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Nanotoxicology, 2015; 9(S1): 118–132
! 2015 Informa UK Ltd. DOI: 10.3109/17435390.2014.991431
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Towards an alternative testing strategy for nanomaterials used in
nanomedicine: Lessons from NanoTEST
M. Dusinska1, S. Boland2, M. Saunders3, L. Juillerat-Jeanneret4, L. Tran5, G. Pojana6,7, A. Marcomini7, K. Volkovova8,
J. Tulinska8, L. E. Knudsen9, L. Gombau10, M. Whelan11, A. R. Collins12, F. Marano2, C. Housiadas13, D. Bilanicova6,7,
B. Halamoda Kenzaoui4,11, S. Correia Carreira14, Z. Magdolenova1, L. M. Fjellsbø1, A. Huk1, R. Handy15, L. Walker16,
M. Barancokova8, A. Bartonova1, E. Burello11,17, J. Castell10, H. Cowie5, M. Drlickova8,18, R. Guadagnini2, G. Harris11,
M. Harju1, E. S. Heimstad1, M. Hurbankova8, A. Kazimirova8, Z. Kovacikova8, M. Kuricova8, A. Liskova8, A. Milcamps11,
E. Neubauerova8, T. Palosaari11, P. Papazafiri19, M. Pilou14, M. S. Poulsen9, B. Ross5, E. Runden-Pran1, K. Sebekova20,
M. Staruchova8, D. Vallotto6,7, and A. Worth11
1
Health Effects Laboratory-MILK, NILU – Norwegian Institute for Air Research, Kjeller, Norway, 2Unit of Functional and Adaptive Biology (BFA),
Laboratory of Molecular and Cellular Responses to Xenobiotics (RMCX)), Univ Paris Diderot, Sorbonne Paris Cité, UMR 8251 CNRS, Paris, France,
3
Department of Medical Physics & Bioengineering, BIRCH, Bioengineering, Innovation & Research Hub, St. Michael’s Hospital, University Hospitals
Bristol NHS Foundation Trust, Bristol, United Kingdom, 4University Institute of Pathology, Lausanne, Switzerland, 5Institute of Occupational
Medicine, Riccarton, Edinburgh, UK, 6DFBC – Department of Philosophy and Cultural Heritage, University Ca’ Foscari Venice, Venice, Italy, 7DAIS –
Department of Environmental Sciences, Informatics and statistics, University Ca’ Foscari Venice, Venice, Italy, 8Faculty of Medicine, Slovak Medical
University, Bratislava, Slovakia, 9Faculty of Health and Medicinal Sciences, Institute of Public Health, University of Copenhagen, Copenhagen,
Denmark, 10Leitat Technological Center, Scientific Park, Barcelona, Spain, 11Institute for Health and Consumer Protection, European Commission
Joint Research Centre, Ispra (VA), Italy, 12Department of Nutrition, University of Oslo, Oslo, Norway, 13Thermal Hydraulics and Multiphase Flows
Laboratory, Institute of Nuclear & Radiological Sciences & Technology, Energy & Safety, NCSR ‘‘Demokritos’’, Agia Paraskevi, Greece, 14Bristol Centre
for Functional Nanomaterials, University of Bristol, Bristol, UK, 15School of Biomedical and Biological Sciences, Plymouth University, Plymouth, UK,
16
Bristol Heart Institute, School of Clinical Sciences, University of Bristol, Bristol, UK, 17Computational Chemistry Group, RAPID Department
(Risk Analysis of Products in Development), TNO, Zeist, The Netherlands, 18Centre for Chemical Substances and Preparations, Bratislava, Slovakia,
19
Department of Biology, University of Athens, University Campus, Athens, Greece, and 20Medical Faculty, Institute of Molecular Biomedicine,
Comenius University, Bratislava, Slovakia
Abstract
Keywords
In spite of recent advances in describing the health outcomes of exposure to nanoparticles
(NPs), it still remains unclear how exactly NPs interact with their cellular targets. Size, surface,
mass, geometry, and composition may all play a beneficial role as well as causing toxicity.
Concerns of scientists, politicians and the public about potential health hazards associated with
NPs need to be answered. With the variety of exposure routes available, there is potential for
NPs to reach every organ in the body but we know little about the impact this might have. The
main objective of the FP7 NanoTEST project (www.nanotest-fp7.eu) was a better understanding
of mechanisms of interactions of NPs employed in nanomedicine with cells, tissues and organs
and to address critical issues relating to toxicity testing especially with respect to alternatives to
tests on animals. Here we describe an approach towards alternative testing strategies for
hazard and risk assessment of nanomaterials, highlighting the adaptation of standard methods
demanded by the special physicochemical features of nanomaterials and bioavailability studies.
The work has assessed a broad range of toxicity tests, cell models and NP types and
concentrations taking into account the inherent impact of NP properties and the effects of
changes in experimental conditions using well-characterized NPs. The results of the studies
have been used to generate recommendations for a suitable and robust testing strategy which
can be applied to new medical NPs as they are developed.
Hazard assessment, in vitro, nanoparticles,
NanoTEST, testing strategy
History
Received 14 August 2014
Revised 2 November 2014
Accepted 19 November 2014
Published online 29 April 2015
Abbreviations: AFM: atomic force microscopy; BBB: blood–brain barrier; BET: Brunauer–
Emmett–Teller; BSA: bovine serum albumin; CBMN: cytokinesis-block micronucleus; CS: calf
serum; CNS: central nervous system; DCFH-DA: 2,7-dichlorodihydro-fluorescein diacetate; DLS:
dynamic light scattering; DNA: deoxyribonucleic acid; ELISA: enzyme-linked immunosorbent
assay; EDX/EDS: energy-dispersive X-ray spectroscopy; FBS: fetal bovine serum; Fl-25 SiO2:
fluorescent 25 nm silica; GM-CSF: granulocyte macrophage colony-stimulating factor; H2AX:
H2A histone family member X; HE: hydroethidine; HTS: high-throughput screening; IL:
Correspondence: Dr Maria Dusinska, Health Effects Laboratory, Norwegian Institute for Air Research (NILU), Instituttveien 18, 2007 Kjeller, Norway.
Tel: +4763898157. E-mail: maria.dusinska@nilu.no
An alternative testing strategy for nanomaterials
DOI: 10.3109/17435390.2014.991431
119
interleukin; LDH: lactate dehydrogenase; LTT: lymphocyte transformation test; mBBr:
monobromobimane; MTT: 3-(4,5-dimethyl-thiazol-2-yl)-2,5-diphenyl-tetrazolium bromide;
NaFlu: sodium fluorescein; NP: nanoparticle; NTA: nanoparticle tracking analysis; OC-Fe3O4:
Na-oleate-coated iron oxide; PBMC: peripheral blood mononuclear cells; PBPK: physiologically
based pharmacokinetic; PI: propidium iodide; PLGA-PEO: polylactic-co-glycolic acid-Poly poly
ethylene oxide; (Q)SAR: quantitative structure–activity relationship; ROS: reactive oxygen
species; RTqPCR: quantitative real time RT-PCR; SANS: small angle neutron scattering; SB: strand
breaks; SD: stock dispersion; SEM: scanning electron microscopy; SLS: static light scattering;
SOPs: standard operating procedures; SP-ICP-MS: single particle inductively coupled plasmamass spectrometry; TEM: transmission electron microscopy; U-Fe3O4: uncoated iron oxide;
WST1: 2-(4 -iodophenyl)-3-(4-nitrophenyl)-5-(2,4-disulphophenyl)-2H-tetrazolium;
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Introduction
The rapid and enormous development of nanotechnology has been
accompanied by a deep concern about the effects that nanoparticles (NPs) may have on human health and the environment.
However, the knowledge gaps in our understanding of the
behaviour of NPs, their transformation and fate in different
environments including biological systems, make it difficult to
evaluate their toxic effects and to perform adequate hazard and
risk assessment. Selection of the best endpoints and methods in
appropriate cell models and adaptation, standardization and
validation of methods are still needed.
NPs can potentially enter the human body through a range of
exposure routes (Elsaesser & Howard 2012; Hagens et al., 2007)
including intravenous injection, inhalation and ingestion via the
digestive tract. They can then translocate to the blood from where
they can reach most organs and possibly accumulate, before being
eliminated through processes that are not yet clearly understood
(Oberdörster et al., 2005).
In the respiratory tract, NPs interact with bronchial and
alveolar epithelial cells, inducing cell activation and reaction.
