Upload
somenath
View
215
Download
2
Embed Size (px)
Citation preview
ORIGINAL PAPER
Anticancer and immunostimulatory role of encapsulated tumorantigen containing cobalt oxide nanoparticles
Sourav Chattopadhyay • Sandeep Kumar Dash • Totan Ghosh •
Sabyasachi Das • Satyajit Tripathy • Debasis Mandal •
Debasis Das • Panchanan Pramanik • Somenath Roy
Received: 27 February 2013 / Accepted: 30 August 2013 / Published online: 17 September 2013
� SBIC 2013
Abstract The purpose of this study is to evaluate the
prospect of using surface modified cobalt oxide(CoO)
nanoparticles as carriers of cancerantigens to human mac-
rophages. N-Phosnomethyliminodiacetic acid (PMIDA)
was used for surface modification to overcome the toxic
effect of CoO nanoparticles. Here, the phosphonate group
of the PMIDA acts as a surface-anchoring agent and the
remaining –COOH groups bind nonspecifically with tumor
associated antigens. This modification allows the conju-
gation of human oral carcinoma (KB) cell lysate (CL) as an
antigen with PMIDA coated CoO nanoparticles (CL–
PMIDA–CoO). Particle characterization was performed by
dynamic light scattering, atomic force microscopy, and
scanning electron microscopy studies. Fourier transform IR
spectroscopy was used to investigate conjugation of the
protein with nanoparticles. Protein encapsulation was
confirmed by protein gel electrophoresis. Active uptake of
antigen-conjugated nanoparticles by macrophages was
confirmed by fluorescence microscopy. The antitumor
activity of the nanocomplex pulsed macrophages was
investigated on a human oral carcinoma cell line (KB)
in vitro. The modified nanocomplexes upregulate IFN-cand TNF-a and induce an anticancer immune response by
activating macrophages. The use of TNF-a inhibitor con-
firmed the ability of the CL–PMIDA–CoO nanocomplex to
stimulate TNF-a mediated immunostimulation. CL–PMI-
DA–CoO nanoparticles efficiently increased the CD4?
population. Thus, our findings provide insight into the use
of PMIDA coated CoO nanoparticles as antigen delivery
vehicles.
Keywords Cobalt oxide nanoparticle � Antigen
delivery � Macrophage � TNF-a � CD4? �Immunotherapy
Abbreviations
AFM Atomic force microscopy
ASA Acetylsalicylic acid
cAMP Cyclic adenosine monophosphate
CL Cell lysate
CL–PMIDA–CoO Cell lysate conjugated
N-phosnomethyliminodiacetic
acid coated cobalt oxide
COX Cyclooxygenase
DC Dendritic cell
DLS Dynamic light scattering
EDC N-Ethyl-N0-(3-dimethylaminopropyl)-
carbodiimide
FCS Fetal calf serum
IFN-c Interferon-c
Electronic supplementary material The online version of thisarticle (doi:10.1007/s00775-013-1044-y) contains supplementarymaterial, which is available to authorized users.
S. Chattopadhyay � S. K. Dash � S. Das � S. Tripathy �D. Mandal � S. Roy (&)
Immunology and Microbiology Laboratory,
Department of Human Physiology with Community Health,
Vidyasagar University, Midnapore
721102, West Bengal, India
e-mail: [email protected]
T. Ghosh � D. Das
Department of Chemistry,
University of Calcutta,
92 A.P.C Road, Kolkata
700009, West Bengal, India
P. Pramanik
Nano Materials Laboratory,
Department of Chemistry,
Indian Institute of Technology,
Kharagpur, West Bengal, India
123
J Biol Inorg Chem (2013) 18:957–973
DOI 10.1007/s00775-013-1044-y
iNOS Inducible nitric oxide synthase
MTT 3-(4,5-Dimethylthiazol-2-yl)-2,5-
diphenyltetrazolium bromide
NP Nanoparticle
PBS Phosphate-buffered saline
PMIDA N-Phosnomethyliminodiacetic acid
PMIDA–CoO N-Phosnomethyliminodiacetic acid
coated cobalt oxide
POF Pentoxifylline
RBC Red blood cell
SDS-PAGE Sodium dodecyl sulfate
polyacrylamide gel electrophoresis
SEM Scanning electron microscopy
Th1 Type 1 T helper
Th2 Type 2 T helper
Introduction
The use of nanoparticles (NPs) in biomedical applications
is attracting interest owing to their wide range of biotech-
nological applications in drug delivery systems [1], vaccine
administration [2], and cell separation [3]. Biodegradable
and biocompatible NPs are widely established for delivery
of protein antigens to a variety of cell types, including
dendritic cells (DCs), and have induced immunity in ani-
mals [4]. Some scientists have shown the importance of
ligand density in the outcome of an immune response to a
DC targeted NP-based vaccine delivery system [5].
Poly(lactic-co-glycolic acid) mediated antigen delivery is
more efficient than conventional soluble lysate in evoking a
favorable cytolytic CD8? T cell driven antitumor response
in vitro [6].
Metal NPs are also promising tools for delivery of
protein antigens to antigen presenting cells, including DCs,
and have induced an antitumor immune response. Single
walled carbon nanotubes successfully delivered peptide
antigens and generated an immunoresponse [7]. Metal NPs
are attracting interest especially in advanced biomedical
applications [8], including drug and gene delivery [9–11]
and protein antigen delivery [12].
Cobalt is an organometallic compound and also a bio-
polymer [13]. Cobalt has a physiological role as a cofactor
of vitamin B12. Cobalt cannot be regarded only as an
essential element. Among cobalt-based NPs, particularly
cobalt oxide (CoO) NPs are currently attracting enormous
interest owing to their unique size and shape dependent
properties and potential applications, such as pigments,
catalysis, sensors, electrochemistry, magnetism, and energy
storage [14]. Cobalt-based magnetic fluids have been
designed for possible use in medical applications owing to
the better magnetic properties and greater effects on proton
relaxation [15]. Recent developmental work has largely
focused on the use of new metal NPs such as cobalt and
nickel NPs. Cobalt NPs have the ability to enter to the cell
very rapidly [16], which has drawn the interest of
researchers to biomedical application systems based on
cobalt NPs.
Magnetic cobalt NPs are used in drug delivery in eye
surgery to repair detached retinas [17, 18]. However, the
use of cobalt NPs is restricted because of their toxicity.
Recently, it has been understood that polymeric or inor-
ganic coatings on magnetite/maghemite NPs can overcome
the toxicity issue [19]. This modification involves the
chemical modification of the surface of the magnetic NPs
with organophosphorus compounds, which offer a prom-
ising alternative in the coupling of organic components to
metal oxides [20]. The bonding of organophosphorus
molecules to the inorganic phase results from the formation
of strong M–O–P bonds through heterocondensation and
coordination. Homocondensation with the formation of P–
O–P bridges is unlikely, and such bridges are not stable in
the presence of water. Organophosphorus coupling agents
react specifically with metal oxide surfaces and assist only
monolayer formation. The resulting monolayers are highly
stable under physiological conditions [21, 22].
This study aimed to develop a potent antigen delivery
vehicle using N-phosnomethyliminodiacetic acid (PMIDA)
coated CoO (PMIDA–CoO) NPs. Our previous report
showed that PMIDA–CoO NPs have anticancer activity
without affecting normal cells [23]. In this article, we
intend to establish that PMIDA–CoO NPs have the ability
to bind with tumor-associated antigens and act as an
effective antigen delivery carrier to stimulate macrophages
and to evaluate the macrophage-mediated killing of oral
cancer cells in vitro.
