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Introduction

Psoriasis is a T cell mediated, chronic inflammatory autoimmune skin disease (1) with joint manifestations, that affects up to 2–3% of the global population (2) and leads to a decrease in quality of life (3). Psoriasis is associated with psoriatic arthritis (4) and depressive illness (5,6). Several cardiometabolic pathologies (7) are also associated with psoriasis, including obesity (8), dislipidemia (9), diabetes (10) and venous thromboembolism (11).

The causes of psoriasis are not fully understood; genetic factors and an inneffective immune system seem to be the main factors involved in the etiology of this pathology. Other aggravating factors are skin trauma, streptococcal infections, endocrine factors, certain medications, emotional stress, smoking, alcohol and environmental factors (12).

From a clinical point of view, psoriasis can be divided in two main groups: non-pustular (psoriasis vulgaris, guttate, erythrodermic, palmoplantar, psoriatic arthritis and inverse psoriasis) and pustular psoriasis (generalized pustular psoriasis, impetigo herpetiformis and localized pustular psoriasis) (13). These clinical variants have common features consisting of erythema, skin scaling and thickening. The assessment of psoriasis severity and evolution is based on clinical indicators (PASI score) (14), but also on the quality of life of the patient (DLQI score) (15). The clinical type of psoriasis and the severity of the psoriatic lesions are important elements in establishing the treatment in this disease. There are three main types of therapies: Topical treatment (for mild forms), light therapy (for moderate to severe forms) and systemic medication (for severe forms) (16).

Clinical and experimental data accumulated in recent years highlighted the important role played by the immune system in the pathogenesis of psoriasis. Although it is considered a T-cell-mediated inflammatory disease, the pathogenesis of psoriasis involves cells belonging to both adaptive and innate immunity (dendritic cells, NK cells, macrophages) as well as non-immune cells (keratinocytes, endothelial cells) (17). The autoantigens that activate autoimmune reactions in psoriasis are not fully described. LL-37, an antimicrobial peptide produced by keratinocytes was found overexpressed in moderate to severe psoriatic forms (18). Recent studies reveal another possible autoantigen, ADAMTS-like protein 5, that is produced by melanocytes and was shown to activate the Th17 response (19).

Two phases are described in the pathogenesis of psoriasis: the initiation and the maintenance of the disease. Some triggering factors trigger the secretion of TNF-α, IFN-γ and IL-6 by plasmacytoid dendritic cells, NK cells, macrophages and keratinocytes. These mediators activate myeloid dendritic cells that release IL-12 and IL-23. IL-12 leads to differentiation of naive T lymphocytes in Th1 lymphocytes, which will secrete IFN-γ and TNF-α; IL-23 causes differentiation of naive T lymphocytes in Th17 lymphocytes, which secrete IL-17A, IL-17F and IL-22. These mediators further activate keratinocytes that induce the production of antimicrobial peptides (LL-37), proinflammatory cytokines (TNF-α, IL-1β, IL-6), chemokines and S100 proteins, hence maintaining and propagating inflammation (20).

Due to the importance of immunological mechanisms in the pathogenesis of psoriasis, therapeutical research has been directed towards isolating compounds that block or inhibit these mechanisms. Clinical trials using biological agents that target specific components of the immune system are currently underway. There is a panel of drugs already approved or that are in the testing stage (21–26). Currently available biological therapies are: anti-TNF-α agents (Infliximab, Adalimumab, Etanercept), anti-LFA-1 (Efalizumab), IL-17 inhibitors (Brodalumab, Ixekizumab and Secukinumab), IL-23 inhibitors (Guselkumab), and IL-12/23 inhibitors (Ustekinumab) (27,28).

Non-human psoriasis models are an important research tool that attempts to reproduce in vitro and in vivo the clinical features of the disease in order to explain the pathogenesis of psoriasis and to identify possible therapeutic targets. Animal models of psoriasis must reflect specific clinical features of the disease, including histological alterations, a similar pathogeny and a comparable response to therapeutic agents. Although murine models successfully mimic psoriasiform dermatitis, the differences between the two species (mouse vs. human) are a disadvantage of in vivo models. Traditional models of experimental psoriasis in mice, based on spontaneous mutations or genetic engineering, are defined by high costs and expertise.