Very small NPs may translocate through the lung epithelium and
the endothelium of the blood vessels into the blood and lymph
circulation. Similar mechanical properties as in the respiratory
tract can be expected in the digestive tract cells in which NPs can
induce cell activation and tissue reaction, oxidative stress and loss
of the barrier functions of the epithelium. In the blood, NPs can
interact with circulating cells, inducing cell activation, increased
adhesion of the NPs to each other or endothelial cells. Interaction
with cells of the vascular wall can induce vascular reaction,
activation and vascular leakage, and uptake of NPs by endothelial
cells and perivascular cells. The liver is the major site for
biotransformation and defence against foreign materials and
xenobiotics, and this is very likely also true for NPs, possibly
inducing hepatocyte and/or sinusoidal endothelial and Kupffer
cell activation. The kidney transports and excretes NPs from the
blood to the urine, or reabsorbs them from urine. The central
nervous system (CNS) is separated from the blood by the blood–
brain barrier (BBB), represented by a very specialized vascular
system consisting of endothelial cells, pericytes and astrocytes,
but limiting access to the brain. NPs may induce the activation of
brain endothelial, astroglial and microglial cells. The placenta is a
biological barrier of particular interest in relation to the sensitive
nature of the foetus and NPs may induce placental inflammation
associated with foetal defects. Representative cells and cell lines
originating from these organs were used to test NPs selected in the
NanoTEST project (Tables 1 and 2) and to select the best in vitro
models to determine modes of action for hazard assessment
(Juillerat-Jeanneret et al., 2015).
A strategy for in vitro toxicity testing in a regulatory context
requires a battery of tests addressing different mechanisms and
covering all main important toxicity endpoints. Thus, to identify
relevant short-term hazard models, we used several standard
toxicity assays for different markers such as cell viability, proinflammatory response, oxidative stress, genotoxicity, immunotoxicity, cell uptake and transport. OECD recommended methods
were chosen where possible, such as in the case of genotoxicity
(Magdolenova et al., 2012a,b) and when necessary methods were
adapted for NP testing (Guadagnini et al., 2015a) and fully
documented in relevant publications or NanoTEST protocols
(www.nanotest-fp7.eu). The specific focus of our biomarker
validation strategy was to identify the most suitable conditions for
detecting a significant response and, by including relevant
positive and negative controls, to ensure that the method is
reliable and gives reproducible results.
Table 1. Selected nanoparticles (NPs).
Name
Abbreviation
Nanomagnetite coated with
Na-oleate
Nanomagnetite uncoated
Polylactic-co-glycolic acid
Red-Fluorescent 25 nm
silica
Red-Fluorescent 50 nm
silica
Nanosilica powder, 20 nm
OC-Fe3O4
PlasmaChem (Hamburg, D)
U-Fe3O4
PLGA-PEO
Fl-25 SiO2
PlasmaChem (Hamburg, D)
Advancell (Barcelona, E)
Microspheres-nanospheres
Fl-50 SiO2
Microspheres-nanospheres
SiO2
Nano-sized titanium dioxide AeroxideP25; anatase/rutile powder of
21 nm (nominal size)
Dextran-coated ferumoxide
TiO2
NM-203 Reference Material, Joint Research Centre,
(Ispra, Italy)
NM-105, P25-Degussa-Evonik (Essen, Germany),
obtained from Joint Research Centre (Ispra, Italy)
Endorem
Source
Guerbet (Paris, F)
Comment
Reference NPs, positive control
Negative control, in clinics
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120
M. Dusinska et al.
Nanotoxicology, 2015; 9(S1): 118–132
To verify the suitability of in vitro models, in vivo studies
were carried out. A single i.v. administration of TiO2 or
Na-oleate-coated iron oxide (OC-Fe3O4) NPs (0.1, 1 and 10%
of LD50) to young female rats did not elicit overt acute or
subacute toxicity (Sebekova et al., 2014; Volkovova et al., 2015)
but seemed to have an immunomodulatory effect. The in vitro
model of human peripheral blood cells generally reflected in vivo
responses of peripheral blood immune cells to TiO2 and OCFe3O4 NPs in exposed rats and proved the reliability of our panel
of immune assays proposed as biomarkers for assessment of
immunotoxicity in vitro (Tulinska et al. in preparation). There was
also a good correlation in genotoxicity tests between in vitro/
in vivo micronucleus tests and the comet assay for both TiO2 and
OC-Fe3O4 NPs (Kazimirova et al., in preparation). In addition, in
silico methods were considered and a new model for predicting
the oxidative stress potential of oxide NPs was proposed (Burello
& Worth, 2011, 2015). The in vitro and in silico methods
developed for NPs used in nanomedicine can also be utilised for
the assessment of health effects of NPs used and applied in other
areas and thus can have a wider impact on all 3 R’s (replacement,
reduction and refinement of animals) for toxicity testing.
The overall aim of NanoTEST was to provide testing strategies
for hazard identification and risk assessment of NPs, and to
propose recommendations for evaluating potential risks associated with new medical NPs. The specific objective was to
develop a set of master standard operating procedures (SOPs) for
at least two assays for each type of toxicity (including cell
viability, pro-inflammatory response, oxidative stress, genotoxicity, immunotoxicity, cell uptake and transport). The most
advanced and standardised techniques would be adapted for
automation and prepared for validation.
The project addressed the factors responsible for variability in
the results of nanotoxicity studies – namely, the source and type of
NP, method of preparation or synthesis, stabilizers used, dispersion method, state of agglomeration, presence of impurities;
as well as variations in experimental conditions such as pH,
temperature and sonication. The treatment regime is critical;
results can depend on cell type used, exposure time, dose, the
assay method used, and possible interference with the detection
system (Dusinska et al., 2011, 2012, 2013; Guadagnini et al.,
2015a, 2015b) as discussed below. The overall goal of the current
paper is to summarise the artefacts and issues identified in
nanotoxicology, into a coherent set of tables and guidelines for
use by the research community in the design of testing strategies
and to suggest modifications of assays where appropriate.
Characterization of NPs
A recommended list of physico-chemical properties to be
characterized when testing specific manufactured nanomaterials
for human health and environmental safety, has been proposed by
the OECD (Report no. 36ENV/JM/MONO(2012)40, 2012). It
includes particle size distribution (in solid and in liquid media),
shape, agglomeration/aggregation, water solubility/dispersability,
as well as parameters occasionally measured such as octanol–
water partition coefficient (where relevant), redox potential and
radical formation potential. It is now clear that discrepancies
between reported toxicity results are caused not only partly by
different intrinsic properties, both physical (size, shape, etc.) and
chemical (crystal structure, surface chemistry, etc.) of nominally
similar, or identical, NPs, but also by the application of different
testing conditions of NPs in physiological media, which could
affect transport kinetics in the investigated fluids (Kato et al.,
2009; Magdolenova et al., 2012a). Clearly, a testing strategy for
nanomaterials needs to include a comprehensive characterization
(Bouwmeester et al., 2011), including in particular a determination of the main physical and chemical properties of NPs, and the
properties pertaining to NP behaviour in biological media used for
evaluating toxicological effects. The most frequently employed
techniques are scanning and transmission electron microscopy
(SEM and TEM, respectively), Brunauer–Emmett–Teller (BET),
dynamic or static light scattering (DLS and SLS, respectively),
NP tracking analysis (NTA) and small angle neutron scattering
(SANS; Hassellöv & Kaegi, 2009). No single technique could
adequately characterize a selected NP (Warheit, 2008); only a
proper combination of various techniques is able to describe the
Table 2. Cell models selected for use in toxicity studies.