Materials and methods
Chemicals and reagents
PMIDA, crystal violet, 3-(4,5-dimethylthiazol-2-yl)-2,5-
diphenyltetrazolium bromide (MTT), histopaque 1077,
acetylsalicylic acid (ASA), indomethacin, pentoxifylline
(POF), N-ethyl-N0-(3-dimethylaminopropyl)carbodiimide
(EDC), and rhodamine 123 were procured from Sigma (St.
Louis, MO, USA). Anti-CD4? antibody was purchased
from Partec (Germany). Minimum essential medium,
RPMI 1640, fetal calf serum (FCS), penicillin, streptomy-
cin, sodium chloride, sodium carbonate, sucrose, Hanks
balanced salt solution, ethylenediaminetetraacetate, and
dimethyl sulfoxide were purchased from Himedia (India).
Tris(hydroxymethyl)aminomethane–HCl,
958 J Biol Inorg Chem (2013) 18:957–973
123
tris(hydroxymethyl)aminomethane buffer, KH2PO4, K2HPO4,
HCl, formaldehyde, alcohol, and all other chemicals of the
highest purity grade were procured from Merck (Mumbai,
India).
Culture of the cancer cell line
The oral carcinoma cell line (KB) was obtained from the
National Centre for Cell Sciences (Pune, India) and was
cultured in MEM (Minimum essential medium) medium
supplemented with 10 % FCS, 100 U/ml penicillin,
100 lg/ml streptomycin, and 4 mM L-glutamine under a
5 % CO2 and 95 % humidity atmosphere at 37 �C for
in vitro experiments.
Cell lysate preparation of the KB cell line
The cell suspension was collected in a centrifuge tube and
centrifuged at 1,500 rpm for 5 min. The supernatant was
decanted, and the cell pellets were resuspended in ice cold
phosphate-buffered saline (PBS) at concentrations from
2 9 105 cells per milliliter and were subjected to four
freeze thaw cycles (alternating liquid nitrogen and 37 �C
water bath treatment) followed by sonication (ultrasonic
processor, Tekmar, Cincinnati, OH, USA) for 20 s on ice.
Lysates were centrifuged at 12,000 rpm for 20 min at 4 �C
to remove cellular debris. Supernatants were collected and
stored at -20 �C [6]. The protein content of the lysate
preparations was measured according to the method
described by Lowry et al. [24] using bovine serum albumin
as a standard.
Synthesis of cell lysate conjugated PMIDA–CoO NPs
PMIDA–CoO NPs were prepared by a thermal decompo-
sition technique, and were characterized by X-ray diffrac-
tion, dynamic light scattering (DLS), and transmission
electron microscopy studies as described in our previous
report [23]. PMIDA–CoO NPs (10 mg/ml) were suspended
into 5 ml PBS (pH 7.4). Six hundred microliters of lysed
cell suspension containing a protein concentration of 5 mg/
ml and 5 mg/ml EDC was added to the solution. The entire
solution was stirred in the dark for 12 h, and the particles
were separated by centrifugation at 10,000 rpm for 12 min.
Assessment of protein encapsulation and protein release
rate
The rate of release of proteins from NPs was measured
during incubation under controlled conditions [25]. A
sticky mass of 5 mg of NPs was suspended in 1 ml of PBS
and was incubated at 37 �C for different time intervals with
continuous agitation in an orbital shaker incubator. After
the incubation, the suspension was centrifuged at
10,000 rpm for 5 min at 37 �C. The supernatant was ana-
lyzed for the total protein content according to the method
described by Lowry et al. [24]. The release efficiency was
calculated using the following formula:
Cumulative protein released=total protein content of NPsð Þ� 100 %:
Sodium dodecyl sulfate polyacrylamide gel
electrophoresis analysis
To assess whether a representative selection of tumor-
associated proteins was encapsulated and released, the
protein compositions of preencapsulation and postencap-
sulation samples were compared on sodium dodecyl sulfate
polyacrylamide gel electrophoresis (SDS-PAGE) gels by
using Coomassie brilliant blue staining. A portion of the
tumor lysate suspension served as the preencapsulation
sample. Protein samples were then boiled with 69 sample
buffer run on 12 % SDS-PAGE gels and stained with
Coomassie brilliant blue to visualize protein bands [6].
Characterization of cell lysate conjugated
PMIDA–CoO NPs
Dynamic light scattering
DLS analysis was done with a Zetasizer Nano ZS (Malvern
Instruments) according to the method of Chakraborty et al.
with some modifications. The concentration of the CoO
NPs was 100 lg/ml, the CoO NPs were sonicated for
2 min, and dynamic particle sizes were measured by sus-
pending two drops of an aqueous suspension of NPs in
10 ml of Millipore water. When the NPs had completely
dispersed in water, they were analyzed with a DLS ana-
lyzer. The experiments were repeated several times to
obtain the average size of the NPs [23].
Atomic force microscopy
The size and surface topography of a drop-coated film of
cell lysate (CL) conjugated PMIDA–CoO (CL–PMIDA–
CoO) NPs were investigated by atomic force microscopy
(AFM; NanoScope, 111a MultiMode, Veeco Instruments,
USA), and high-resolution surface images were produced.
In AFM characterization, the contact mode (NP10) with a
silicon probe over scan sizes of 10 lm was used [26].
Scanning electron microscopy
The particle size and microstructure were studied by high-
resolution scanning electron microscopy (SEM; instrument
from Nikon, Japan) according to the method of Ghosh et al.
J Biol Inorg Chem (2013) 18:957–973 959
123
with some modifications. In brief, CL–PMIDA–CoO NPs
were suspended in deionized water at a concentration of
1 mg/ml and then the sample was sonicated using a soni-
cator bath until the sample formed a homogenous suspen-
sion. For size measurement, the sonicated stock solution of
CL–PMIDA–CoO NPs (0.5 mg/ml) was diluted 20 times.
SEM was used to characterize the size and shape of the
PMIDA–CoO NPs [26].
Surface morphology analysis by Fourier transform IR
spectroscopy
The conjugation of CL with PMIDA–CoO NPs was
investigated by Fourier transform IR spectroscopy with a
PerkinElmer Spectrum RX I Fourier transform IR system
with a frequency ranging from 500 to 4,000 cm-1 and a
resolution of 4 cm-1. The KBr pellet method was used to
prepare the samples [26].
Isolation of macrophages and lymphocytes from peripheral
blood mononuclear cells
Fasting blood samples were collected from all groups of
individuals satisfying the Helsinki protocol. The peripheral
blood mononuclear cells were isolated from heparinized
blood samples according to the method of Hudson and Hay
[27]. Blood was diluted with PBS (pH 7.0) in an equal ratio
and then layered very carefully on the density gradient
(histopaque 1077) in a 1:2 ratio and centrifuged at
1,400 rpm for 20 min. The white milky layer of mononu-
clear cells was carefully removed and cultured in RPMI
1640 medium supplemented with 10 % FCS, 100 U/ml
penicillin, 100 lg/ml streptomycin, and 4 mM L-glutamine
under a 5 % CO2 and 95 % humidity atmosphere at 37 �C
for 2 h. After 2 h, the nonadherent layer of the cultured
cells was washed twice with PBS and centrifuged at
2,000 rpm for 10 min to obtain the required pellet of
lymphocytes. The adherent portion was cultured for 8 days
to obtain monocyte-derived macrophages.