A more accessible and easier-to-implement alternative is the induction of psoriasis-like skin lesions by the topical application of Imiquimod (IMQ), a nucleoside (1-isobutyl-1H-imidazo[4,5-c]quinolin-4-amine) analogue of imidazoquinoline family (29). It is an anti-viral and anti-neoplastic drug used in the treatment of genital warts, basal cell carcinoma and actinic keratosis. IMQ is a ligand of TLR7 and TLR8 (30), an activator of the NF-κB and, consequently, a potent immune modulator. IMQ mimics partially the pathogenic processes of psoriasis, acting at the interface between innate and acquired immunity both directly and indirectly (31). Direct action consists of binding of TLR7 and TLR8 on macrophages, monocytes and dendritic cells, and indirect action refers to the induction of pro-inflammatory cytokine secretion, such as IFN-γ, IL-6 and TNF-α. IMQ increases the ability of Langerhans cells to present the antigen and stimulates their migration to the lymph nodes where the antigens are presented to T lymphocytes, thus activating the adaptive immune response. Topical application of IMQ induces increased IL-6 and IL-8 production by activated keratinocytes (32). IMQ-induced cytokine production elicits a Th1-weighted cellular immune response, enhancing the activation of cytotoxic T cells and inhibiting the Th2-mediated response (33). The IMQ-based model of psoriasiform dermatitis offers a series of advantages: it is relatively easy to use, control and reproduce, while the induced dermatitis closely mimics the pathologic changes in human psoriasis.

In order to emphasize changes in immune cell populations involved in lesion pathogenesis, we performed a murine model of psoriasiform dermatitis model by topical IMQ application. IMQ-induced skin inflammation and lesions were assessed using in vivo measurements and histological data, while the cellular evaluation for T, B and NK cell populations was performed by flow cytometry. The changes in these cell populations were analysed in peripheral blood, spleen and skin to observe the immune area affected by the pathological process. The evaluation was intended to establish the immune framework of this experimental model that could be further used for etipathogenic mechanisms identification and/or for studies regarding targeted therapies.

Materials and methods

Animal strain

C57BL/6 mice, purchased from Jackson Laboratory (Bar Harbor, ME, USA), were provided by the Animal Husbandry from Victor Babeș National Institute. The animals were maintained in a temperature-controlled, air-conditioned animal house (20±4°C, 55±10% humidity) with a 12/12-light/dark cycle. The mice were housed in individual cages in an open cage system and received food and water ad libitum. The animals were monitored daily. The study protocol was approved by the Ethics Committee from ‘Victor Babeș’ Institute (Bucharest, Romania), and mouse handling was done in accordance with recognized principles of laboratory animal care in the framework of EU Directive 2010/63/EU for animal experiments (34).

IMQ-based murine model of psoriatic dermatitis

In order to induce psoriatic dermatitis, an IMQ-based murine model of psoriasiform dermatitis was replicated according to the protocols described in literature (35). Three groups of C57BL/6 mice were considered (1:1 sex ratio), 8–11 weeks old, with a mean weight of 21±3 g (Balance Scientech SL-3100D; Boulder, CO, USA), free of any medication in the previous 72 h: (i) the psoriasis group (10 mice) received a daily topical dose of 62.5 mg IMQ cream (5% Aldara Cream; Meda AB, Sweden) on the shaved back for 5 consecutive days (a daily dose of 3.125 mg of active compound); (ii) the control group (10 mice) was treated similarly with vaseline-based cream (Locobase Cream, Astellas Pharma European BV, Leiderdorp, The Netherlands); and (iii) the normal group (15 mice) with no topical treatment.

Evaluation of IMQ-induced skin inflammation in vivo measurements

The progress and the severity of the inflammation of the back skin were monitored daily for erythema (redness), desquamation (skin scaling) and induration (thickening), on a scale from 0 to 4: 0, none; 1, slight; 2, moderate; 3, marked; and 4, very marked. A modified PASI score was calculated as a cumulative score (erythema + scaling + thickening; the affected area was not taken into account), on a range from 0 to 12 for each day of treatment.

Blood and tissues sampling

After 6 days from the experiment initiation all the animals were weighed and anesthetized with ketamine/acepromazine, 100 mg/kg/5 mg/kg (Ketathesia; Henry Schein Animal Health, Dublin, OH, USA/Phoenix Pharmaceuticals, St. Joseph, MO, USA) prior to blood collection. Blood was collected by retro-orbital puncture in K2-EDTA coated tubes (Microvette; Sarstedt AG & Co., Numbrecht, Germany). All the animals were sacrificed for spleens and skin sampling.

Assessing the splenomegaly

The spleens were weighed (Balance AEP-1500 A; Adam Equipment Co., Ltd., Milton Keynes, UK) separately in order to assess the splenomegaly by calculating the ratio of the weight of the spleen (SW) and bodyweight (BW).

Histopathological evaluation

Skin samples removed from the back skin were fixed in 10% buffered formalin, embedded in paraffin, sectioned in 5 µm thick sections, stained with haematoxylin and eosin (H&E) and examined by pathologists.

