- Research article
- Open Access
Equine dendritic cells generated with horse serum have enhanced functionality in comparison to dendritic cells generated with fetal bovine serum
© The Author(s). 2016
Received: 9 January 2016
Accepted: 7 November 2016
Published: 15 November 2016
Dendritic cells are professional antigen-presenting cells that play an essential role in the initiation and modulation of T cell responses. They have been studied widely for their potential clinical applications, but for clinical use to be successful, alternatives to xenogeneic substances like fetal bovine serum (FBS) in cell culture need to be found. Protocols for the generation of dendritic cells ex vivo from monocytes are well established for several species, including horses. Currently, the gold standard protocol for generating dendritic cells from monocytes across various species relies upon a combination of GM-CSF and IL-4 added to cell culture medium which is supplemented with FBS. The aim of this study was to substitute FBS with heterologous horse serum. For this purpose, equine monocyte-derived dendritic cells (eqMoDC) were generated in the presence of horse serum or FBS and analysed for the effect on morphology, phenotype and immunological properties. Changes in the expression of phenotypic markers (CD14, CD86, CD206) were assessed during dendritic cell maturation by flow cytometry. To obtain a more complete picture of the eqMoDC differentiation and assess possible differences between FBS- and horse serum-driven cultures, a transcriptomic microarray analysis was performed. Lastly, immature eqMoDC were primed with a primary antigen (ovalbumin) or a recall antigen (tetanus toxoid) and, after maturation, were co-cultured with freshly isolated autologous CD5+ T lymphocytes to assess their T cell stimulatory capacity.
The microarray analysis demonstrated that eqMoDC generated with horse serum were indistinguishable from those generated with FBS. However, eqMoDC incubated with horse serum-supplemented medium exhibited a more characteristic dendritic cell morphology during differentiation from monocytes. A significant increase in cell viability was also observed in eqMoDC cultured with horse serum. Furthermore, eqMoDC generated in the presence of horse serum were found to be superior in their functional T lymphocyte priming capacity and to elicit significantly less non-specific proliferation.
EqMoDC generated with horse serum-supplemented medium showed improved morphological characteristics, higher cell viability and exhibited a more robust performance in the functional T cell assays. Therefore, horse serum was found to be superior to FBS for generating equine monocyte-derived dendritic cells.
Dendritic cells are antigen-presenting cells specialized in uptake and presentation of antigens to T cells . They are the only antigen-presenting cells capable of inducing primary immune responses in naïve T cells and are thus pivotal for the development of T cell responses [2, 3]. The function of dendritic cells is reflected in a number of specific properties. Their distinct shape with many cellular processes offers a large surface area for antigen recognition and uptake . Furthermore, the high surface expression of MHC class II in connection with high levels of costimulatory molecules allows for optimal stimulation of T cells. Initially, studies using dendritic cells have been hindered by difficulties in obtaining sufficient numbers of these cells, as their frequency is very low (<1%). The discovery that granulocyte-macrophage colony stimulating factor (GM-CSF) was the key cytokine needed to differentiate viable dendritic cells from murine blood  allowed the development of standardized methods to generate large numbers of dendritic cells ex vivo from hematopoietic progenitors. In humans, dendritic cells can be generated from peripheral blood CD14+ monocytes by using GM-CSF and Interleukin-4 (IL-4) [6, 7]. Due to the higher frequency of CD14+ cells, this method has been widely used to generate dendritic cells for experimental purposes in the human field and for immunotherapy. Monocyte-derived dendritic cells (MoDC) were shown to be homogeneous and could be fully matured using autologous monocyte-conditioned medium [8, 9] or, alternatively, through a cocktail of inflammatory cytokines, namely IL-1β, Tumor necrosis factor-α (TNF-α), IL-6 and Prostaglandin E2 (PGE2) . The generation of MoDC has been described in a number of domestic animal species such as cattle , pigs , sheep  and horses [14–17].
Fetal bovine serum (FBS) represents an important source of nutrients for in vitro cell growth, metabolism and proliferation  and is widely used in cell culture media. Prior to the emergence of variant Creutzfeldt-Jakob disease as a result of the bovine spongiform encephalitis (BSE) crisis at the end of last century, FBS was considered reasonably safe for humans. In animals however, the safety of FBS was always more questionable with more animal diseases potentially being transmissible between species. The main advantage in using serum from unborn animals consists in the absence of interfering substances like inflammatory molecules, hormones or exogenous antigens, including feed-derived components. However, FBS batches are known to be heterogeneous in their performance and need to be batch-tested. Moreover, diluted and altered FBS has been sold recently in Europe, underlining the challenges to FBS selection . Accordingly, FBS production is increasingly subject to regulations and restrictions, not least to protect animals under the 3R guidelines and reduce unnecessary pain, suffering, distress or lasting harm.