Macrophage pulsing
Macrophages (104 cells per milliliter) were pulsed with
25 lg/ml CL–PMIDA–CoO NPs and 25 lg/ml ovalbumin
antigen in complete RPMI 1640 medium for 24 h at 37 �C
[8]. The dose of NPs was selected on the basis of our
previous report [23].
The cytotoxicity of protein–CoO NPs toward macrophages
and lymphocytes
Normal human lymphocytes and macrophages were seeded
into 96 wells of tissue culture plates containing 180 ll of
complete medium and were incubated for 48 h. Ovalbumin
antigen and CL–PMIDA–CoO NPs were added to the cells
at different concentrations (1, 5, 10, and 25 lg/ml), and the
mixtures were incubated for 48 h at 37 �C in a humidified
incubator (NBS) maintained at 5 % CO2. The cell viability
was estimated by MTT assay according to our previous
report [23]. The plates were read on a microplate reader
(model 550, Bio-Rad, Tokyo, Japan) at a wavelength of
570 nm. Cytolysis was calculated as a percentage.
Hemolysis assay
Ethylenediaminetetraacetic acid stabilized human blood
samples were freshly obtained from healthy subjects
according to the Hay protocol. First, 5 ml of blood sample
was added to 10 ml of PBS, and then red blood cells
(RBCs) were isolated from serum by centrifugation at
10,016g for 10 min. The RBCs were further washed five
times with 10 ml of PBS. The purified RBCs were diluted
to 50 ml with PBS. RBCs were incubated with deionized
water and with PBS and were used as the positive and
negative controls, respectively. Then, 0.2 ml of diluted
RBC suspension was added to 0.8 ml of CL–PMIDA–CoO
NP solutions at systematically varied concentrations and
mixed by gentle vortexing. The CL–PMIDA–CoO NPs
suspended in PBS solutions with different concentrations
were prepared immediately before RBC incubation by
serial dilution. All the sample tubes were kept in a static
condition at room temperature for 12 h. Finally, the
mixtures were centrifuged at 10,016g for 3 min, and
100 ll of the supernatant of all samples was transferred to
a 96-well plate for measurement of the hemoglobin con-
centration. The absorbances of the supernatants at 570 nm
were determined using a microplate reader with the
absorbance at 655 nm as the reference [28]. The con-
centration of hemoglobin was calculated using the fol-
lowing formula:
Hemoglobin gm=dlð Þ ¼ ðsample absorbancesÞ=ðHb standard absorbanceÞ � concentration of Hb standard:
ð1Þ
Cancer cell co-culture with pulsed macrophages
The pulsed macrophages were collected by trypsinization
and were centrifuged at 1,500 rpm for 5 min. The pellet
cells were washed with PBS at room temperature. After
they had been washed three times, the cells were resus-
pended in RPMI 1640 medium with 5 % FCS. KB cells
were plated in culture plates at a density of 4 9 104 cells
per well and were incubated in minimum essential medium
with 5 % FCS for 24 h at 37 �C. After the adherence of KB
cells to the plate, pulsed macrophages were added to each
960 J Biol Inorg Chem (2013) 18:957–973
123
well in a ratio of 5:1 or 10:1 (macrophages to cancer cells)
and were then incubated for 1, 3, and 5 days at 37 �C [29].
Cancer cell viability assay
After co-culture, each well was washed with sterile saline
to remove the macrophages and dead KB cells. The sur-
viving KB cells were stained with 0.1 % crystal violet/
methanol at room temperature for 10 min. The plates were
read on a microplate reader (model 550, Bio-Rad, Tokyo,
Japan) at an wavelength of 570 nm. Cytostasis was cal-
culated as a percentage. The absorbance of surviving KB
cells in the absence of macrophages (control absorbance)
was set at 100 %, and the experimental absorbance was
divided by the control absorbance [29].
Uptake of protein-CoO NPs by macrophages
Macrophages (104 cells per milliliter) were pulsed with
25 lg/ml rhodamine 123 tagged CL–PMIDA–CoO NPs in
complete RPMI 1640 medium for 3 h at 37 �C. After they
had been washed twice with ice cold PBS, the cells were
incubated with 0.25 % trypsin in PBS for 3 min at 37 �C.
The cells were then fixed with 1 % paraformaldehyde in
ice-cold PBS. A fluorescence image of the cells was taken
with a phase-contrast fluorescence microscope at 9400
magnification [25].
NO release assay
The NO concentration was measured by a microplate assay
method with Griess reagent (1 % sulfanilamide, 0.3 %
naphthylethylenediaminedihydrochloride, 7.5 % H3PO4).
Briefly, culture supernatants (100 ll) were mixed with
100 ll of Griess reagent. The nitrite concentration in the
culture supernatant was measured at a wavelength of
550 nm after 10 min of mixing [30].
Co-culture of pulsed macrophages with lymphocytes
The pulsed macrophages were plated at 2 9 103 cells per
well. Lymphocytes were then added to the culture plate in a
ratio of 5:1 (macrophages to lymphocytes) and the mixture
was then incubated for 24 h at 37 �C [31]. After co-culture,
each well was washed with sterile saline. The cells were
stained with 0.1 % crystal violet/methanol at room tem-
perature for 10 min. The plates were read on a microplate
reader (model 550, Bio-Rad, Tokyo, Japan) at a wave-
length of 570 nm. Cytostasis was calculated as a percent-
age. The absorbance of surviving lymphocytes in the
absence of macrophages (control absorbance) was set at
100 %, and the experimental absorbance was divided by
the control absorbance [30].
Flow-cytometric analysis of CD4? cells
Lymphocyte surface markers were detected using mono-
clonal antibodies against CD4? conjugated with different
fluorochromes (Partec, Germany). After treatment, lym-
phocytes were incubated for 30 min at room temperature
with fluorescein isothiocyanate conjugated anti-human
CD4? monoclonal antibody. After three washings, samples
were resuspended in PBS and analyzed with a BD FAC-
SCalibur flow cytometer. The results are given as the
percentage of positively stained cells. The percentage of
CD4? T cells from different groups are shown as repre-
sentative histograms [6].
Cytokine analysis
To investigate the effect of CL–PMIDA–CoO NPs on
cytokine production, an ELISA technique was used for the
determination of interferon-c (IFN-c), TNF-a, and IL-12
production. Freshly prepared human-monocyte-derived
macrophages were cultured at 1 9 105 cells per milliliter
and were treated with various concentrations of CL–PMI-
DA–CoO (1–25 lg/ml) for 24 h. After treatment of the
NPs, cell-free supernatants were harvested via successive
10-min centrifugations (2,000, 7,000, and 13,000 rpm) and
were stored at -80 �C until analysis. ELISA was per-
formed by the protocol of eBiosciences kits, with all
samples analyzed in triplicate.
Incubation with POF
Human blood macrophages were isolated from heparinized
blood by histopaque density centrifugation as previously
described. Macrophages were co-cultured with cancer cells
in a ratio of 1:10 for 1, 3,and 5 days in RPMI medium
alone, and with 1 mM POF [32]. After incubation, cell
viability was measured by crystal violet cell proliferation
assay [30].
Incubation with ASA and indomethacin
In another experiment, ASA and indomethacin at final
concentrations of 1 mM and 50 lM [33], respectively,
were included in the reaction mixture of pulsed macro-
phages and target cells, and the protocol described in the
previous section was followed [30].
Protein estimation
Protein content was determined using bovine serum albu-
min as a standard according to the method of Lowry et al.
[24].
