.; Galdiero, M.; Marsh, D.; Galdiero, S.; D'Errico, G. Biochim.
Biophys. Acta Biomembranes,2011, 1808, 2517–2526.
[53] Vitiello, G.; Di Marino, S.; D’Ursi, A. M.; D'Errico, G. Langmuir, 2013, 29, 14239–
14245.
[54] Esquenet, C.; Terech, P.; Boué F.; Buhler, E. Langmuir, 2004, 20, 3583-3592.
[55] Semenov, A. N.; Rubinstein, M. Macromolecules, 2002, 35, 4821-4837.
[56] Muller, F.; Manet, S.; Jean, B.; Chambat, G.; Boué, F.; Heux, L.; Cousin, F.
Biomacromolecules, 2011, 12, 3330–3336.
32
[57] Mangiapia, G.; D’Errico, G.; Simeone, L.; Irace, C.; Radulescu, A.; Di Pascale, A.;
Colonna, A.; Montesarchio, D.; Paduano, L. Biomaterials, 2012, 33, 3770-3782.
[58] Guinier, A.; Fournet, G. "Small-Angle Scattering of X-Rays", John Wiley and Sons,
1955, New York.
[59] Kotlarchyk, M.; Ritzau, S. M. J. Appl. Cryst.,1991, 24, 753-758.
[60] Harvey, R. D.; Barlow, D. J.; Drake,A. F.; Kudsiova, L.; Lawrence, M. J.; Brain, A. P.
R.; Heenan, R. K. J. Colloid Interf. Sci., 2007, 315, 648-661.
[61] Angelov, B; Angelova, A.; Garamus, V. M.; Lebas, G.; Lesieur, S.; Ollivon, M; Funari,
S. S.; Willumeit, R.; Couvreur, P. J. Am. Chem. Soc., 2007, 129, 13474-13479.
[62] Angelova, A.; Angelov, B.; Garamus, V. M.; Couvreur, P.; Lesieur, S. J. Phys. Chem.
Lett., 2012, 3, 445-457.
[63] Frielinghaus, H. Phys. Rev. E, 2007, 76, 0516031-0516038.