In recent years, the ex vivo generation of dendritic cells for the induction of anti-tumor responses has been a focus point for cancer immunotherapy research [20–23]. When generating dendritic cells for clinical applications, such as tumor vaccines, reproducibility and safety are of paramount importance. The use of FBS as a poorly defined cocktail of proteases and other active substances has always been less than ideal, and for both humans and animal species, the use of xenogeneic reagents needs to be avoided.
The utility of autologous serum or serum free media for the generation of MoDC has been questioned [24–26]. In horses, the use of homologous serum for cell culture has been described widely in systems other than DC generation or maintenance. Hamza et al.  used autologous serum in cell culture for functional assays involving equine peripheral blood mononuclear cells (PBMC). The use of horse serum for culture of primary equine bronchial fibroblasts  has also been described.
In the present study we examined the morphology, viability, phenotype and functional properties of eqMoDC generated under different serum conditions. For this purpose, three FBS batches from two different manufacturers were compared to horse serum produced in one of our laboratories. The data demonstrate that eqMoDC generated in the presence of heterologous horse serum perform equally well or better than dendritic cells generated with FBS.
Horses and blood samples
Blood samples were collected from the jugular vein of six healthy horses (4 geldings, 2 mares) using Sodium-Heparin containing vacutainers (Vacuette®; Greiner, St.Gallen, Switzerland). The horses were of diverse breeds (Warmblood, Freiberger, Icelandic horse) and spanned a large age range (4–25 years, mean age = 12.7 years). They had been vaccinated yearly against equine influenza and tetanus, and dewormed regularly. The horses belonged to the Swiss Institute of Equine Medicine, Vetsuisse Faculty, University of Bern.
Horse and fetal bovine sera
For preparation of horse serum (HS), blood was collected from a healthy horse into Serum Clot Activator containing vacutainers (Vacuette®; Greiner, St.Gallen, Switzerland). HS was separated by leaving the blood to clot for 2 h followed by centrifugation at 2684×g (Rotanta 46 RSC centrifuge, Hettich AG, Bäch, Switzerland) for 10 min at 4 °C and inactivation for 30 min at 56 °C in a water bath. Serum was then stored at -20 °C until used.
Three commercially available batches of fetal bovine serum were used: FBS (A15-101), Lot A10106-1060 (PAA Pasching, Austria); FBS (S0113), Lot 1107A (Biochrom GmbH, Berlin Germany); FBS Superior (S0613), Lot 0503B, (Biochrom).
In vitro generation of eqMoDC
PBMC were isolated by two sequential Ficoll density gradient centrifugations, using Biocoll 1.090 g/ml and 1.077 g/ml (Biochrom) as described by Mauel et al. . The PBMC-containing fraction was then washed twice in PBS and re-suspended in PBS supplemented with 2 mM EDTA and 0.5% of FBS or HS. Monocytes were isolated by magnetic separation (MACS technology, Miltenyi Biotec GmbH, Bergisch-Gladbach, Germany) according to the manufacturer’s standard protocols, using a monoclonal anti-equine CD14 antibody (clone 105) . Briefly, PBMC were first incubated with anti-CD14 and, after a washing step, with secondary goat anti-mouse micro beads. The cells were then separated on a LS column (Miltenyi Biotec GmbH). 2 × 106 monocytes were incubated in a 12-well tissue culture plate (Falcon, BD Biosciences, San Jose CA, USA) in 2 ml RPMI 1640 medium with HEPES and L-glutamine (Gibco, Life Technologies Ltd, Paisley UK) supplemented with 1% penicillin and streptomycin (Gibco), 1% MEM vitamins, 1% Na pyruvate, 1% Non-essential amino acids (all Biochrom) and either 10% FBS (A15-101), FBS (S0113), FBS (S0613) or 5% HS.
Endotoxin contamination was assessed in all serum-supplemented media using a qualitative in vitro end-point endotoxin assay (ToxinSensor™, GenScript, Piscataway, NJ, USA). Lipopolysaccharide (LPS) levels were below 0.06 I.U./ml in all media. Differentiation into eqMoDC was induced by addition of 25 ng/ml recombinant (r.) equine GM-CSF and 10 ng/ml (r.) equine IL-4 (both Kingfisher Biotech Inc., St. Paul MN, USA) and cells were cultured for 3 days. Cells were monitored daily by light microscopy for changes in morphology.