J Biol Inorg Chem (2013) 18:957–973 961
123
Statistical analysis
The data were expressed as the mean ± the standard error
of the mean (n = 6). Comparisons between the means of
control and treated groups were made by one-way analysis
of variance (using the statistical package Origin 6.1;
OriginLab, Northampton, MA, USA) with multiple com-
parison t tests, and p \ 0.05 as the limit of significance.
Results and discussion
NPs have been used successfully to deliver macromole-
cules such as drugs, protein, genes, and human growth
factors [6]. For these purposes, different NPs have been
used, such as poly(lactic-co-glycolic acid)-coated NPs,
poly(ethylene glycol)-coated NPs, and metal NPs. Metal
NPs have been used successfully for separation of proteins,
drug delivery [34], and vaccination [7]. Recently, Cho et al.
[35] proved that CoO NPs could be a very useful adjuvant
where both type 1 T helper (Th1) and type 2 T helper
(Th2) responses are needed to clear pathogens. In our study,
we have tried to deliver antigen (CL) against oral cancer
cells (KB) to macrophages by PMIDA–CoO NPs, to
establish a potent anticancer immunotherapy.
Synthesis of PMIDA–CoO and CL–PMIDA–CoO NPs
We synthesized CoO NPs by a calcination method using
COCl2 as raw material. It was modified by conjugating
0 5 10 15 20 25
0.0
0.5
1.0
1.5
2.0
2.5
*
*
*
Pro
tein
con
cent
ratio
n (m
g/m
l)
Time point in hour
% of Protein release
Protein release assay
0 5 10 15 20 25
1.5
2.0
2.5
3.0
3.5
4.0
4.5
5.0
5.5
*
*
*
*
% of Protein concentration in sup
Con
cent
ratio
n of
pro
tein
(m
g/m
l)
Time point in hourProtein concentration in sup
0 5 10 15 20 250
10
20
30
40
50
60
70
*
*
*
Pro
tein
con
cent
ratio
n (m
g/m
l)
Time point in hour
% of Protein encapsulation with NP
Protein encapsulation with NP
a b
c
Fig. 1 a The percentage of protein encapsulated by nanoparticles
(NPs), b the percentage of protein in the supernatant (sup), and c the
percentage of protein released from the NPs. n = 6; values are
expressed as the mean ± the standard error of the mean. Asterisks
indicate a significant difference as compared with the control group
962 J Biol Inorg Chem (2013) 18:957–973
123
PMIDA, which led to the formation of a stable aqueous
dispersion nanocluster. The formation of NPs was con-
firmed by X-ray diffraction, DLS, and transmission elec-
tron microscopy [23]. Conjugation of PMIDA with CoO
NPs was determined by Fourier transform IR spectroscopy
[23]. Then, the PMIDA–CoO NPs were stirred with cancer
cell lysate following incubation for 12 h. The pellet was
collected by centrifugation at 14,000 rpm for 20 min. It
was washed with deionized water three times and dried for
further experiments.
Characterization of CL–PMIDA–CoO NPs
Encapsulation of tumor-associated antigens in polymeric
NPs is a promising approach to enhance the efficiency of
antigen delivery for antitumor vaccines [6]. Here, we report
that PMIDA–CoO NPs were successfully bound with
cancer cell lysate antigens. Encapsulation of cancer cell
lysate antigens by NPs depends on the exposure time,
because increased protein encapsulation was observed with
increasing exposure time (Fig. 1). The concentration of
cancer cell lysate bound NPs was 63.23 % after 24 h
(Fig. 1a).
Protein (CL antigens) release was found to be time-
dependent. This finding was due to the large concentration
gradient between the CL–PMIDA–CoO complex and the
outer water phases [36, 37]. The biphasic release pattern is
potentially useful for delivery of antigens to DCs, as it
provides a continuous supply of antigens to the DCs [38].
CL–PMIDA–CoO NPs contain tumor lysate antigens of
different molecular weights. We observed the protein
release rate increased with the incubation time (Fig. 1c).
The size distribution of CL–PMIDA–CoO NPs in
aqueous medium was characterized by DLS. The mean size
of the NPs in aqueous solution was 120 ± 20 nm, as
shown in Fig 2a. This study of the NPs further confirmed
the presence of stable protein-tagged CoO NPs.
The morphology of the CL–PMIDA–CoO NPs was
studied by AFM and SEM. The AFM image and SEM
morphology of CL–PMIDA–CoO NPs showed they have
nearly spherical geometry with a mean size of
90 ± 15 nm. This finding is represented in Fig. 2b and c.
The presence of some bigger particles is attributed to
aggregation or overlapping of some small particles. The
observed NP size was approximately larger than the
hydrodynamic diameter obtained from the DLS experi-
ment. SEM describes the size in the dried state of the
sample, whereas DLS measures the size in the hydrated
state of the sample, so the size measured by DLS was a
hydrodynamic diameter and was larger. However, one has
to bear in mind that by SEM analysis we measured the
image of dried particles, whereas DLS gives an average
size estimation, which is biased toward the larger-size end
of the population distribution.
The conjugation of cancer cell lysate with PMIDA–CoO
NPs was investigated by Fourier transform IR spectros-
copy, which showed a sharp peak at 648 cm-1, indicating
the presence of M-O-M vibration, and it was shifted from
the characteristic IR band of CoO NPs at 566 cm-1 [23].
The bands in the regions of 1,078 and 1,238 cm-1 were
60 80 100 120 140 1600
20
40
60
80
Num
ber
(%)
Meandiameter (nm)
a
b
c
Fig. 2 a Dynamic light scattering histogram of the cell lysate (CL)-
conjugated N-phosnomethyliminodiacetic acid (PMIDA)-coated
cobalt oxide (CL–PMIDA–CoO) NPs, b Atomic force microscopy
image of CL–PMIDA–CoO NPs, and c scanning electron microscopy
picture of CL–PMIDA–CoO NPs
J Biol Inorg Chem (2013) 18:957–973 963
123
mainly due to the symmetric and asymmetric stretching
modes of phosphodiester groups, respectively [39, 40]. The
peaks at 1,216, 1,440, 1,666, and 3,464 cm-1 were clearly
separated and were assigned to the stretching vibrations of
the amide group and the hydroxyl group, respectively,
which were the typical protein absorption peaks. The peaks
observed at 1,072 and 2,922 cm-1 correspond to C–H
bonding due to the formation of a coordination bond
between CL and CoO (Fig. 3a, b) [41].
To confirm the protein encapsulation and release of
tumor lysate tagged CoO NPs, whole cell lysate was sub-
jected to electrophoretic separation on SDS-PAGE gels
followed by staining. Prominent bands were observed
which indicate tumor protein encapsulation (Fig. 3c). The
conjugations of protein with NPs were facilitated by EDC
and N-hydroxysuccinimide. EDC and N-hydroxy-
succinimide reacted with the surface carboxylate (–COOH)
group on the NP to yield an O-acylisourea active
intermediate. This intermediate was then attacked by a
primary amine (–NH2) group of the protein’s lysine side
chain, forming a stable covalent bond between the protein
and the NP [42].