Isolation of spleen cells

Single cell suspensions (for all groups of mice) were prepared from spleen by mechanical disruption; the spleens were harvested in RPMI-1640 media with 5% FBS (Biochrom GmbH, Berlin, Germany) and passed through a 70 µm cell strainer (BD Falcon; BD Biosciences, San Jose, CA, USA). The suspensions were centrifuged for 5 min at 350 g and resuspended in Cell Staining Buffer (BioLegend, San Diego, CA, USA) at 106 cells/ml.

Preparation of skin cell suspensions

Skin cell suspensions (for test and control groups) were prepared from skin by mechanical disruption (Tissue Ruptor, Qiagen Istruments Hambrechtikon, Switzerland); the skin samples were harvested in RPMI-1640 media with 5% FBS (Biochrom GmbH) and passed through a 70 µm cell strainer (BD Falcon; BD Biosciences) after the mechanical disruption. The suspensions were centrifuged for 5 min at 350 g and resuspended in Cell Staining Buffer (BioLegend) at 106 cells/ml.

Flow cytometry analysis

Blood samples, spleen and skin cell suspensions (for considered groups of mice) were incubated with TruStain fcX (anti-mouse CD16/32, isotype Rat IgG2a, λ) antibody (BioLegend) in order to block non-specific antibody binding, then stained for 20 min at room temperature with the following antibodies: Alexa Fluor 647 anti-mouse CD3ε (clone 145-2C11, isotype Armenian Hamster IgG) (BioLegend), Brilliant Violet 421 anti-mouse CD4 (clone GK1.5, isotype Rat IgG2b, κ) (BD Horizon; BD Biosciences), Alexa Fluor 488 anti-mouse CD8a (clone 53–6.7, isotype Rat IgG2a, κ), PerCP/Cy5.5 anti-mouse CD19 (clone 6D5, isotype Rat IgG2a, κ) (both from BioLegend) and Brilliant Violet 510 anti-mouse NK1.1 (clone PK136, isotype mouse IgG2a, κ) (BD Horizon; BD Biosciences). Surface staining was followed by red blood cell lysis with BD Pharm Lyse (BD Biosciences) for 3 min at 37°C and centrifugation for 5 min at 350 g. Cells were washed twice with cell staining buffer and analysed by flow cytometry. Unlabeled cells were used as controls; nonspecific fluorescence signals due to spectral overlap were automatically compensated.

Data acquisition was performed on MoFlo Astrios EQ cell sorter with Summit software (Beckman Coulter, Brea, CA, USA). Data analysis (blood and spleen suspensions samples) was performed using FlowJo v.10 software (TreeStar; BD Biosciences), with CD3ε+ lymphocytes gated as CD4+CD8a− and CD4−CD8a+ populations, and CD3ε− lymphocytes as CD19+NK1.1− and CD19−NK1.1+ populations. The expression of CD3ε, CD4, CD8a, CD19 and NK1.1 from skin samples was evaluated using Overton Subtraction performed with FlowJo v.10 software (TreeStar; BD Biosciences).

Statistical analysis

Data were analysed using Microsoft Excel (Microsoft, Redmond, CA, USA). The results were expressed as mean ± SD. For skin samples, the expression of fluorescence levels was evaluated using Overton Subtraction technique performed with FlowJo v.10 software (TreeStar; BD Biosciences). The results were expressed as mean ± SD calculated using the Overton Subtraction method. For statistical analysis, Student's t-test (two-tailed, assuming equal variance) was used to assess the differences between the experimental groups. P-values <0.05 were considered to indicate a statistically significant difference.

Results

Psoriasiform dermatitis experimental model

In order to assess whether topical IMQ application leads to psoriasis-specific skin lesions, we applied a daily topical dose of Aldara cream on the shaved back skin of 10 C57BL/6 mice for 5 consecutive days. For control, a group of 10 C57BL/6 mice were treated similarly with a vaseline-based cream.

The progress and the severity of the inflammation of the back skin were monitored daily for both groups of mice by scoring of erythema, desquamation and induration parameters, on a scale from 0 to 4: 0, None; 1, slight; 2, moderate; 3, marked; 4, very marked. Erythema was first observed in IMQ-treated mice on day 2; skin scaling and thickening became visible from day 3. Starting from day three, the inflammation of the skin became visible and continued to increase until the end of experiment. Mice treated with vaseline-based cream did not show any sign of inflammation. The independent scores for each parameter (erythema, skin scaling and thickening) and for each experimental group are presented in Fig. 1.