Viability of three day old immature eqMoDC was assessed using the Alexa Fluor 488 annexin V/Dead Cell Apoptosis Kit for Flow Cytometry (Invitrogen Life Technologies, Paisley, UK) according to the protocol provided by the manufacturer. Briefly, cells were harvested from the cell culture plates, washed and an aliquot of cells was suspended in 0.4% Trypan Blue for counting using a hemocytometer (Neubauer). The cells were resuspended in annexin-binding buffer, incubated with 5 μl AF488 annexin V and 1 μl of 100 μg/ml propidium iodide for 15 minutes at room temperature, then analysed immediately by flow cytometry.
Analysis of eqMoDC phenotype by flow cytometry
MoDC phenotypes were assessed by surface marker expression analysis using the following monoclonal antibodies: anti-equine CD14 mAb (clone 105) , anti-human CD206 clone 3.29B1.10 (Beckman Coulter, High Wycombe, UK) and anti-human CD86 clone IT2.2 (Becton Dickinson, Oxford, UK). Unlabelled antibodies were labelled using anti-mouse IgG1 zenon Kits (Invitrogen Life Technologies). Appropriate isotype controls were used. Analysis of cells was performed using a BD LSRII Flow Cytometer (BD Biosciences) and FlowJo software 6 (Tree Star Inc. Ashland OR, USA).
Transcriptome analysis of eqMoDC populations
RNA was extracted from cell pellets of 1 × 106 cells using the RNAqueous micro Kit (Life Technologies, Qiagen, Crawley, UK) and stored at -80 °C. RNA quality was assessed with the RNA 6000 Pico Labchip kit on the Agilent 2100 Bioanalyzer (Agilent Technologies, Berkshire, United Kingdom). The Ovation PicoSL WTA System v2 kit (NuGEN, Leek, The Netherlands) was used to amplify cDNA from 50 ng total RNA. The MinElute Reaction Cleanup Kit (Qiagen) option was used to purify cDNA, and 1 μg was then labelled using a one-color DNA labelling kit (NimbleGen, Madison, USA). For each sample, 4 μg labelled cDNA was hybridised to the NimbleGen 12 × 135 K custom equine arrays (Roche, Madison, USA). Three biological repeats were analysed for each data set. Hybridised arrays were scanned at 2 μm resolution with the Agilent High-resolution C Microarray Scanner (Agilent, Wokingham, UK). Microarray images were processed using DEVA v1.2.1 software (Roche, Madison, USA) to obtain a report containing the signal intensity values corresponding to each probe. The raw data was pre-processed using the DEVA v1.2.1 software by log2 transformation followed by RMA normalisation and summarisation to yield a signal intensity value for each probe set. The data set was then filtered by variance and Principal Component Analysis (PCA) was performed using Qlucore v2.0 software (Qlucore, Lund, Sweden). Variance levels were set using the δ/δmax method.
EqMoDC maturation and functional T cell stimulation assays
For antigen-presentation assays, immature eqMoDC were re-suspended at 2×105 cells per 150ul of RPMI 1640 complete medium containing FBS or HS and incubated for 90 min at 37 °C either with 20 μg/ml tetanus toxoid (Schweizerisches Serum und Impfinstitut Bern, Switzerland) as a recall antigen, or 20 μg/ml of the primary antigen ovalbumin (OVA, kindly provided by the Swiss Institute for Allergy and Asthma Research, University of Zürich, Davos Switzerland), or with medium alone as a control. After antigen uptake, eqMoDC were washed and cultured in a 96-well round bottom tissue culture plate (Sarstedt, Nümbrecht, Germany) at 2×104 eqMoDC per well in quadruplicates.
For maturation, antigen-primed eqMoDC were exposed overnight to a maturation cocktail comprising 1 μg/ml LPS (Sigma-Aldrich St. Louis MO, USA), 1 μg/ml PGE2 (Enzo Life Sciences, Exeter, UK), 20 ng/ml equine TNF-α, 10 ng/ml equine IL-1β, 20 ng/ml equine IL-6 and 100 ng/ml equine IFN-γ (all R&D Systems, Abingdon, UK) according to Moyo et al. .
Fresh CD5+ T lymphocytes were enriched by positive selection using MACS technology as above-mentioned, employing an anti-equine CD5 mAb (clone CVS5, Abd Serotec, Kidlington UK) and re-suspended in RPMI 1640 medium containing FBS or HS, respectively. Purity of CD5+ lymphocytes after bead selection was assessed by flow cytometry and was shown to be > 94%. 105 autologous CD5+ T lymphocytes were added to the MoDC in the 96-well plate and co-cultured for 5 days at 37 °C/5% CO2. 5 μCi/well [3H] thymidine (Perkin Elmer, Waltham MA, USA) was added for the last 18 h of culture. DNA was then harvested onto a glass fibre filter plate and thymidine incorporation was measured on a scintillation counter (Inotech, LabLogic Systems Inc., Brandon FL, USA).