Effect of CL–PMIDA–CoO NPs on macrophages
and lymphocytes
The toxicity of the CL–PMIDA–CoO NPs toward normal
human macrophages and lymphocytes in vitro was
checked. CL–PMIDA–CoO NP mediated cytotoxicity
toward these normal cells was measured by MTT assay
[34]. It was found that there was no significant difference in
cell viability between the cells treated with CL–PMIDA–
CoO NPs and the cells treated with ovalbumin antigen. The
cell proliferation assay showed that ovalbumin antigen
(25 lg/ml) increased the macrophage population up to
1.02-fold and the lymphocyte population up to 1.14-fold
Fig. 3 Fourier transform IR spectra of CL (a) and CL–PMIDA–CoO (b). c Sodium dodecyl sulfate polyacrylamide gel electrophoresis analysis
of the marker (lane 1), cancer cell lysate (lane 2), and CL–PMIDA–CoO complex (lane 3)
964 J Biol Inorg Chem (2013) 18:957–973
123
compared with the negative control. Hence, these NPs are
safe for biomedical applications (Fig. 4a).
Hemolytic activity
The hemolytic potentials of CL–PMIDA–CoO NPs were
assessed by incubating NPs with human RBCs for 12 h,
followed by colorimetric analysis of the hemoglobin
released. The CL–PMIDA–CoO NPs displayed no hemo-
lytic activity. The surface functionalization with cellular
protein made these metal NPs biocompatible nanocom-
plexes (Fig. 4b, c).
Effect of CL–PMIDA–CoO NP pulsed macrophages
on KB cells
The cytotoxicity of CL–PMIDA–CoO pulsed macrophages
toward KB cells was considerable (Fig. 5). We compared
all the results by using ovalbumin antigen as a positive
control. The result showed a high level of cytotoxicity
when KB cells were co-cultured with CL–PMIDA–CoO
pulsed macrophages and ovalbumin pulsed macrophages.
Our result suggested that CL–PMIDA–CoO pulsed mac-
rophages have greater cytotoxicity toward KB cells in
comparison with ovalbumin pulsed macrophages. As
shown in Fig. 5a, during the co-culture of pulsed macro-
phages with KB cells in a ratio of 5:1, there was a low
amount of cell killing on day 3 (30.36 %), but on day 5 the
killing was higher (46.22 %). At a ratio of 10:1, a signifi-
cant amount of KB cell killing induced by pulsed macro-
phages was observed on day 3 (35.62 %) and on day 5
(54.82 %) (Fig. 5b). All the results were significant at the
p \ 0.05 level.
Uptake of CL–PMIDA–CoO NPs by macrophages
The cellular internalization of NPs is an endocytic process
[43]. Cargo binds to the plasma membrane and is inter-
nalized into membrane-bound endocytic vesicles that are
transported through the cell by motor proteins moving
along the cytoskeleton [44]. From the fluorescence images
(Fig. 6), the CL–PMIDA–CoO nanocomplex was found to
be distributed in the cytoplasm, leaving a clear zone for the
nucleus, indicating cellular uptake instead of adhesion to
the surface and the NPs preferentially targeted the cancer
cells and were internalized. This internalization might be
due to the receptor-mediated endocytosis [34, 45, 46].
NO release
Stimulated macrophages secreted several cytotoxic factors
such as TNF-a and NO [47–49]. This clearly demonstrated
that the cytotoxic factors were secreted by the macrophages
when stimulated with the CL–PMIDA–CoO complex and
ovalbumin antigen. In the presence of the CL–PMIDA–
CoO complex and ovalbumin antigen, single culture of
macrophages generated a significant amount of NO
(p \ 0.05) in the medium after 1, 3, and 5 days of incu-
bation (Fig. 7a). Our result showed the presence of a high
concentration of NO in the co-culture medium of pulsed
macrophages and KB cells on day 3 (27.65 %, 59.65 %)
and day 5 (45.85 %, 62.85 %) for ratios of 5:1 and 10:1,
respectively (Fig. 7b, c), since the amount of this NO was
(+)v
e Con
trol
(-)ve
Con
trol
1 µg
/ml
5 µg
/ml
10 µ
g/m
l
25 µ
g/m
l
0.0
0.5
1.0
1.5
2.0
2.5
3.0
3.5
* ****
Con
cent
ratio
n of
Hb
(gm
/dl)
CL-PMIDA-CoO NP
0 5 10 15 20 25
0.9
1.0
1.1
1.2
1.3
1.4
1.5
1.6
***
***
* **
**
Cel
l Via
bili
ty
Nanoparticles (µg/ml)
Macrophage + TAA-PMIDA-CoO NP Lymphocytes + TAA-PMIDA-CoO NP Macrophage + OVA Lymphocytes + OVA (-)Ve Control
a
b
Fig. 4 a Cytotoxicity of ovalbumin (OVA) antigen and CL–PMIDA–
CoO NPs toward normal human lymphocytes and macrophages.
b Estimation of hemolytic activity of CL–PMIDA–CoO NPs against
normal human red blood cells. n = 6; values are expressed as the
mean ± the standard error of the mean. Asterisks indicate a
significant difference as compared with the control group. Hb
hemoglobin, TAA tumor-associated antigen
J Biol Inorg Chem (2013) 18:957–973 965
123
correlated with the cytotoxicity toward KB cells. In the
presence of ASA and indomethacin, the NO release was
54.65 % on day 3 and 69.85 % on day 5 for the highest
ratio (Fig. 7d). Several studies have evaluated the rela-
tionship between inducible nitric oxide synthase
(iNOS) and cyclooxygenase (COX)-2. However, most of
the previous works did not evaluate how COX-2 influ-
ences iNOS expression. For instance, NO donor and
NO derivatives such as peroxynitrite (ONOO2) have
been reported to induce COX-2 expression [50, 51]
Peroxynitrite, the coupling product of NO and superoxide,
activates both COX-1 and COX-2 [52]. Another report
[53] demonstrated that low-dose NO induces COX-2
expression in macrophages in which NO was found to
inhibit apoptosis. Moreover, there have been several
observations that suggest an interaction between COX-2
and iNOS. Both enzymes are expressed in the same
population of colonic epithelial cells in ulcerative colitis
patients, as well as in Barrett’s esophagus and esophageal
adenocarcinomas [45, 54]. In vitro, peroxynitrate, which
E: T- 5:1
a
Day 1 Day 3 Day 5
0
20
40
60
80
100
**
*
**
**
*
% o
f cel
l via
blity
Macrophage / KB cell
KB Cells Normal Macrophages+KB Cells
OVA pulsed Macrophages+KB Cells
CL-PMIDA-CoO pulsed Macrophages+KB Cells
E: T- 10:1
Day 1 Day 3 Day 5
0
20
40
60
80
100
**
*
**
**
*
% o
f cel
l via
blity
Macrophage / KB cell
KB Cells Normal Macrophages+KB Cells
OVA pulsed Macrophages+KB Cells
CL-PMIDA-CoO pulsed Macrophages+KB Cells
E: T- 10:1
Day 1 Day 3 Day 5
0
20
40
60
80
100*
*
*
*
*
*
*
% o
f cel
l via
blity
Macrophage / KB cell
KB Cells Normal Macrophages+KB Cells
OVA pulsed Macrophages+KB Cells
CL-PMIDA-CoO pulsed Macrophages+KB Cells
b
c
Fig. 5 Cytotoxicity of CL–PMIDA–CoO NP pulsed macrophages
co-cultured with KB cells at ratios of macrophages to KB cells of 5:1
(a) and 10:1 (b). n = 6; values are expressed as the mean ± the
standard error of the mean. Asterisks indicate a significant difference
as compared with the control group
966 J Biol Inorg Chem (2013) 18:957–973
123
is derived from NO and O2, has been shown to activate
COX [50–52].