Organ/tissue
Blood
Endothelial
cells
Cell model
Abbreviation
References
Human lymphocyte cell line
TK6
Magdolenova et al. (2012a, 2015)
Human blood cells (lymphocytes)
Rat brain-derived endothelial cells
EC219
Tulinska et al. (2015)
Juillerat-Jeanneret et al. (1992)
Murine lung-derived endothelial cells
Human brain-derived endothelial cells
Rat hepatocytes
Rat liver macrophages (Kupffer cells)
Human lung-derived alveolar cells
Human lung-derived bronchial cells
ECp23
HCEC
Placenta
Placental choriocarcinoma cells
BeWo b30
Central nervous system
Rat brain-derived endothelial cells
Human brain-derived endothelial cells
Human glioblastoma (astroglioma)
cells
Distal tubule epithelial cells
Proximal tubule epithelial cells
Monkey kidney cells
EC219
HCEC
LN229
Juillerat-Jeanneret et al. (1992)
Halamoda Kenzaoui et al. (2012b)
Aranda et al. (2013)
Aranda et al. (2013)
Guadagnini et al. (2015a)
Guadagnini et al. (2015b);
Hussain et al. (2010)
Saunders (2009), Correia Carreira
et al., (2015), Poulsen et al. (2015);
Cartwright et al. (2011)
Juillerat-Jeanneret et al. (1992)
Halamoda Kenzaoui et al. (2012b,c)
Halamoda Kenzaoui et al. (2013a)
MDCK
LLC-PK
COS 1
Halamoda Kenzaoui et al. (2013b)
Halamoda Kenzaoui et al. (2013b)
Magdolenova et al. (2012a,b)
Human kidney cells
HEK 291
Magdolenova et al. (in preparation)
Liver
Lung
Kidney
A549
16HBE140
Source
ATCC CRL-8015
ECACC (cat. no.
95111735)
Primary cells
Primary culture
Primary culture
ATCC CCL-185
ATCC CRL-2611
ATCC CCL-34
ATCC CL-101
ATCC CRL-1573
ECACC 88031701
An alternative testing strategy for nanomaterials
DOI: 10.3109/17435390.2014.991431
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Table 3. Average hydrodynamic diameters of TiO2 NPs dispersed in stock dispersion SD-TB and SD-TC then added to investigated biological media
(TiO2 NPs concentration in media: 0.3 mg/ml) and measured by dynamic light scattering (DLS) after 30 min and 48 h.
Biological medium
Hydrodynamic
diameter (nm) after
30 min for
SD-TB
Hydrodynamic
diameter (nm) after
30 min for
SD-TC
DMEM
DMEM + 10% FBSa
DMEM-HG
DMEM-HG + 10% FBSa
RPMI-1640
RPMI-1640 + 10% FBSa
DMEM-F12-HAMc
DMEM-F12-HAMc + 10% FBSa
Large agglomeratesb
752 ± 397
Large agglomeratesb
642 ± 283
Large agglomeratesb
779 ± 382
2130 ± 1160
756 ± 422
85 ± 14/246 ± 54
112 ± 20/296 ± 55
100 ± 15/266 ± 50
80 ± 18/276 ± 73
92 ± 18/270 ± 69
102 ± 15/285 ± 67
92 ± 18/270 ± 69
84 ± 13/245 ± 55
Hydrodynamic
diameter (nm)
after 48 h
for SD-TB
Large
Large
Large
Large
Large
Large
Large
Large
agglomeratesb
agglomeratesb
agglomeratesb
agglomeratesb
agglomeratesb
agglomeratesb
agglomeratesb
agglomeratesb
Hydrodynamic
diameter (nm)
after 48 h for SD-TC
109 ± 22/363 ± 64
125 ± 27/366 ± 65
108 ± 21/318 ± 69
94 ± 17/283 ± 69
114 ± 22/371 ± 82
116 ± 14/352 ± 49
110 ± 13/286 ± 45
123 ± 20/360 ± 63
TiO2 NPs, an anatase/rutile powder of 21 nm (nominal size), NM-105. Sub-samples of NM-105 were packed under Good Laboratory Practice
conditions and preserved under argon in the dark until use.
TiO2 NPs dispersion protocol SD-TB. Stock solutions of TiO2 NPs were made by weighing 20 mg of TiO2 NPs and suspending in 10 ml of culture
medium containing 15 mM Hepes buffer without FBS in a 15 ml plastic tube. The suspensions were sonicated using an ultrasonic probe sonicator
(Labsonic, Sartorius) for 3 min at 60 W (on ice and water mixture to allow the cooling down of the solution). Within 2 min after sonication and
directly after 10 sec of vortexing, the solution was divided into 10 microcentrifuge tubes and stored at 20 C for further use. Immediately before use
TiO2 NPs were thawed, vortexed for 10 s before being immediately sonicated for 1 min (on ice and water mixture) at 60 W, and added to cell culture
medium to achieve a 0.3 mg/ml working solution.
TiO2 NPs dispersion protocol SD-TC. Stock solutions at 5 mg/ml of TiO2 NPs were prepared fresh each time. To prepare 1 ml of stock solution, 1 ml of
20% foetal bovine serum (FBS) in PBS was added to 5 mg of TiO2 NPs in a microcentrifuge tube. The dispersion was sonicated with a UP200S probe
sonicator by Hielscher Ultrasonic Technology (Teltow, Germany) for 15 min at 100 Watt (cycle: 100%). The dispersion was cooled during sonication
with an ice/water bath in order to prevent heating of the dispersion. The resulting stock suspension was added to cell culture medium to achieve a
0.3 mg/ml working suspension.
All media were purchased from Sigma-Aldrich RPMI – 1640 cat.no. R8758; DMEM cat.no.D6046; DMEM-HG cat.no. D5796; DMEM-F12-HAM
cat.no. D6421
a
For ethical reasons, only one type of FBS was used: Sigma-Aldrich cat.no.F9665.
b
Formation of very large agglomerates not detectable by DLS technique, unstable dispersion.
c
DMEM-F12-HAM was supplements with 1% Amphotericin B (cat. no. A2942) + 1% L-Glutamine–Penicillin–Streptomycin solution (cat. no. G6784).
NP properties driving the observed toxicological behaviour. There
is no consensus yet on the strategy to identify an optimal set of
techniques and procedures, mainly because of the rapidly
increasing variety of available NPs and the limited comparative
evaluations carried out so far on the advantages and constraints of
each analytical method and technique applied to date in toxicological testing (Stone et al., 2010; Zuin et al., 2007).
Preparation of NP dispersions for treatment of cells
An accurate characterization of NPs additionally to primary
characteristics at different stages of testing (i.e. as supplied,
before/after administration, during the course of experiments) is
essential to find a meaningful correlation between NP structural
properties and toxicity (Jiang et al., 2009; Oberdörster et al.,
2005; Powers et al., 2007). Properties of nanomaterials change
depending on the surrounding environment. NPs tend to precipitate, agglomerate and aggregate, which can affect their toxic
potential and the tendency for agglomeration/aggregation has
already been proposed as a key property for the interpretation of
(eco)toxicological results (Kato et al., 2009). The stability of the
dispersion depends on the effect of various forces (electrostatic
and steric hindrance, Van der Waals forces, magnetic attraction
force), which are determined mainly by the properties of the
particle and the dispersing medium (as mentioned above) and
particle surface properties, i.e. surface chemistry (OECD Report
no. 36ENV/JM/MONO(2012)40, 2012). Most proposed protocols
so far are simply derived from protocols previously developed for
standard chemicals, and rarely cope with the intrinsic instability
of NPs in biological media (Handy et al., 2012). Differences in
handling procedures and dispersion protocols for NPs have
recently been demonstrated to strongly affect the overall toxicological behaviour of NPs (Magdolenova et al., 2012a).
A satisfactory stability of dispersion in culture medium is,
however, sometimes extremely difficult to achieve because of the
intrinsic properties of some NPs and the selected experimental
conditions (Handy et al., 2012; Ramirez-Garcia et al., 2011).
Within NanoTEST, primary and secondary characteristics of NPs
were published by Guadagnini et al. (2015a). Properties of NPs
and their toxic effects can also be influenced by the different
physical and chemical properties of solvents used for dispersing or
dissolving them. Factors such as pH, salinity, water hardness,
temperature and the presence of dissolved or natural organic
particles can influence the biological reactivity of NPs. Thus, they
might behave differently in water, culture medium, PBS and other
solvents (Handy et al., 2012), with pronounced effects on their
uptake, cellular localization and hence the observed toxic
response. For in vitro toxicity testing, it is essential to characterize
NPs in the treatment medium immediately before and if possible
also after treatment. Particle size, state of agglomeration, surface
properties and stability of the dispersion stock solution as well as
of the NPs dispersed in the final treatment medium should be
measured. However, methods to follow the transformation and
fate of NPs are not yet fully developed. It is recommended to
measure particle size distribution using at least two methods
[OECD Report no. 36ENV/JM/MONO(2012)40, 2012]. In
NanoTEST, a wide range of techniques were employed including
SEM, TEM, atomic force microscopy (AFM) and DLS. The
experience from NanoTEST showed that the NP dispersion should
always be freshly prepared, i.e. immediately before the experiment, as the stability of NP suspensions is in most cases limited
(Table 3). Most common dispersion protocols include bovine
serum albumin (BSA) or fetal bovine or calf serum (FBS or CS),
as the presence of proteins prevents agglomeration. The data on
stabilities of TiO2 NPs in various culture media showed that the
preparation of stock dispersion and use of serum proteins in stock
dispersion as well as in final medium have impact on NP size and
dispersion stability. While a stock dispersion prepared without
122
M. Dusinska et al.
serum resulted in large agglomerates, preparation with FBS gave a
more stable (up to 48 h) bimodal dispersion with two peaks more
or less in the nanosized range (Table 3). However, the protein
corona that forms around NPs affects their toxicological properties (Lundqvist et al., 2011; Mahon et al., 2012; Magdolenova
et al., 2012a; Mortensen et al., 2013; Yang et al., 2013).