A mixed leukocyte reaction (MLR) was performed in addition to the autologous co-cultures by incubating matured eqMoDC with CD5+ T lymphocytes from another horse.
Cell counts of immature eqMoDC generated after 3 days in vitro
Non-parametric paired sample Wilcoxon (signed rank) test was again used to assess differences in serum conditions with regard to induction of T cell proliferation by antigen-primed MoDC (Figs. 5 and 6). Overall, p-values ≤ 0.05 were considered significant.
Morphology of differentiating eqMoDC differs between cells generated in the presence of HS or FBS
Immature eqMoDC generated in the presence of HS exhibit a higher viability
Surface marker expression of eqMoDC reflects maturation status and is comparable between serum conditions
Transcriptome comparison of eqMoDC preparations and populations
Induction of T cell proliferation by antigen-primed MoDC
Dendritic cells are key players in the immune system, particularly competent in modulating the immune responses . Thus they are promising tools both for cancer immunotherapy and to limit immune responses to treat allergic reactions [30, 31]. The ability to generate these otherwise scarce immune cells in large quantities from progenitors and in particular monocytes, reinitiated research in this field around 20 years ago [6, 7, 32]. The identification of distinct DC populations in vivo, among them DC specialized in cross-presenting antigens to CD8+ cytotoxic T cells  has widened the opportunities to study specialized subsets of DC. MoDC remain the first choice for personalized therapeutic approaches, such as loading DC ex vivo, as they were shown to substitute for all DC functions, including cross-presentation .
Fetal bovine serum (FBS) is widely used in cell culture media, but has come under more intense scrutiny in recent years: as well as being a possible source for disease transmission its use in therapeutic vaccines may lead to adverse immune reactions against FBS [35, 36]. The problem of batch variability, including the contamination with LPS (which is detrimental to MoDC differentiation), was immediately recognised as an issue for therapeutic use of DC .
Early work to replace the 5–10% FBS commonly used to generate human MoDC by an equal amount of human sera (either autologous or batch tested) has not been successful (Steinbach et al., unpublished; various personal communications). This was explained by the plasticity of monocytes as uncommitted myeloid cells during differentiation allowing them to acquire a macrophage rather than a DC phenotype . It was accordingly suggested to replace the 10% FBS by 1% autologous plasma, but while the phenotypical and functional data were analogous to FBS-derived MoDC, the DC yield obtained was very low (around 20% compared to FBS based protocols) with a significantly reduced enrichment . This was offset by larger scale production , which, however, does not address the issue of cell debris from dead cells in such cultures.
In horses, previous studies to generate MoDC under the influence of GM-CSF and IL-4 used FBS [14, 16, 17] and pilot studies have also shown the potential use of such ex vivo generated MoDC for treatment of tumors . However, previous experience where FBS-specific IgE was induced through MoDC application , eliminated such equine MoDC for the purpose of allergen immunotherapy.
In a preliminary experiment, we compared the use of autologous and heterologous equine serum with FBS from PAA (A15-101), which was used in one of our laboratories for the maintenance of cells lines. Intriguingly, while both equine serum preparation delivered encouraging results, the A15-101 FBS led to morphologically more heterogeneous populations with giant cells that we presumed to be the result of cell death followed by phagocytosis, not matching previous descriptions [14, 17]. Since the results obtained with the two serum preparations from horses were very similar, we decided to generate a heterologous serum to achieve a better standardisation for subsequent experiments. In addition, it became necessary to expand our study to other FBS batches able to reproduce previous results . Thus, we decided to conduct a small study comparing three different FBS with HS during the generation of equine MoDC and their application in functional assays. The aim was to determine if equine MoDC could be successfully generated using horse serum that was freshly prepared rather than commercial serum that previously failed to deliver equine MoDC (Steinbach et al., unpublished).
The differentiation from monocytes to MoDC is characterised by the formation of tight cell clusters, where cells gradually become non-adherent and develop typical dendrites [6, 41]. It was notable that equine MoDC differentiated with HS developed larger clusters faster than monocytes incubated with FBS, which showed only limited clustering by day 2 (Fig. 1). It is not known whether the formation of cell clusters and thus close cell-to-cell contact is necessary for differentiating monocytes to become fully functional, but eqMoDC cultured in the presence of HS were also significantly more viable. It is thus likely that cell-cell signalling within clusters promotes viability of cells in culture. Not surprisingly and in line with the preliminary data, FBS batch A15-101 showed the highest proportion of non-viable cells. These results, however, do not explain whether HS contains additional viability factors which are lacking in FBS, or whether the changes and additions made to FBS batch A15-101 were detrimental to eqMoDC differentiation. Interestingly, there seems to be an inherent variation between individual horses in the proportion of non-viable cells that was independent of the serum used. Regardless of the serum condition, the same horse delivered the highest as well as the lowest proportion of dead cells. Thus, it is reasonable to propose that individual disposition (from genetics to an individual’s current health status) likely affects the generation of eqMoDC ex vivo. This resonates an earlier study showing that monocytes from Lupus Erythematosus patients required more GM-CSF and IL-4 to obtain viable DC .