Effect of CL–PMIDA–CoO NP pulsed macrophages
on lymphocytes
Macrophages have several important physiological
applications, including initiation of acquired immunity
such as antigen processing and presentation, production of
cytotoxic factors such as oxygen species or NO, activation
of T cells, and secretion of the cytokines that regulate
acquired immunity. The proliferation of lymphocytes with
the co-culture of pulsed macrophages clearly established
that the amount of proliferation of lymphocytes was
comparable to that with CL–PMIDA–CoO pulsed mac-
rophages (Fig. 8a). In this experiment we showed the
viability of lymphocytes but not CD4? or CD8? cells
specifically though as they are the specific marker. From
this study we tried to show the viability profile by co-
culturing freshly isolated lymphocytes with pulsed mac-
rophages, and we reveled that lymphocyte proliferation
was increased (nonsignificant at p \ 0.05) in the presence
of pulsed macrophages in culture medium. The potential
activation of primary immune cells by PMIDA–CoO NPs
is the key parameter that helps in the generation of an
anticancer immune response. After incubation with CL–
PMIDA–CoO NPs at a concentration of 25 lg/ml for 24
h, the percentage of CD4? cells was significantly
increased (Fig. 8b). PMIDA–CoO NPs promoted differ-
entiation of T cells (1.61 % in ovalbumin and 1.56 % in
CL–PMIDA–CoO NPs) and made the Th1/Th2 balance
move to the Th1 type, by significantly increasing the
CD4? cell count.
Cytokine estimation from CL–PMIDA–CoO NP pulsed
macrophages
After treatment, cell-free supernatants were used to quan-
tify cytokine levels using an ELISA. The results demon-
strated significant dose-dependent increases in the levels of
IFN-c and TNF-a at all NP concentrations tested. The
results showed that macrophages increased the production
of IFN-c by 1.44-, 1.69-, 1.75-, and 2.39-fold, TNF-a by
1.91-, 2.18-, 2.5-, and 2.76-fold, and IL-12 by 1.1-, 1.29-,
1.87-, and 2.96-fold compared with negative controls at NP
doses of 1, 5, 10, and 25 lg/ml, respectively (Fig. 9).
Nanomaterials have been shown to modulate expression of
cytokines, which are soluble biological protein messengers
that regulate the immune system. Published studies have
demonstrated the ability of certain nanomaterials to induce
cytokine production, although this appears heavily depen-
dent on a variety of factors, including material composi-
tion, size, and method of delivery [55]. Much remains to be
learned, however, regarding the proinflammatory potential
of CL–PMIDA–CoO NPs. Studies were performed to
evaluate the ability of NPs to modulate IFN-c, TNF-a, and
IL-12 cytokine production in primary human immune cells
(Fig. 9). These particular cytokines were chosen because
they represent critical pathways that are involved in the
inflammatory response and differentiation processes. The
results demonstrated significant dose-dependent increases
in the levels of IFN-c, IL-12, and TNF-a at all NP con-
centrations tested. This results confirmed the activation of
macrophages by pulsing with CL–PMIDA–CoO NPs. CL–
PMIDA–CoO NPs were capable of inducing some key
components of inflammation such as IFN-c, TNF-a, and
IL-12 in vitro. CL–PMIDA–CoO NPs induce high levels of
TNF-a, help to promote Th1 differentiation [56, 57], and
function as a regulator of acute inflammation [58]. The
ability of CL–PMIDA–CoO NPs to induce IL-12, IFN-c,
and TNF-a at NP concentrations below those causing
appreciable cytotoxicity indicates immunomodulatory
effects that may function to bias the immune response
toward Th1-mediated immunity. It is the cytokine profile
that directs the development and differentiation of T helper
cells into the two different subsets, Th1 and Th2 [56].
Relevant to our findings, IL-12 and IFN-c play a critical role in
Th1 development, and help set up a perpetuating loop whereby
more Th1 development is favored. Our findings indicate that
careful titration of CL–PMIDA–CoO NP based therapeutic
interventions may be successful in elevating the levels of a
group of cytokines important for eliciting a Th1-mediated
immune response with effective anticancer actions.
Fig. 6 Internalization of rhodamine 123 tagged CL–PMIDA–CoO
NPs into macrophages by fluorescence imaging: a gray scale and
b fluorescence images
J Biol Inorg Chem (2013) 18:957–973 967
123
Incubation with POF
The production of TNF-a by mononuclear phagocytes is
regulated by the intracellular levels of cyclic adenosine
monophosphate (cAMP) [59]. Exogenous cAMP analogues
and substances such as prostaglandin E, which are capable of
increasing the intracellular level of cAMP, reduce the release
of bioactive TNF-a by downregulating the expression of the
TNF-a gene [59, 60]. Recent studies reported the ability of
theophylline and POF, both phosphodiesterase inhibitors, to
suppress monocyte/macrophage TNF-a production by
increasing the intracellular accumulation of cAMP [61, 62].
POF is a xanthine which has been used clinically for the
treatment of vascular diseases since 1984 [63–66]. There is
increasing evidence that POF may also play a therapeutic role
in the inhibition of inflammatory processes. POF has been
shown to improve resistance against sepsis or endotoxin
challenge in mice, rats, and humans [65, 67], most likely by
decreasing circulating TNF-a levels [29]. POF is able to
inhibit the synthesis of messenger RNA for TNF-a in mouse
Day 1 Day 3 Day 50
5
10
15
20
25
30
35
40
45
50
*
*
*
*
**
µM
/mg
prot
ein
NO release by macrophages / KB cell Co-culture
Control OVA treated CL-PMIDA-CoO treated
E: T- 5:1
Day 1 Day 3 Day 50
5
10
15
20
25
30
35
40
45
50
55
60
65
70
75
* *
*
*
*
**
*
*
**
*µM
/ m
g pr
otei
n
NO release by Macrophages
Control Macrophage 1µg protein-PMIDA-CoO 5µg protein-PMIDA-CoO 10µg protein-PMIDA-CoO 25µg protein-PMIDA-CoO
a
Day 1 Day 3 Day 50
5
10
15
20
25
30
35
40
45
50
55
60
65
70
75
*
*
**
*
µM
/mg
prot
ein
NO release by Macrophages / KB cell Co-culture
Control OVA Antigens CL-PMIDA-CoO NPs
E: T- 10:1
Day 1 Day 3 Day 50
5
10
15
20
25
30
35
40
45
50
55
60
65
70
*
*
*
**
µM
/mg
prot
ein
NO release by Macrophages / KB cell Co-culture
Control OVA Antigen CL-PMIDA-CoO treated
b
c d
Fig. 7 a Release of NO after co-culture of CL–PMIDA–CoO NP
exposed macrophages. NO release after co-culture of CL–PMIDA–
CoO NP pulsed macrophages with KB cells at ratios of macrophages
to KB cells of 5:1 (b) and 10:1 (c), and in the presence of
acetylsalicylic acid (ASA) and indomethacin at a ratio of 10:1 (d).
n = 6; values are expressed as the mean ± the standard error of the
mean. Asterisks indicate a significant difference as compared with the
control group
968 J Biol Inorg Chem (2013) 18:957–973
123
peritoneal macrophages at the transcriptional level [32]. Also
in humans, POF is able to reduce the release of TNF-a by
peripheral blood macrophages [30]. The present study showed
that use of POF in culture medium increased the cancer cell
viability by 98.15 % and 95.15 % on day 1, by 94.43 % and
82.61 % on day 3, and by 88.52 % and 81.03 % on day 5 after
co-culture with CL–PMIDA–CoO NP pulsed macrophages
(Fig. 10a). The viability was increased more in the presence of
POF than in the presence of ASA. Our findings for human
peripheral blood macrophages show that TNF-a is responsible
for CL–PMIDA–CoO NP mediated anticancer therapy.