Sonication of the dispersion also protects against agglomeration
and is widely used. However, severe sonication can affect the
properties of nanomaterials (Taurozzi et al., 2011).
It is also important to note that the in vitro treatment medium
should mimic real in vivo conditions as closely as possible, e.g.
addition of serum proteins is conceivable for endothelial or blood
cells but not for respiratory cell cultures for which surfactant
components could be used to achieve good dispersions; composition and proportion of proteins and other components should be
similar to those present in the organism.
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Expression of concentrations (metrics)
The concentration of NPs is commonly expressed in mass units –
[mg/ml], [mg/cm2] or [mg/cell]. The relationship between the mass
units can vary depending on the type of culture plates, amount of
medium and number of cells used. In addition, concentrations can
be expressed as number of NPs per ml, per cm2 or per cell as well
as surface area of NPs per ml, per cm2 or per cell. In the
NanoTEST project, we recommended that concentrations be
expressed in at least two different units, not only as mass but also
as number of NPs or as surface area, since surface properties and
size are among those physicochemical properties of NPs that may
impact on toxicity and thus these units might be more informative
for the comparative evaluation of toxicity of different NPs.
Primary particle size and agglomerate size of the suspensions
should thus be measured which will also allow calculation of the
number concentration if this is not determined experimentally
(calculation using nominal values should be avoided). The
surface area should also be determined experimentally when
possible as porosity and roughness will influence the actual
surface area of the particles. The expression of concentration per
cell seems most appropriate for NP testing and should be
considered in in vitro toxicity testing. In the NanoTEST experiments, concentrations were expressed in mg/ml and in mg/cm2 and
aspects of experimental set up such as the plate surface area,
number of cells, volume of medium used, for all toxicity tests
were the same whenever possible. In the future, concentration per
cell could or should be verified using emerging methods such as
single particle inductively coupled plasma-mass spectrometry
analysis (SP-ICP-MS) or imaging with energy-dispersive X-ray
spectroscopy (EDX/EDS) subject to particle composition
(Laborda et al., 2013).
Concentrations used should be realistic, i.e. relevant to
possible human exposures. For some assays, notably the comet
assay, recommended concentrations should range from non-toxic
to around 80% cell viability, since breakage of deoxyribonucleic
acid (DNA) can be a secondary effect of cytotoxicity and so the
use of cytotoxic concentrations could give false positive results. In
some tests (micronucleus assay), the toxicity range is normally
from non-toxic to around 50% viability.
NPs have a tendency to agglomerate and therefore the
concentration of NPs should not exceed the level at which
agglomeration is enhanced. The stability of the dispersion
decreases with increasing concentration. When agglomeration
occurs, it is difficult to quantify exposure as it varies and is most
likely reduced either due to changes in concentration mass,
reduced particle count or surface area. Agglomeration of NPs
affects their bioavailability to the cell and thus might lead to false
positive/negative results. High concentrations can also give rise to
Nanotoxicology, 2015; 9(S1): 118–132
overload effects that can be misinterpreted as evidence of
cytotoxicity (Wittmaack, 2011).
Exposure conditions: time of treatment and
concentration range
The exposure time is crucial. For testing ordinary chemicals
in vitro, 3–6 h and 24 h exposures are usually recommended. NPs
may need more time to enter the cells. NP uptake in cells with
macrocytic activity is usually shorter than in most of the other cell
types. Liver macrophages (Kupffer cells) but not hepatocytes
were able to internalize silica NPs after 4 h (Aranda et al., 2013).
For NP toxicity studies in NanoTEST, both shorter (1–3 h) as
well as longer (at least 24–72 h) treatments were used depending
on the endpoint studied; a longer treatment was preferred to
ensure uptake by cells.
For certain tests, such as the micronucleus assay, 24 h
treatment is necessary to cover at least 1–1.5 cell cycles, as
some compounds including NPs might be active only at a specific
cell cycle stage and also access to nuclear DNA will be facilitated
by the absence of nuclear membrane during mitosis. The
concentration range of nanomaterials should ensure adequate
exposure that reflects possible exposure scenarios and the
concentrations used need to be scientifically justified.
Positive and negative controls and reference standards
Positive and negative controls are integral parts of the testing
procedure that are always included in experiments, for the
purpose of quality control, to demonstrate correct performance of
the assay and to ensure reproducibility. Negative controls consist
of dispersion solutions without NPs but otherwise processed
identically to NP dispersions (e.g. same sonication schedule, etc.).
A positive control (an agent inducing toxicity appropriate to the
particular assay and cell type) is included in each experiment to
check that the assay is performing correctly and giving the
expected positive response. In the case of metal NPs, metal ions
should be used as an additional control, since metal ions released
from NPs can cause production of reactive oxygen species (ROS)
via Fenton-like reactions and so it is important to test whether the
presence of these ions, rather than the NPs, is inducing toxicity.
Coating materials or NP stabilizers can also cause toxicity and
thus should also be tested and included in the experimental set-up
as additional reference material (control). NPs are good carriers,
and if a stabilizer or coating is toxic, low, normally non-toxic
concentrations can cause damage due to their enhanced internalization into cells. Within NanoTEST, OC-Fe3O4 NPs were
tested and Na-oleate was included in the genotoxicity testing as
well as other tests of cell stress (Magdolenova et al., 2015; Schütz
et al., 2014). These additional controls to discriminate between
coating/solvent/stabiliser effects and effects of NPs are of utmost
importance.
A challenge for nanotoxicity studies is the choice of nanospecific positive/negative controls. In the NanoTEST project,
dextran-coated iron oxide EndoremÕ was used as negative control
(Cowie et al., 2015). There are several initiatives currently
focusing on selection of nanomaterials with appropriate properties
to be recommended as reference standards (Stone et al., 2010;
reviewed by Stefaniak et al., 2013). ZnO NPs were suggested as a
positive control for the comet assay in the EU NanoGenotox
project report (http://www.nanogenotox.eu/files/PDF/nanogenotox_web.pdf); however, results were not reproducible, being
particularly affected by the type of cell used. Certified nanospecific reference standards for use as positive controls are
urgently needed. The NanoTEST project also suggested several
positive controls for each toxicity endpoint as discussed below.
Reproducibility is crucial for any test method but especially for
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An alternative testing strategy for nanomaterials
123
NPs with so many factors that may contribute to variability
between and within tests. Thus, building historical positive and
negative controls (average values from all experiments performed
in the laboratory with particular cell model and test over period of
several years) as used in regulatory toxicology is good practice for
quality assurance and evaluation of safety of nanomaterials.
and by the physical properties of the membranes used to develop
two-chamber models as TranswellÕ inserts. Permeable membranes are available from a number of manufacturers and can
differ widely in terms of composition, coating and pore size, all of
which have the potential to introduce artefacts in cell seeding and
NP interactions (Ragnaill et al., 2011; Saunders, 2009).
Bioavailability of nanomaterial: uptake, subcellular
localization and NP release
Selection of cell models and assays
For evaluation of toxicity generally, knowledge of bioavailability
of the tested compound is essential. In the case of NPs, uptake
studies are needed to show whether NPs are able to reach and
enter the cells. The internalization of NPs is highly sizedependent; however, uptake might not follow commonly defined
size limits, and kinetics of uptake for the same type of NPs varies
in the different cell types (dos Santos et al., 2011). NP transport is
most affected by tightness of the cell barrier, with transport
increasing in the order: brain5placenta5kidney after 2 h and
brain5kidney5placenta after 24 h exposure as shown from
transport studies of OC-Fe3O4 NPs utilising different cell types
(Figure 1; Correia Carreira et al., 2015; Halamoda Kenzaoui
et al., 2012a, 2013b). The different order in extent of transport
with time is likely to be due to changes in cell growth in each
model and will reflect differences in the tightness of the barrier
formed.