As with the morphology and viability, clear differences were observed for the phenotype between the four tested sera: again, eqMoDC incubated with the two FBS from Biochrom displayed very similar phenotypes and maturation patterns, which were likely due to a similar FBS composition that should be observed using high performance FBS batches. Slightly surprising though was the relatively high level of CD14 remaining on MoDC generated with the Biochrom FBS. Since we tested all media for LPS this can be excluded as the causative factor. MoDC generated with HS expressed slightly higher levels of CD86 already at the immature stage. Overall, though all cells displayed a phenotype in accordance with MoDC differentiation and maturation and only trends were observed that made cells treated with HS preferable, i.e. is more in line with the published gold standard, to those treated with FBS. Accordingly, it was not surprising that in a whole transcriptome analysis the three differentiation stages were clearly separable, whereas the different sera clustered strongly together similar to previous results . This is not astonishing, since across a whole population of cells of the same lineage, only minute shifts in gene expression will suffice to induce the changes in protein expression and morphology such as observed by flow cytometry. This emphasises that all four sera delivered equine MoDC of some quality.
It is important to consider that ultimately, DC are not defined by the presence or absence of certain markers, but by their functional ability to stimulate T cells. Here, HS clearly demonstrated an advantage through not inducing non-specific proliferation. This result, observed with all batches of FBS, may reflect their xenogenous and antigenetic nature, with T cells in adult horses reacting against foreign serum components or exogenous agents. To exclude the latter we tested the FBS batches for the presence of pestivirus RNA (a common contaminant of FBS) and can exclude this as a factor. However, as all horses in this study were regularly vaccinated, a sensitisation to foreign proteins present in these vaccines may well have occurred and has been described for equine vaccines before . The strongest proliferation was induced in the heterologous mixed leukocyte reaction (MLR) followed by an antigen-specific recall response against tetanus toxoid. This was to be expected compared to a primary antigen like OVA, where the response relies on the activation of naïve rather than memory T cells. Using the stimulation index to determine the specific reaction above the background, the best performance was observed with HS.
It can be concluded that eqMoDC generated in the presence of HS showed improved morphological characteristics, higher cell viability and were superior with a more robust performance in the functional T cell assays. While HS did not perform significantly better in all assays, it is the mixture of results that favours HS for the generation of eqMoDC. While PAA’s FBS (A15-101) did not perform worst in all experiments, its inferior performance in morphology and viability assays and the lack of clarity surrounding its composition and thereby functional reproducibility exclude this product completely from use . While FBS can in general be considered further for in vitro research, the results here re-emphasize the need for batch testing. These results are very encouraging for the clinical application of equine MoDC and confirm a most recent report using cells generated with horse serum for recall responses . However, the effect of autologous serum or different serum conditions on the phenotype and function of equine MoDC had not been systematically investigated previously. Prior to clinical application, though horse sera need to be tested extensively for extraneous agents, like the widespread equine hepaciviruses and or treated for inactivation of such. Thus, the serum free generation of MoDC would be desirable, but this has proven inefficient, resulting in very limited cell numbers [8, 45] and is still a matter of debate [24–26, 46, 47]. With the recent progress in defining serum free media for various purposes (discussed in ) this goal can be achieved in the near future, but requires further studies to ensure good compliance with MoDC functionality as well.
We would like to thank Dr. Andreas Zurbriggen, Department of Clinical Research and Veterinary Public Health, Vetsuisse Faculty, University of Bern for his continuous support, Dr. Bettina Wagner at the Department of Population Medicine and Diagnostic Sciences, College of Veterinary Medicine, Cornell University, Ithaca, 825 NY 14853, USA for providing the anti-equine CD14 antibody. We are also thankful to Biochrom GmbH for providing the FBS samples used in this study.
This work was supported by a grant of the Department of Clinical Research VPH, Vetsuisse Faculty, University of Bern, by the Swiss National Science Foundation grant no. 310030-160196/1 and by the APHA grant SCRD0092 ‘Systems Biology for Veterinary Species’.