Incubation with ASA
Cell viability significantly decreased in the presence of
ASA and indomethacin in medium (63.43 % on day 3 and
Day 1 Day 3 Day 50
20
40
60
80
100
120
% o
f cel
l via
blity
Macrophage / lymphocytes
Control Lympo. OVA pulsed Macrophages+Lympo.
TAA-NP pulsed Macrophages+Lympo. a
b
Fig. 8 a Viability of
lymphocytes after co-culture
with CL–PMIDA–CoO pulsed
macrophages in a 1:10 ratio.
b CD4? cell count was
measured by fluorescence-
activated cell sorting; negative
control (I), positive control (II),
CL–PMIDA–CoO treatment
(III)
J Biol Inorg Chem (2013) 18:957–973 969
123
46.03 % on day 5) in a ratio of 10:1 (Fig. 10b). By using
inhibitors of the COX pathway [33], we have been able to
show that NP pulsed macrophages exhibit lower cytotoxic
activity against cancer cells in vitro. We found that the
cytotoxicity was inhibited in the presence of ASA and
indomethacin.
We believe that we have successfully established a
model in which cytotoxicity toward oral cancer is
exhibited by activation of normal human macrophages
with the help of the CL–PMIDA–CoO complex. This
model allows basic studies of delivery of tumor lysate to
macrophages and activated-macrophage-mediated
immunostimulation against oral cancer cells. It has
already been reported that human macrophages lack the
cofactor tetrahydrobiopterin, which is necessary to pro-
duce NO [68]. It is seen that the presence of ASA in
medium increased NO production, which is responsible
for killing cells. Besides, there are other cytotoxic factors
which are responsible for macrophage-mediated killing of
oral cancer cells [69, 70]. To find the factors involved in
anticancer activity in our experiment, we used POF, a
potent TNF-a blocker. It was found that TNF-a was
responsible for killing KB cells as evident from the
increase in KB cell viability in the presence of POF in
a
IFN-gamma
0123456789
1011121314151617 *
* *
*
*
Pg
/ ml
Control OVA Control 1µg/ml NP 5µg/ml 10µg/ml 25µg/ml
TNF-alpha0123456789
10111213141516171819
*
*
*
*
*
Pg
/ ml
Control OVA Control 1µg/ml NP 5µg/ml 10µg/ml 25µg/ml
IL-120
5
10
15
20
25
30
35
40 *
*
*
*
Pg
/ ml
Control OVA Control 1µg/ml NP 5µg/ml 10µg/ml 25µg/ml
b
c
Fig. 9 Estimation of cytokine release from CL–PMIDA–CoO NP
pulsed macrophages at different doses. Release of interferon (IFN)-c(a), TNF-a (b), and IL-12 (c) was estimated by ELISA. n = 6; values
are expressed as the mean ± the standard error of the mean. Asterisks
indicate a significant difference as compared with the control group
970 J Biol Inorg Chem (2013) 18:957–973
123
medium (Fig. 9). Inhibition of COX-2 also increases KB
cell viability, but the viability is lower than that resulting
from blocking TNF-a. From this point of view, we say
that CL–PMIDA–CoO NPs stimulate TNF-a-mediated
anticancer immunotherapy, and a probable pathway is
presented in Scheme 1.
Conclusions
The results show that PMIDA–CoO NPs efficiently bind
with tumor cell lysate antigens and deliver antigens to
macrophages. The pulsed macrophages show good anti-
cancer activity. Such a metal nanocarrier system offers
E: T- 10:1
Day 1 Day 3 Day 50
20
40
60
80
100*
*
*
*
*
*
*
% o
f cel
l via
blity
Macrophage / KB cell
KB Cells Normal Macrophages+KB Cells
OVA pulsed Macrophages+KB Cells
CL-PMIDA-CoO pulsed Macrophages+KB Cells
Day 1 Day 3 Day 50
20
40
60
80
100
**
*
% o
f cel
l via
blity
Macrophage / KB cell (10:1)
KB Cells Normal Macrophages+KB Cells
OVA pulsed Macrophages+KB Cells
CL-PMIDA-CoO pulsed Macrophages+KB Cells a
E: T- 10:1
b
Fig. 10 Viability of cancer cells after co-culture with CL–PMIDA–
CoO NP pulsed macrophage in a 1:10 ratio in the presence of
a pentoxifylline (POF) and b ASA. n = 6; values are expressed as the
mean ± the standard error of the mean. Asterisks indicate a
significant difference as compared with the control group
Scheme 1 Proposed pathway.
COX-2 cyclooxygenase 2, iNOS
inducible nitric oxide synthase,
MØ macrophage, NFjB nuclear
factor jB
J Biol Inorg Chem (2013) 18:957–973 971
123
versatility in that it can simultaneously deliver an adjuvant
with the antigen to trigger macrophages. As the study was
an in vitro study, only the direct effects of cytotoxicity
toward cancer cells were observed. Therefore, in vivo
experiments are needed to observe the influences of other
coexisting factors.
Acknowledgments The authors express their gratefulness to the
Department of Biotechnology, Government of India, for funding. The
authors also express their gratefulness to the Indian Institute of
Technology, Kharagpur and Vidyasagar University, Midnapore, for
providing the facilities to execute these studies.
Conflict of interest The authors declare that there are no conflicts
of interest.