Uptake and subcellular localization of NanoTEST NPs
were extensively studied in different cell types (Correia Carreira
et al., 2015; Halamoda Kenzaoui et al., 2012a,b,c, 2013a,b;
Magdolenova et al., 2015; Poulsen et al., 2015). If toxicity testing
gives negative results, toxic effects cannot be excluded unless
uptake of NPs has been demonstrated. On the other hand, a
demonstration of non-uptake does not necessarily imply nontoxicity, since NPs may act indirectly via oxidative stress (Hussain
et al., 2010) or inflammation, in which case they do not need to be
internalized.
Studies of transport and release of NPs are limited to labelled
NPs and NPs that can be detected at low concentration in buffers
and to NPs which do not agglomerate under such cell culture
conditions. They are also limited due to lack of analytical methods
Figure 1. Cell line and exposure-dependent transport of OC-Fe3O4 NPs
across cell barriers. The appearance of OC-Fe3O4 NPs in the basal
chamber was determined over the course of 2 h (open bars) and 24 h
(filled bars). The initial applied amount of iron of 50 mg was added to the
apical chamber (100 mg/mL) and results are expressed as the percentage
of the iron added to the apical chamber as detected in the basal chamber,
quantified using the Prussian blue reaction and normalised to the amount
transported across the Transwell insert (3 mm Costar polyester membrane)
in the absence of cells.
Appropriate cellular model systems were selected in the
NanoTEST project, representing different target organs and
retaining organ-specific functions including cell activation and
metabolic modification.
Criteria for selection of the best cell models (either primary
cells or cell lines) include (a) their commercial availability, (b)
their growth in culture media with minimal addition of growth
factors which could be absorbed by the NPs, (c) expression of
organ specific functions and (d) their stability under culture
conditions. The initial selection and evaluation of cells (under
NanoTEST) resulted in the adoption of a range of cell models as
laid out in Table 2.
NP-induced toxicity may primarily result from direct interaction of particles with cells and cell organelles such as
mitochondria, or DNA, or indirectly through the enhanced
production of ROS by cellular constituents in response to their
interaction with the particles (Magdolenova et al., 2014). Both
pathways may depend on surface properties, the presence of
transition metals, intracellular iron mobilization and lipid
peroxidation processes. ROS can also be the cause of the
secondary toxicity, via the inflammatory response of host cells.
Oxidative stress has often been described as a key mechanism
underlying the ability of NPs to cause cellular injury including
DNA damage (Karlsson, 2010).
The broad range of toxicity assays tested under NanoTEST,
including cytotoxicity, oxidative stress, inflammatory stress,
immunotoxicity, genotoxicity, uptake and transport assays, are
described in more detail in (Aranda et al., 2013; Correia Carreira
et al., 2015; Guadagnini et al., 2015a, 2015b; Halamoda Kenzaoui
et al., 2012a,b,c, 2013a,b; Harris et al., 2015; Kazimirova et al.,
2012; Magdolenova et al., 2012a,b, 2015; Poulsen et al., 2015;
Tulinska et al., 2015). SOPs for each selected model and assay,
detailed culture conditions, exposure to the NPs and experimental
protocols are described in a database, available from the project
website (www.nanotest-fp7.eu).
We have evaluated statistically the results of experiments
comparing cells representing different organs. Cytotoxic effects
induced by NPs depend on the test used, exposure conditions
and the cell type (Aranda et al., 2013; Correia Carreira et al.,
2015; Guadagnini et al., 2015; Halamoda Kenzaoui et al.,
2012a,c, 2013a,b; Harris et al., 2015; Kazimirova et al., 2012;
Magdolenova et al., 2012a, 2015; Poulsen et al., 2015; Tulinska
et al., 2015). The data also suggest that while there are
differences between the cell lines, the strongest effect is from
the NPs as seen with the OC-Fe3O4 NPs results (Figure 2). For
genotoxicity screening of NPs, the various cell types used give
consistent results but with different sensitivity, allowing the
study of target organ specificity and cell type sensitivity
(Cowie et al., 2015).
Technical limitations of the assays: possible interference
of nanomaterial with the test
Properties of NPs such as adsorption capacity, optical properties,
hydrophobicity, chemical composition, surface charge and surface
properties, catalytic activities as well as agglomeration can result
in interference with standard toxicity tests (Aranda et al., 2013;
Guadagnini et al., 2015a; Kroll et al., 2012). The interference of
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124
M. Dusinska et al.
NPs with specific assays was observed for metallic oxide solid
core NPs and was demonstrated with a range of in vitro cell
viability assays [MTT (3-(4,5-dimethyl-thiazol-2-yl)-2,5-diphenyl-tetrazolium bromide], LDH (lactate dehydrogenase), WST-1
(2-(4-iodophenyl)-3-(4-nitrophenyl)-5-(2,4-disulphophenyl)-2Htetrazolium), Annexin V/PI (propidium iodide), neutral red,
caspase activation, propidium iodide, 3H-thymidine incorporation, automated cell counting], inflammatory responses (ELISA
for granulocyte macrophage colony-stimulating factor (GM-CSF),
interleukin (IL)-6 and IL-8] and oxidative stress detection
[monoBromoBimane (mBBr), dichlorodihydro-fluoresceindiacetate (DCFH-DA), NO assays; Guadagnini et al., 2015a; Kroll
et al., 2012]. Interferences found were assay as well as NPspecific. Thus, the evaluation of possible interference is required
to ensure reliable results. This is mainly relevant for cytotoxicity
assays, oxidative stress responses of cells and the production by
the cells of bio-molecules such as peptides, proteins or others
(Guadagnini et al., 2015a). It is clear that for nanotoxicity testing
most of the assays need to be adapted and modified to avoid
measuring artefacts. Aranda et al. (2013) showed that despite the
quenching effect of NPs on DCFH-DA assay, it can be considered
as a useful tool for quantitative measurement of NPs-induced
oxidative stress by minor modifications of the standardized
protocol. Additional standards need to be included as controls for
the interference. For genotoxicity, interference was reported so far
with the micronucleus test (Gonzalez et al., 2011; Magdolenova
et al., 2012b) and the comet assay (Karlsson, 2010; Stone et al.,
2009). The protocol for the micronucleus assay needed modification as cytochalasin B (used in this assay) inhibits endocytosis
and may prevent uptake of NPs (Gonzalez et al., 2011;
Magdolenova et al., 2012b). Using the comet assay, with 6 NPs,
we found no interference. (Magdolenova et al., 2012b). However,
to prevent false-negative/false-positive results, we recommend
testing for possible interference of NPs in the gel, using both
untreated cells and cells exposed to a known genotoxic compound
(causing DNA strand breaks as well as oxidized DNA lesions).
This would be a sensible precaution to be sure that no
overestimation or underestimation of damage is occurring.
Testing strategy
We investigated whether tests used in the NanoTEST are reliable,
give reproducible results and are suitable for NP testing.
In addition, we set out to validate a battery of tests covering all
Nanotoxicology, 2015; 9(S1): 118–132
important toxic endpoints (Table 4). Methodological consideration of these tests has been addressed in Guadagnini et al.
(2015a) for cytotoxicity, oxidative stress and inflammatory
markers and for genotoxicity in Magdolenova et al. (2012b).
As mentioned above, one of the main obstacles for assessing
the toxicity of nanomaterials is the lack of knowledge of how
physicochemical properties relate to the interaction of NPs with
biological systems and the mechanism of toxicity. It is clear that
physical and chemical properties can influence NP behaviour and
may have an impact on toxicity; they must therefore be an integral
part of toxicity testing. This is one of the key aspects of toxicity
screening strategies (Dusinska & NanoTEST Consortium, 2009;
Dusinska et al., 2011, 2012, 2013). Both primary and secondary
characterizations of tested NPs are crucial, including in situ
characterization during exposure. The physico-chemical properties that should be considered for assessing toxic effects of
nanomaterials include as a minimum chemical composition,
particle size, shape, surface properties, size distribution, agglomeration state and crystal structure. Regarding the likelihood of
biomolecular corona formation, it is also important to set up
experimental conditions that can mimic exposure in humans. As
NPs change their properties depending on the surrounding milieu,
we recommend at least two different exposure conditions for
testing the NP’s effects (Magdolenova et al., 2012a).