Availability of data and materials
The array data has been deposited in GEO, accession number GSE84031.
AZ carried out the immunological experiments, assisted in the design of the study and drafted the manuscript. HE carried out the transcriptome analysis. EH participated in and supervised the immunological experiments. MG was responsible for production and purification of the ovalbumin used in this study. VG provided the horses used in this study and edited the manuscript. EM participated in the design and coordination of the study and assisted with statistical analysis and preparation of the manuscript and figures. FS conceived the study, participated in its design and edited the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent for publication
This study was approved by the Ethical Committee for Animal Experiments of the Canton of Berne, Switzerland (No. BE 51/13).
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Steinman RM. The dendritic cell system and its role in immunogenicity. Annu Rev Immunol. 1991;9:271–96. Review.View ArticlePubMedGoogle Scholar
- Croft M, Duncan DD, Swain SL. Response of naive antigen-specific CD4+ T cells in vitro: characteristics and antigen-presenting cell requirements. J Exp Med. 1992;176(5):1431–7.View ArticlePubMedGoogle Scholar
- Cella M, Sallusto F, Lanzavecchia A. Origin, maturation and antigen presenting function of dendritic cells. Curr Opin Immunol. 1997;9(1):10–6.View ArticlePubMedGoogle Scholar
- Steinman RM, Nussenzweig MC. Dendritic cells: features and functions. Immunol Rev. 1980;53:127–47. Review.View ArticlePubMedGoogle Scholar
- Inaba K, Inaba M, Romani N, Aya H, Deguchi M, Ikehara S, Muramatsu S, Steinman RM. Generation of large numbers of dendritic cells from mouse bone marrow cultures supplemented with granulocyte/macrophage colony-stimulating factor. J Exp Med. 1992;176(6):1693–702.View ArticlePubMedGoogle Scholar
- Sallusto F, Lanzavecchia A. Efficient presentation of soluble antigen by cultured human dendritic cells is maintained by granulocyte/macrophage colony-stimulating factor plus interleukin 4 and downregulated by tumor necrosis factor alpha. J Exp Med. 1994;179(4):1109–18.View ArticlePubMedGoogle Scholar
- Peters JH, Gieseler R, Thiele B, Steinbach F. Dendritic cells: from ontogenic orphans to myelomonocytic descendants. Immunol Today. 1996;17:273–8.View ArticlePubMedGoogle Scholar
- Romani N, Reider D, Heuer M, Ebner S, Kämpgen E, Eibl B, Niederwieser D, Schuler G. Generation of mature dendritic cells from human blood. An improved method with special regard to clinical applicability. J Immunol Methods. 1996;196(2):137–51.View ArticlePubMedGoogle Scholar
- Bender A, Sapp M, Schuler G, Steinman RM, Bhardwaj N. Improved methods for the generation of dendritic cells from nonproliferating progenitors in human blood. J Immunol Methods. 1996;196(2):121–35.View ArticlePubMedGoogle Scholar
- Jonuleit H, Kühn U, Müller G, Steinbrink K, Paragnik L, Schmitt E, Knop J, Enk AH. Pro-inflammatory cytokines and prostaglandins induce maturation of potent immunostimulatory dendritic cells under fetal calf serum-free conditions. Eur J Immunol. 1997;27(12):3135–42.View ArticlePubMedGoogle Scholar
- Werling D, Hope JC, Chaplin P, Collins RA, Taylor G, Howard CJ. Involvement of caveolae in the uptake of respiratory syncytial virus antigen by dendritic cells. J Leukoc Biol. 1999;66(1):50–8.PubMedGoogle Scholar
- Paillot R, Laval F, Audonnet JC, Andreoni C, Juillard V. Functional and phenotypic characterization of distinct porcine dendritic cells derived from peripheral blood monocytes. Immunology. 2001;102:396–404.View ArticlePubMedPubMed CentralGoogle Scholar
- Chan SS, McConnell I, Blacklaws BA. Generation and characterization of ovine dendritic cells derived from peripheral blood monocytes. Immunology. 2002;107(3):366–72.View ArticlePubMedPubMed CentralGoogle Scholar