References
1. Cheng J, Teply BA, Jeong SY, Yim CH, Ho D, Sherifi I, Jon S,
Farokhzad OC, Khademhosseini A, Langer RS (2006) Pharm Res
23:557–564
2. Schreiber HA, Prechl J, Jiang H, Zozulya A, Fabry Z, Denes F,
Sandor M (2010) J Immunol Methods 356:47–59
3. Tseng P, Carlo DD, Judy JW (2009) Nano Lett 9:3053–3059
4. Gupta RK, Chang AC, Siber GR (1998) Dev Biol Stand 92:63–78
5. Bandyopadhyay A, Fine RL, Demento S, Bockenstedt LK, Fa-
hmy TM (2011) Biomaterials 32:3094–3105
6. Prasad S, Cody V, Saucier-Sawyer JK, Saltzman WM, Sasaki CT,
Edelson RL, Birchall MA, Hanlon DJ (2011) Nanomed Nano-
technol Biol Med 7:1–10
7. Villa CH, Dao T, Ahearn I, Fehrenbacher N, Casey E, Rey DA,
Korontsvit T, Zakhaleva V, Batt CA, Philips MR, Scheinberg DA
(2011) ACS Nano 5:5300–5311
8. Liong M, Lu J, Kovochich M, Xia T, Ruehm SG, Nel AE,
Tamanoi F, Zink JI (2008) ACS Nano 2:889–896
9. Connor EE, Mwamuka J, Gole A, Murphy CJ, Wyatt MD (2005)
Small 1:325–327
10. Ghosh P, Han G, De M, Kim CK, Rotello VM (2008) Adv Drug
Deliv Rev 60:1307–1315
11. Pissuwan D, Niidome T, Cortie MB (2009) J Control Release
149:65–71
12. Maus L, Dick O, Bading H, Spatz JP, Fiammengo R (2010) ACS
Nano 4:6617–6628
13. Wang K, Xu JJ, Chen HY (2005) Biosens Bioelectron
20:1388–1396
14. Liu X, Qiu G, Li X (2005) Nanotechnology 16:3035–3040
15. Parkes LM, Hodgson R, Lu LT, Tung LD, Robinson I, Fernig
DG, Thanh NT (2008) Contrast Media Mol Imaging 3:150–156
16. Papis E, Rossi F, Raspanti M, Isabella DD, Colombo G, Milzani
A, Bernardini G, Gornati R (2009) Toxicol Lett 189:253–259
17. Dailey JP, Phillips JP, Li C, Riffle JS (1999) J Magn Magn Mater
194:140–148
18. Rutnakornpituk M, Baranauskas V, Riffle JS, Connolly J, Pierre
TG, Dailey JP (2002) Eur Cells Mater 3:102–105
19. Pardoe H, Chua-anusorn W, Pierre TG, Dobson J (2001) J Magn
Magn Mater 225:41–46
20. Hubert PM, Guerrero G, Vioux A (2005) J Mater Chem
15:3761–3768
21. Adden N, Gamble LJ, Castner DG, Hoffmann A, Gross G,
Menzel H (2006) Langmuir 22:8197
22. Neouze MA, Schubert U (2008) Monatsh Chem 139:183–195
23. Chattopadhyay S, Chakraborty SP, Laha D, Baral R, Pramanik P,
Roy S (2012) Cancer Nano 3:13–23
24. Lowry OH, Rosebrough NJ, Farr AL, Randall RJ (1951) J Biol
Chem 193:265–275
25. Sahu SK, Chakrabarty A, Bhattacharya D, Ghosh SK, Pramanik P
(2011) J Nanopart Res 13:2475–2484
26. Ghosh T, Chattopadhyay T, Das S, Mondal S, Suresh E, Zangr-
ando E, Das D (2011) Cryst Growth Des 11:3198–3205
27. Hudson L, Hay FC (1991) Practical immunology, 3rd edn.
Blackwell, Melbourne, pp 21–22
28. Balasubramaniam P, Malathi A (1992) J Postgrad Med 38:8–9
29. Staudinger T, Presterl E, Graninger W, Locker GJ, Knapp S,
Laczika K, Klappacher G, Stoiser B, Wagner A, Tesinsky P,
Kordova H, Frass M (1996) Intensive Care Med 22:888–893
30. Hino M, Kohchi C, Nishizawa T, Yoshida A, Nakata K, Inagawa
H, Hori H, Makino K, Terada H, Soma GI (2005) Anticancer Res
25:3747–3754
31. Yongbin M, Chen B, Zhang Y, Hou Y, Xie H, Xia G, Tang M,
Huang X, Ni Y, Hu Q (2011) Int J Nanomed 6:1779–1786
32. Marques LJ, Zheng L, Poulakis N, Guzman J, Costabel U (1999)
Am J Respir Crit Care Med 159:508–511
33. Okada M, Sagawa T, Tominaga A, Kodama T, Hitsumoto Y
(1996) Immunology 89:158–164
34. Mohapatra S, Mallick SK, Maiti TK, Ghosh SK, Pramanik P
(2007) Nanotechnology 18:385102–385111
35. Cho WS, Dart K, Nowakowska DJ, Zheng X, Donaldson K,
Howie SE (2012) Nanomedicine 7:1495–1505
36. O’Hagan DT, Jeffery H, Davis SS (1994) Int J Pharm 103:37–45
37. Hans ML, Lowman AM (2002) Curr Opin Solid State Mater Sci
6:319–327
38. Audran R, Peter K, Dannull J, Men Y, Scandella E, Groettrup M
(2003) Vaccine 21:1250–1255
39. Wood BR, Quinn MQ, Tait B, Romeo M, Mantsch HH (1998)
Biospectroscopy 4:75–79
40. Banyay M, Sarkar M, Graslund A (2003) Biophys Chem
104:477–488
41. Anand KV, Chinnu MK, Kumar RM, Mohan R, Jayavel R (2010)
J Alloys Compd 496:665–668
42. Hermanson GT (1996) Bioconjugate techniques. Academic, New
York
43. Gojova A, Guo B, Kota RS, Rutledge JC, Kennedy IM, Barakat
AI (2007) Environ Health Perspect 155:403–409
44. Tagawa M, Yumoto R, Oda K, Nagai J, Takano M (2008) Drug
Metab Pharmacokinet 23:318
45. Wilson KT, Fu S, Ramanujam KS, Melzer SJ (1998) Cancer Res
58:2929–2934
46. Peters K, Unger RE, Gatti AM, Sabbioni E, Tsaryk R, Kirkpa-
trick C (2007) Int J Immunopathol Pharmacol 20:685–695
47. Lavnikova N, Drapier JC, Laskin DL (1993) J Leukoc Biol
54:322–328
48. Klimp AH, de Vries EG, Scherphof GL, Daemen T(2002) Crit
Rev Oncol Hematol 44:143–161.
49. Morgan DL, Shines CJ (2004) Toxicol In Vitro 18:139–146
50. Salvemini D, Misko TP, Masferrer JL, Seibert K, Currie MG,
Needleman P (1993) Proc Natl Acad Sci USA 90:7240–7244
51. Watkins DN, Garlepp MJ, Thompson PJ (1997) Br J Pharmacol
121:1482–1488
52. Kanematsu M, Keda K, Yamada Y (1997) J Bone Miner Res
12:1789–1796
53. Von Knethen A, Brune B (1997) FASEB J 11:887–895
54. Singer II, Kawka DW, Schloemann S, Terssner T, Riehl T,
Stenson WF (1998) Gastroenterology 115:297–306
55. Hanley C, Thurber A, Hanna C, Punnoose A, Zhang J, Wingett
DG (2009) Nanoscale Res Lett 4:1409–1420
56. Lappin MB, Campbell JD (2000) Blood Rev 14:228
972 J Biol Inorg Chem (2013) 18:957–973
123
57. Dong C, Flavell RA (2001) Curr Opin Hematol 8:47
58. Croft M (2009) Nat Rev Immunol 9:271
59. Katakami Y, Nakao Y, Oizumi TK, Katakami N, Ogawa R, Fujita
T (1988) Immunology 64:719–724
60. Kunkel SL, Spengler M, May MA, Spengler R, Larrick J, Remick
D (1988) J Biol Chem 263:5380–5384
61. Spatafora M, Chiappara G, Merendino AM, Amico DD, Bellia V,
Bonsignore G (1994) J Eur Respir 7:223–228
62. Endres S, Fulle HJ, Sincha B, Stoll D, Dinarello CA, Gerzer R,
Weber PC (1991) Immunology 72:56–60
63. Huh PW, Kotasek D, Jacob HS, Vercellotti GM, Hammerschmidt
DE (1985) Clin Res 33:866–878
64. Strieter RM, Remick DG, Ward PA, Spengler RN, Lynch JP,
Larrick J, Kunkel SL (1988) Biochem Biophys Res Commun
155:1230–1236
65. Schade UF (1990) Circ Shock 31:171–181
66. Schade UF (1989) Eicosanoids 2:183–187
67. Coccia MT, Waxman K, Soliman MH, Tominaga G, Pinderski L
(1989) Crit Care Med 17:36
68. Weinberg JB, Misukonis MA, Shami PJ, Mason SN, Sauls DL,
Dittman WA, Wood ER, Smith GK, McDonald B, Bachus KE
(1995) Blood 86:1184–1195
69. Komada Y, Sakurai M (1997) Leuk Lymphoma 25:9–21
70. Williams MA, Newland AC, Kelsey SM (2000) Leuk Res
24:317–330
J Biol Inorg Chem (2013) 18:957–973 973
123