An important question is whether the commonly used assays
for chemicals could be applied to NPs. Our results show that it is
not always possible to use these assays without careful adaptation
because of possible interference (Guadagnini et al., 2015a),
especially between NPs, the dye and the optical detection or with
the assay components during the experiment (Tables 4–6). It is
therefore of crucial importance to test possible interference of all
studied NPs with the foreseen methods prior to evaluating cellular
responses to NPs. To avoid these interferences, special adaptations of standard toxicity tests are also proposed [refer Tables 4
and 5, and Guadagnini et al. (2015a) for more detailed description]. Furthermore, all the assays do not have the same sensitivity
and it is important to choose the most sensitive appropriate assay.
From our results, for the oxidative stress markers, the thiol
depletion and induction of antioxidant enzymes seem to be more
sensitive than the measure of ROS (Guadagnini et al., 2015b).
Our proposal for further evaluation of testing strategies is to
perform first a battery of assays for validation of the effects of
a representative set of well-characterized NPs on the target
cells; then if appropriate and available, to screen larger banks of
Figure 2. Cell viability of EC219, HCEC, LN229 or N11 cells exposed to (A) Si-25 or (B) OC-Fe3O4 NPs for 72 h as measured by the MTT assay.
Values represent average % of untreated control ± SD of three separate experiments for each exposure.
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Assay (SOP)
Cytotoxicity
WST1 (measured in
supernatants)
Endpoint
High throughput
Automation
Costeffective
Userfriendly
Specific equipment
needed
Yes
Possible
Yes
Yes
Multiwell plate reader
(absorbance)
Yes
Possible
Yes
Yes
Multiwell plate reader
(absorbance)
Medium-throughput
Difficult
Yes
No
Flow cytometer
Agglomerated NPs can
interfere with automatic
cell counting
Agglomerated NPs can
interfere with automatic
cell counting
Agglomerated NPs can
interfere with automatic
cell counting
NPs could increase or
decrease OD measurements and NPs could
adsorb MTT
Medium-throughput
if automatic cell
counter
Medium-throughput
if automatic cell
counter
Medium-throughput
if automatic cell
counter
Yes
Possible
Yes
Yes
Possible
Yes
Yes
Possible
Yes
Yes
Possible but often
interference with
NPs
Yes
Yes
No; Light microscope;
automatic counter
(optional)
No; light microscope;
automatic counter
(optional)
No; light microscope;
automatic counter
(optional)
Multiwell plate reader
(absorbance)
Yes (test adsorption of
cytokines on NPs)
NPs could adsorb secreted
cytokines
Yes
No
Yes
Multiwell plate reader
(absorbance)
Pro-inflammatory
response
Yes (use guanidinium thiocyanate–phenol–chloroform RNA extraction
protocol)
NPs could adsorb RNA
(compare recovery
methods and choose
extraction method that
recovers all RNA)
No
Possible but often
interference with
NPs
Difficult
No
No
Real time PCR
instrument
Oxidative stress
Yes (verify interference)
Yes
Possible
Yes
Yes
Oxidative stress
Yes (verify interference)
NPs could increase or
decrease fluorescence
NPs could increase or
decrease fluorescence
Yes
Possible
Yes
Yes
Multiwell plate reader
(fluorescence)
Multiwell plate reader
(fluorescence)
Oxidative stress
Yes (verify interference)
NPs could increase or
decrease fluorescence
Yes
Possible
Yes
Yes
Multiwell plate reader
(fluorescence)
Oxidative stress
Yes (adapt gating to
exclude free NPs from
analysis and to account
NPs could increase or
decrease fluorescence
and NP agglomerates
Medium-throughput
Difficult
Yes
No
Flow cytometer
PI uptake by flow
cytometry
Cytotoxicity
Plating efficiency
Cytotoxicity
Relative growth activity
Cytotoxicity
Trypan blue exclusion
Cytotoxicity
MTT
Cytotoxicity
Pro-inflammatory response
ELISA
Pro-inflammatory
response
125
(continued )
An alternative testing strategy for nanomaterials
NPs could increase or
decrease OD measurements (use supernatants)
NPs could increase or
decrease OD measurements and LDH may be
absorbed by some NPs
NPs could increase or
decrease fluorescence
(adapt gating)
Cytotoxicity
Oxidative stress
ROS detection by DHE
using plate readers
ROS detection by carboxy-fluorescein
using plate readers
Thiols detection by bromobimane using
plate readers
ROS detection by HE
using flow cytometry
Interference/technical problems with NPs
Yes (measurement on supternatants; spin/filter out
NPs)
Yes (ensure colorimetric
controls are included and
test adsorption of LDH
on NPs)
Yes (gating to exclude free
NPs from analysis and to
account for changes in
fluorescence by NPs)
Yes/No (only when automatic method for counting cells is used)
Yes/No (only when automatic method for counting cells is used)
Yes/No (only when automatic method for counting cells is used)
Yes (verify interference)
Cytotoxicity
Lactate dehydrogenase
(LDH)
RTqPCR
Modifications in assay for
NPs versus standard
chemicals
DOI: 10.3109/17435390.2014.991431
Table 4. Implementation of standard in vitro toxicity assays for nanomaterial testing.
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126
Table 4. Continued
Endpoint
Interference/technical problems with NPs
could be counted as cells
or debris
NPs could adsorb RNA
(compare recovery
methods and choose
extraction method that
recovers all RNA)
Uptake
Not used for chemicals
Cell fluorescence quantified by flow
cytometry
Uptake
Yes (adapt gating to
exclude free NPs from
analysis)
Transmission electron
microscopy (TEM)
Uptake
No
Single and double
strand breaks
No
Comet assay with repair
enzyme
Genotoxicity: base
DNA damage
No
Cytokinesis-block
micronucleus assay
Transport
Barrier permeability
(NaFlu)
Barrier transport of NP
in Transwells
Genotoxicity/
mutagenicity
Yes (cytochalasin B 24 h
after NPs)
Barrier integrity
Yes (rinse barrier with PBS
prior to assessment)
Yes (porous membrane
needs to be optimised for
RTqPCR
Uptake
Side scatter of laser
light in flow
cytometry
Genotoxicity
Comet assay
Oxidative stress
Transport of NPs across
barrier
Automation
Costeffective
Userfriendly
Specific equipment
needed
No
Difficult
No
No
Real time PCR
instrument
Can only be used for NPs
which scatter light;
gating needed to exclude
free NPs and dead cells;
imaging flow cytometry
needed to distinguish
NPs bound on cell
surface
Can only be used for NPs
which are fluorescent;
gating needed to exclude
free NPs; use of
quenchers or imaging
flow cytometry needed
to distinguish NPs bound
on cell surface
Verification required that
objects seen are actually
NPs e.g. by EDS/EDX
Medium-throughput
Difficult
Yes
No
Flow cytometer/imaging
flow cytometer
Medium-throughput
Difficult
Yes
No
Flow cytometer/imaging
flow cytometer
No
No
Yes
No
Electron microscope
Ensure NPs in gel do not
interfere by using both
untreated cells and cells
exposed to known genotoxic compound
Normally NPs do not come
in contact with enzyme:
However, additional
control, cells with oxidized lesions and NPs in
gel, can be included.
Cytochalasin B can inhibit
NP uptake
Yes
Possible
Yes
Yes
Fluorescence microscope, image analysis
Yes
Possible
Yes
Yes
Fluorescence microscope, image analysis
Yes
Possible
Yes
Yes
Light microscope,
image analysis
Potential interference of
NPs with fluorescence
NP may adhere to Transwell
membrane and retention
of NPs by porous
Possible
No
Yes
Yes
Plate reader; Transwells
Possible
No
Yes
Yes
Plate reader; Transwells
Nanotoxicology, 2015; 9(S1): 118–132
for changes in fluorescence by NPs)
Yes (use guanidinium thiocyanate–phenol–chloroform RNA extraction
protocol)
High throughput
M. Dusinska et al.
Assay (SOP)
Modifications in assay for
NPs versus standard
chemicals
An alternative testing strategy for nanomaterials
Liquid scintillation
counter
Yes
No
Difficult
Possible
NPs could interfere with
counts per minutes
measurements
Flow cytometer
No
No
Difficult
Medium-throughput
Potential interference of
NPs with fluorescence
Difficult
Medium-throughput
Potential interference of
NPs with fluorescence
Immunotoxicity
Immunotoxicity
Natural killer cell activity by flow cytometry
Proliferative response of
lymphocytes by 3H
thymidine
incorporation
Yes (adapt gating to
exclude free NPs from
analysis and to account
for changes in fluorescence by NPs)
Yes (adapt gating to
exclude free NPs from
analysis and to account
for changes in fluorescence by NPs)
Yes (verify interference)
Immunotoxicity
Immunotoxicity
Phagocytic activity and
respiratory burst of
leukocytes by flow
cytometry
membrane will reduce
transport:assess NP
interaction with membrane filter and NP
transport. NP detection
methods need to be
refined
particle type and cell
type)
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Yes
No
Flow cytometer
DOI: 10.3109/17435390.2014.991431
127
NPs using automated procedures on a predefined set of representative cells. Appropriate statistical analyses must always be
implemented.