- Mauel S, Steinbach F, Ludwig H. Monocyte-derived dendritic cells from horses differ from dendritic cells of humans and mice. Immunology. 2006;117(4):463–73.View ArticlePubMedPubMed CentralGoogle Scholar
- Dietze B, Cierpka E, Schäfer M, Schill W, Lutz MB. An improved method to generate equine dendritic cells from peripheral blood mononuclear cells: divergent maturation programs by IL-4 and LPS. Immunobiology. 2008;213(9–10):751–8.View ArticlePubMedGoogle Scholar
- Cavatorta DJ, Erb HN, Flaminio MJ. Ex vivo generation of mature equine monocyte-derived dendritic cells. Vet Immunol Immunopathol. 2009;131(3–4):259–67.View ArticlePubMedGoogle Scholar
- Moyo NA, Marchi E, Steinbach F. Differentiation and activation of equine monocyte-derived dendritic cells are not correlated with CD206 or CD83 expression. Immunology. 2013;139(4):472–83.View ArticlePubMedPubMed CentralGoogle Scholar
- Bettger WJ, McKeehan WL. Mechanisms of cellular nutrition. Physiol Rev. 1986;66(1):1–35. Review.PubMedGoogle Scholar
- Köppele W. Unbekannte Zusätze. Laborjournal. 2013;9:67–69.Google Scholar
- Tacken PJ, Jolanda I, de Vries M, Torensma R, Figdor CG. Dendritic-cell immunotherapy: from ex vivo loading to in vivo targeting. Nat Rev Immunol. 2007;7:790–802.View ArticlePubMedGoogle Scholar
- Palucka KA, Banchereau J. Cancer immunotherapy via dendritic cells. Nat Rev Cancer. 2012;12:265–77.View ArticlePubMedPubMed CentralGoogle Scholar
- Apostolopoulos V, Pietersz GA, Tsibanis A, Tsikkinis A, Stojanovska L, McKenzie IF, Vassilaros S. Dendritic cell immunotherapy: clinical outcomes. Clin Transl Immunology. 2014;3(7), e21.View ArticlePubMedPubMed CentralGoogle Scholar
- Anguille S, Smits EL, Bryant C, van Acker HH, Goossen H, Lion E, Fromm PD, Hart DN, van Tendeloo VF, Berneman ZN. Dendritic Cells as Pharmacological Tools for Cancer Immunotherapy. Pharmacol Rev. 2015;67(4):731–53.View ArticlePubMedGoogle Scholar
- Pietschmann P, Stöckl J, Draxler S, Majdic O, Knapp W. Functional and phenotypic characteristics of dendritic cells generated in human plasma supplemented medium. Scand J Immunol. 2000;51(4):377–83.View ArticlePubMedGoogle Scholar
- Loudovaris M, Hansen M, Suen Y, Lee SM, Casing P, Bender JG. Differential effects of autologous serum on CD34(+) or monocyte-derived dendritic cells. J Hematother Stem Cell Res. 2001;10(4):569–78.View ArticlePubMedGoogle Scholar
- Garderet L, Cao H, Salamero J, Vergé V, Tisserand E, Scholl S, Gorin NC, Lopez M. In vitro production of dendritic cells from human blood monocytes for therapeutic use. J Hematother Stem Cell Res. 2001;10(4):553–67. Review.View ArticlePubMedGoogle Scholar
- Hamza E, Doherr MG, Bertoni G, Jungi TW, Marti E. Modulation of allergy incidence in icelandic horses is associated with a change in IL-4-producing T cells. Int Arch Allergy Immunol. 2007;144(4):325–37.View ArticlePubMedGoogle Scholar
- Franke J, Abs V, Zizzadoro C, Abraham G. Comparative study of the effects of fetal bovine serum versus horse serum on growth and differentiation of primary equine bronchial fibroblasts. BMC Vet Res. 2014;10:119.View ArticlePubMedPubMed CentralGoogle Scholar
- Kabithe E, Hillegas J, Stokol T, Moore J, Wagner B. Monoclonal antibodies to equine CD14. Vet Immunol Immunopathol. 2010;138(1–2):149–53.View ArticlePubMedGoogle Scholar
- Grabbe S, Beissert S, Schwarz T, Granstein RD. Dendritic cells as initiators of tumor immune responses: a possible strategy for tumor immunotherapy? Immunol Today. 1995;16(3):117–21. Review.View ArticlePubMedGoogle Scholar
- Steptoe RJ, Thomson AW. Dendritic cells and tolerance induction. Clin Exp Immunol. 1996;105(3):397–402. Review.View ArticlePubMedPubMed CentralGoogle Scholar
- Porcelli S, Morita CT, Brenner MB. CD1b restricts the response of human CD4-8- T lymphocytes to a microbial antigen. Nature. 1992;360(6404):593–7.View ArticlePubMedGoogle Scholar
- Merad M, Sathe P, Helft J, Miller J, Mortha A. The dendritic cell lineage: ontogeny and function of dendritic cells and their subsets in the steady state and the inflamed setting. Annu Rev Immunol. 2013;31:563–604.View ArticlePubMedGoogle Scholar