For the evaluation of the different cell models, depending on
route of exposure and use of NPs there should be several organ
models used for testing. Blood is an important model both as a
direct target as well as surrogate target tissue and gives an
indication of toxicity. Peripheral blood lymphocytes are suitable
cells but unfortunately not always accessible; the TK6 (lymphoblastic) cell line is an alternative. We additionally propose that
commercially available human cell lines for each representative
organ be included in the testing strategy, e.g. for lung cells
available cell lines (A549 cells is one alternative), CaCo2 cells
(colon), LN229 cells (glioblastoma) and HEK293 or MDCK
(human or porcine kidney, respectively).
For short-term hazard assessment, the testing strategy should
include all important toxicity endpoints such as cytotoxicity,
oxidative stress, genotoxicity or immunotoxicity to investigate the
mode of action of NPs in biological systems. In vitro experiments
with cells representing different organ targets revealed that
oxidative stress and toxic effects induced by NPs depend on the
NPs’ properties, the test used and the cell type. Polylactic-coglycolic acid (PLGA-PEO) NPs induced little or no oxidative
stress in any cell type compared with solid-core metallic NPs
which generally produced ROS (Guadagnini et al., 2015b;
Halamoda Kenzaoui et al., 2012c, 2013b). Genotoxicity induced
by NPs depends on the NPs, the dispersion protocol and the
measured endpoint (Magdolenova et al., 2012a). All cells tested
were able to detect the positive response but with different
sensitivity showing tissue specific effects (Cowie et al., 2015).
In the initial stages of testing, cytotoxicity assays should be
used to identify non-cytotoxic concentrations of the NPs for more
specific in vitro studies. Moreover, inclusion of nanospecific
positive and negative controls is strongly recommended.
The strategy proposed for a battery of in vitro tests is explained
as follows.
(1) To determine possible cytotoxicity and induction of oxidative
stress.
– For cytotoxicity studies, basal cellular toxicity tests such as
relative growth activity and plating efficiency and the MTT
and WST-1 assays and a time course of 24 and 72 h, using
OC-Fe3O4 NPs as positive control NPs and PLGA-PEO NPs
as negative control NPs.
– For oxidative stress, the thiol depletion measured by
monobromobimane assay (and possibly DCFH-DA; Aranda
et al., 2013) and the induction of antioxidant enzyme mRNA
expression measured by RT-qPCR (Guadagini et al., 2015b),
4 and 24 h time-course, using uncoated iron oxide (U-Fe3O4)
NPs and TiO2 NPs as positive control NPs and PLGA-PEO
NPs as negative control NPs.
(2) to determine the uptake and possible release, following
uptake, of the NPs by relevant cells of the different organs, at
non-cytotoxic concentrations of the NPs.
– For uptake, TEM and depending on NP properties flow
cytometry (if light scattering or fluorescent) or analytical
methods (ICP-MS). Analytical chemistry on cell supernatants could be used to study the release of NPs (dos Santos
et al. 2011; Elsaesser et al, 2011).
– For uptake and release studies, 24 h uptake followed by 24 h
release, using U-Fe3O4 NPs as positive control NPs
(Halamoda Kenzaoui et al., 2012b, 2013b).
– For transport studies, 24 h time-course, using OC-Fe3O4
NPs as positive control NPs, limiting these experiments to
NPs which do not agglomerate in the culture conditions
(Correia Carreira et al., 2015; Halamoda Kenzaoui et al,
2013b).
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128
Table 5. Nanomaterial properties which could be problematic for specific test methods.
Cytotoxicity
PI uptake by flow cytometry
Agglomeration
Adsorption of dyes
OK
OK
OK
Need filtration
before analysis
OK
OK
Quantification of cell-associated fluorescent NMs by
flow cytometry
Need filtration
before analysis
OK
OK
Quantification of cell associated iron containing NMs
by plate reader
Quantification of cell-associated fluorescent NMs by
plate reader
OK
OK
OK
OK
OK
OK
OK
OK
OK
OK
Plating efficiency
Relative growth activity
Uptake
Quantification of cell-associated light scattering NMs
by flow cytometry
Transmission electron microscopy (TEM)
Pro-inflammatory response
ELISA
RTqPCR
Oxydative stress measurements
by fluorescent dyes (DCFHDA, HE, mBBr etc) using
plate reader
OK if adjust gating
Problem
Problem
OK
Absorption/scattering of light
Affinity to labware
material
Stability/solubility
of particles
OK if adjust gating
OK
OK
Problem
OK
OK
OK
OK
OK
OK
OK
OK
OK
Problem (dependents on wavelength as PI
staining needed)
Need fluorescent
NMs (problem if
bleaching or
quenching of
fluorescence)
Problem (depends
on wavelength)
Need NMs which
scatter light
OK
Problem
Problem (adjust
gating)
OK
Problem
Problem
Problem
OK
Problem
Problem
Problem
OK
Need fluorescent
NMs (problem if
bleaching or
quenching of
fluorescence)
OK
OK
OK
Problem
Problem
Problem if adsorbe
RNA (adapt
extraction
technique)
OK
OK
OK
OK
OK
OK
OK
OK
OK
OK
Need filtration
before analysis
OK
OK if adjust gating
Problem (depending
on wavelength)
OK if adjust gating
OK
OK
OK
Problem if adsorbe
RNA (adapt
extraction
technique)
OK
OK
OK
OK
OK
OK
Problem
Problem (depending
on wavelengh)
Problem
Problem if interference with
detection
OK
OK
Nanotoxicology, 2015; 9(S1): 118–132
Oxidative stress
Oxidative stress measurements
by fluorescent dyes
(DCFH-DA, HE, mBBr etc)
using flow cytometry
RTqPCR
Problem if automatic
counting
Problem if automatic
counting
OK
Fluorescence
Problem (depends
on wavelength)
Problem (depends
on wavelength)
OK
LDH
Need filtration
before analysis
OK
Adsorption of
proteins
M. Dusinska et al.
Assay
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OK
OK
OK
OK
OK
OK
OK
OK
OK
OK
OK
OK
OK
Problem as proteins
may affect uptake
OK
OK
OK
OK
OK
OK
OK
Problem
Problem (depending
on wavelengh)
OK
OK
OK
Problem (may not
pass through
Transwell pores)
OK
OK
OK (need of detectable NPs)
OK
Problem (NP may
adhere to
Transwell
membrane)
Problem (depending
on detection
method)
Need filtration
before analysis
OK
OK if adjust gating
Problem (depends
on wavelength)
OK if adjust gating
OK
OK
Need filtration
before analysis
OK
OK
OK if adjust gating
OK if adjust gating
OK
OK
OK
Problem if quenching of
scintillation
Problem (depends
on wavelength)
Problem if quenching of
scintillation
Problem if quenching of
scintillation
OK
OK
DCFH-DA: 2,7-dichlorodihydro-fluorescein diacetate; ELISA: Enzyme-Linked ImmunoSorbent Assay; HE: Hydroethidine; LDH: lactate dehydrogenase; mBBr: Monobromobimane; MTT: 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyl-tetrazolium bromide; NaFlu: sodium fluorescein; OD: optical density; PI: propidium iodide; ROS: reactive oxygen species; RTqPCR: quantitative real time RT-PCR; TEM: transmission
electron microscopy; WST1: 2-(4-iodophenyl)-3-(4-nitrophenyl)-5-(2,4-disulphophenyl)-2H-tetrazolium.