- Cheong C, Matos I, Choi JH, Dandamudi DB, Shrestha E, Longhi MP, Jeffrey KL, Anthony RM, Kluger C, Nchinda G, Koh H, Rodriguez A, Idoyaga J, Pack M, Velinzon K, Park CG, Steinman RM. Microbial stimulation fully differentiates monocytes to DC-SIGN/CD209+ dendritic cells for immune T cell areas. Cell. 2010;143:416–29.View ArticlePubMedPubMed CentralGoogle Scholar
- Selvaggi TA, Walker RE, Fleisher TA. Development of antibodies to fetal calf serum with arthus-like reactions in human immunodeficiency virus-infected patients given syngeneic lymphocyte infusions. Blood. 1997;89(3):776–9.PubMedGoogle Scholar
- Mackensen A, Dräger R, Schlesier M, Mertelsmann R, Lindemann A. Presence of IgE antibodies to bovine serum albumin in a patient developing anaphylaxis after vaccination with human peptide-pulsed dendritic cells. Cancer Immunol Immunother. 2000;49(3):152–6.View ArticlePubMedGoogle Scholar
- Schuler G, Steinman RM. Dendritic cells as adjuvants for immune-mediated resistance to tumors. J Exp Med. 1997;186(8):1183–7.View ArticlePubMedPubMed CentralGoogle Scholar
- Palucka KA, Taquet N, Sanchez-Chapuis F, Gluckman JC. Dendritic cells as the terminal stage of monocyte differentiation. J Immunol. 1998;160(9):4587–95.PubMedGoogle Scholar
- Berger TG, Feuerstein B, Strasser E, Hirsch U, Schreiner D, Schuler G, Schuler-Thurner B. Large-scale generation of mature monocyte-derived dendritic cells for clinical application in cell factories. J Immunol Methods. 2002;268(2):131–40.View ArticlePubMedGoogle Scholar
- Steinbach F, Bischoff S, Freund H, Metzner-Flemisch S, Ibrahim S, Walter J, Wilke I, Mauel S. Clinical application of dendritic cells and interleukin-2 and tools to study activated T cells in horses - first results and implications for quality control. Vet Immunol Immunopathol. 2009;128(1–3):16–23.View ArticlePubMedGoogle Scholar
- Steinbach F, Krause B, Bläß S, Burmester GR, Hiepe F. Development of accessory phenotype and function during the differentiation of Monocyte-derived dendritic cells (MoDC). Res Immunol. 1998;149:627–32.View ArticlePubMedGoogle Scholar
- Steinbach F, Henke F, Krause B, Thiele B, Burmester GR, Hiepe F. Monocytes from SLE patients are severely altered in phenotype and lineage flexibility. Ann Rheum Dis. 2000;59:283–8.View ArticlePubMedPubMed CentralGoogle Scholar
- Newton JR, Geraghty RJ, Castillo-Olivares J, Cardwell M, Mumford JA. Evidence that use of an inactivated equine herpesvirus vaccine induces serum cytotoxicity affecting the equine arteritis virus neutralisation test. Vaccine. 2004;22:4117–23.View ArticlePubMedGoogle Scholar
- Meulenbroeks C, van der Meide NM, Willemse T, Rutten VP, Tijhaar E. Recombinant Culicoides obsoletus complex allergens stimulate antigen-specific T cells of insect bite hypersensitive Shetland ponies in vitro. Vet Dermatol. 2015;26(6):467–109.View ArticlePubMedGoogle Scholar
- Toungouz M, Quinet C, Thille E, Fourez S, Pradier O, Delville JP, Velu T, Lambermont M. Generation of immature autologous clinical grade dendritic cells for vaccination of cancer patients. Cytotherapy. 1999;1(6):447–53.View ArticlePubMedGoogle Scholar
- Lehner M, Morhart P, Stilper A, Holter W. Functional characterization of monocyte-derived dendritic cells generated under serum-free culture conditions. Immunol Lett. 2005;99(2):209–16.View ArticlePubMedGoogle Scholar
- da Silva SG, Saad ST, Gilli SC. An efficient protocol for the generation of monocyte derived dendritic cells using serum-free media for clinical applications in post remission AML patients. Ann Clin Lab Sci. 2014;44(2):180–8.Google Scholar
- van der Valk J, Brunner D, de Smet K, Fex Svenningsen A, Honegger P, Knudsen LE, Lindl T, Noraberg J, Price A, Scarino ML, Gstraunthaler G. Optimization of chemically defined cell culture media -replacing fetal bovine serum in mammalian in vitro methods. Toxicol In Vitro. 2010;24(4):1053–63.View ArticlePubMedGoogle Scholar