An alternative testing strategy for nanomaterials
Immunotoxicity
Phagocytic activity and
respiratory burst of leukocytes by flow cytometry
Natural killer cell activity by
flow cytometry
Proliferative response of
lymphocytes by 3H thymidine incorporation
OK
OK
DOI: 10.3109/17435390.2014.991431
Gentoxicity
Comet assay: strand breaks
Comet assay: enzyme-sensitive
sites
Cytokinesis-block micronucleus assay
Transport
Permeability of cell barriers
using transwell culture
models (NaFlu dye)
Transport of NMs through cell
barriers using Transwell
culture models
129
130
M. Dusinska et al.
Nanotoxicology, 2015; 9(S1): 118–132
Table 6. General problems which may arise from specific nanomaterial properties and should be taken into consideration to choose the best testing
strategy and for correct interpretation of results.
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Agglomeration
Adsorption of
proteins
Problem for flow
cytometry
Change size
Change settling
Change uptake
Pipetting (problem
for correct dosing
and
reproducibility)
Change uptake
Change intracellular transport
Change intracellular
transport
Change
translocation
Change
translocation
Change in
metabolism
Biomarker
interference
Adsorption of
dyes/assay
reagents
Interference with
test methods
Fluorescence
Interference with
read-out system
Change of surface
characteristics if
not core-labelled
Problem of detection
if leaching or
bleaching
Problem if interference with dyes
(3) to determine possible genotoxic effect (Magdolenova et al.,
2012b,2014).
– For DNA damage, cells exposed for 24 h to NPs, using the
comet assay for DNA strand breaks (SB) and oxidized DNA
lesions (TiO2 or OC-Fe3O4 as positive control NPs and
PLGA-PEO NPs as negative control NPs, at non-cytotoxic
concentrations of NPs).
– For mutagenicity and clastogenicity, cytokinesis-block
micronucleus (CBMN) modified protocol for NPs genotoxicity testing. However, positive and negative controls should
be further specified.
– The gH2AX (H2A histone family, member X) assay is an
interesting end-point for automated procedures, but little
information so far exists about predicting NP-induced
genotoxicity using this test.
– Gene mutation assays (in either tk or hprt locus) have not
only been tested within NanoTEST, but should also be
implemented into genotoxicity strategy to cover all genotoxicity endpoints.
(4) To determine immunosafety of NPs, human peripheral whole
blood or isolated peripheral blood mononuclear cells
(PBMC) as representatives of human blood cell model are
proposed for in vitro screening of the immunotoxic potential
of nanoproducts. The main strength is the complexity of the
model containing several cell types and components in a
relatively intact environment. Testing strategy for assessment
of immunotoxic effect of NPs should contain a panel of
immune assays to cover several aspects of the immune
response. Cellular immune response: phagocytic activity and
respiratory burst of leukocytes, natural killer cell activity,
proliferative activity of lymphocytes in vitro stimulated with
mitogens and/or antigens (LTT). Humoral immune response:
production/expression of cytokines.
– For lymphocyte transformation test (LTT), fluorescent 25 nm
silica (Fl-25 SiO2) NPs as immunosuppressive control and
TiO2 NPs as possible candidate for immunostimulatory
control.
– For phagocytic activity and respiratory burst assay, U-Fe3O4
as stimulatory control and OC-Fe3O4 as suppressive nanocontrol.
– For natural killer cell activity, OC-Fe3O4NPs as suppressive
control and Fl-25 SiO2NPs as stimulatory control.
–
Absorption/scattering of light
Affinity to labware material
Stability/solubility
of particles
Interference with
read-out
system
Interference with
read-out
system and
test methods
Change
bioavailability
Problem for dosage/
detection
Problem for
dosage
Change size
Change uptake
Change intracellular
transport
For cytokine gene expression, OC-Fe3O4NPs as suppressive
control for IL-6.
(5) Finally, to perform the more selective evaluations, as
required by the particular characteristics of the organrepresentative cells, such as cytokine production, cellular
localization of NPs inside cells using techniques such as
confocal or electronic microscopy techniques, etc.
Tables 5 and 6 are intended to help choosing the best testing
strategy (toxicity test/dispersion media/adaptation of standard
methods) depending on the physico-chemical characteristics of
the NPs.
Several assays appeared to be suitable for high throughput
screening and automation (Table 4) and their implementation in
a testing strategy is desirable for a large number of NPs.
Increased throughput of the comet assay for detection of SBs
and specific DNA lesions is suggested for robust testing
together with automation and high throughput of assays for
cytotoxicity (measuring cell count, nuclear intensity and nuclear
size) and alternatively also for genotoxicity (gH2AX assay;
Harris et al., 2015). It is recommended to use a multiparametric analysis (high content imaging – HCI) which
provides more information and can allow determination of the
cause of the cytotoxic effect. High-throughput screening (HTS)
assays provide several benefits, including an upscaling of
number of NPs to be tested; for optimization and precision of
the assays; as a support to validations; and if applicable also
for industrial use.
The quantitative structure–activity relationship [(Q)SAR]
models promise to be valuable tools for future testing strategies.
The theoretical model predicting oxidative stress potential led to
the prioritisation of metal oxide NPs for further evaluation. The
proposed model could be used to guide the development of more
rational and efficient screening strategies; in addition, it can
create a more coherent conceptual framework when additional
toxicity related physicochemical properties (e.g. agglomeration
and solubility in water) are included (Burelo & Worth, 2011,
2015).
With proper refinement of computational models and methodologies, physiologically based pharmacokinetic (PBPK) modelling may serve as an alternative testing strategy in future (Pilou
et al., 2015), replacing experiments that are expensive both in
time and resources.
DOI: 10.3109/17435390.2014.991431
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Conclusions and remarks
A strategy for short-term hazard assessment and toxicity testing in
a regulatory context requires a battery of tests addressing different
mechanisms and covering all main important toxicity endpoints
including oxidative stress, genotoxicity, inflammation and
immunotoxicity. Toxicity tests should be performed in an
appropriate treatment medium and uptake should be an integral
part of the testing. Treatment should be long enough for the NPs
to enter the cells and entry and uptake should be confirmed and
quantified where possible (Elsaesser et al., 2011).
Appropriate controls and reference standards should be
included in tests. The solvent and, if NPs are coated, the coating
material need to be tested separately. Historical control data (for
each cell type used) are valuable references for quality control.
Toxicity tests must be accompanied by extensive characterization
of NPs, including in test-media (before and after exposure), and
covering primary and secondary properties of NPs. Number of
cells, cell culture plate format and volume of treatment medium
on the plate are important factors in expressing concentration and
can impact on the effect of NPs, and so they should be constant
within the study, especially when different NPs are compared.
Concentration range and exposure time are also crucial aspects in
toxicity testing and care must be taken to express concentrations
in at least two different units, not only in mass but also in number
of NPs or in surface area as this might be more representative for
evaluation of toxicity of different NPs than using mass units.
Determination of actual size and surface area is important as
number or surface concentrations are sometimes based on the
nominal particle size and may not reflect the actual particle size/
surface.
We propose that for full assessment of NP toxicity, at least 2–3
cytotoxicity tests (the MTT, WST-1 and plating efficiency assays
or relative growth activity), a set of at least 2–3 representative
cells and five NP concentrations should be used. Initially, the
cytotoxicity response to the NPs must be determined, then
oxidative stress response using at least two assays. A testing
strategy for assessment of immunotoxic effects of NPs should
contain assays covering several aspects of the immune response
(inducible proliferative response, phagocytic activity and respiratory burst of leukocytes, natural killer cell activity, production/
expression of cytokines). For genotoxicity, the modified comet
assay for DNA damage (strand breaks as well as oxidised DNA
lesions) should be included in the testing strategy together with
the micronucleus assay and a gene mutation test with the option of
the gH2AX assay in automated procedures. The evaluation of
internalization of NPs by cells should be an integral part of testing
strategy but is not always feasible, and the analytical methods and
the devices designed to evaluate NPs transport across cell layers
need improvements in technology.
Declaration of interest
The authors declare that there is no conflict of interests. The work
was supported by EC FP7 NanoTEST [Health-2007-1.3-4], Contract
no: 201335, EC FP7 QualityNano [INFRA-2010-1.131], Contract no:
214547-2, EC FP7 NANoREG, [NMP.2012.1.3-3], Contract no: 310584,
EC FP7 NanoTOES [PITN-GA-2010-264506] and by NILU internal
projects 106179. The work by UH Bristol was carried out with the support
of the Bristol Centre for Nanoscience and Quantum Information,
University of Bristol.
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