Figure 1. In vivo measurement-scoring for erythema, skin scaling and thickening; PASI cumulative score. C57BL/6 mice (test group) were treated daily with a topical dose of Aldara cream on the shaved back skin for 5 consecutive days. A control group was treated similarly with a vaseline-based cream. Erythema (A), skin scaling (B) and thickening (C) were scored daily (scale 0–4) and the cumulative PASI score (erythema plus skin scaling plus thickening) (D) was calculated daily for each group (test and control). The results are presented as mean ± SD (n=10 for each test and control group).

A modified PASI score was calculated as a cumulative score, including erythema, scaling and thickening scores, for each mouse from both groups, on a range from 0 to 12 for each day of experiment (Fig. 1A-C). The PASI score had a progressive evolution for IMQ-treated mice, reaching at the end of the experiment a value close to maximum (Fig. 1D).

At day 6 the experimental spleens from all the animals were weighed and splenomegaly was assessed by calculating the SW:BW ratio. For IMQ-treated mice the spleen weight was significantly higher compared to the vaseline-treated mouse group (0.23±0.04 vs. 0.09±0.04; P<10−5) (Fig. 2A). The measurements showed that for IMQ-treated mice the spleen weight and the ratio SW/BW is 2.5 times, respectively 3 times greater than in vaseline-treated mice (0.0114±0.003 vs. 0.0036±0.001; P<10−5) (Fig. 2B).

Figure 2. Splenomegaly assessment. C57BL/6 mice (test and control group) were weighed and sacrificed for spleens sampling. The spleens were weighed separately (A) and the ratio of the weight of the spleen (SW) and bodyweight (BW) was calculated (B). The results are presented as mean spleen weight ± SD, respectively mean ratio SW:BW ± SD (n=10 for each test and control group).

Skin inflammation and the disease severity were histopathologically assessed. After 6 days, skin samples from each experimental group (test, normal and control) were harvested for histopathologic evaluation. IMQ treatment induced hyperkeratosis, parakeratosis, acanthosis and elongation of rete ridges (histopathological features that are typical assessed in human psoriatic skin samples) (Fig. 3C and D). None of these histopathological findings were observed in control (vaseline)and normal group (Fig. 3A and B).

Figure 3. H&E staining of skin samples harvested from dorsal area. (A) Normal mouse; (B) Vaseline-based cream treated mouse; (C and D) IMQ-treated mouse. (C and D) Histopathologic evaluation of the skin samples from IMQ-treated mice revealed hyperkeratosis, parakeratosis, acanthosis and elongation of rete ridges. (A and B) None of these histopathological findings were observed in control and normal group skin samples.

Lymphocyte distribution in peripheral blood and spleen samples

To evaluate the immune cell pattern of the tested experimental model blood and spleen suspensions were assessed from all the groups analysed for T, B and NK cells population components by flow cytometry. Data analysis was performed using FlowJo v.10 software (TreeStar; BD Biosciences), with CD3ε+ lymphocytes gated as CD4+CD8a− and CD4−CD8a+ populations, and CD3ε− lymphocytes as CD19+NK1.1− and CD19−NK1.1+ populations. Unlabeled cells were used as controls; non-specific fluorescence signals due to spectral overlap were automatically compensated. Data were analysed using Microsoft Excel (Microsoft). The results were expressed as a percentage from the CD3+ lymphocytes (mean ± SD) (Fig. 4).

Figure 4. Distribution of lymphocyte populations in peripheral blood. (A) Percentage distribution of T-CD4+ and T-CD8a+ lymphocytes in IMQ-treated mice (50±3, *P<10−5 and 45±2, **P<0.0005) as compared to control (vaseline) (58±3 and 39±3) and normal group (57±3 and 40±4). (B) Percentage distribution of CD19+ lymphocytes and NK1.1+ cells in IMQ-treated mice (43±14, *P<10−6 and 8±3, **P<0.05) as compared to control (vaseline) (77±5 and 5±1) and normal group (85±2 and 4±1). (C) Distribution of T-CD4+/T-CD8+ ratio in IMQ-treated mice (1.13±0.11, P<0.0005) as compared to control (vaseline) (1.48±0.18) and normal group (1.46±0.25). The results are presented as a percentage from CD3ε+ lymphocytes (mean ± SD).

In comparison to vaseline-treated mice and the normal group we noted in the IMQ-treated mice peripheral blood percentages of T-CD4+ and B lymphocytes decreased significantly while the percentages of T-CD8a+ lymphocytes and NK1.1+ cells increased (Fig. 4A and B). The values obtained for the control groups (mice treated with vaseline-based cream and normal mice) are similar and the differences are not statistically significant. T-CD4+/T-CD8a+ ratio is lower in mice treated with IMQ compared to control groups and the differences between experimental groups are highly statistically significant (P<0.0005) (Fig. 4C).

To further investigate the immune cell pattern in the main lymphoid organ, we investigated immune cell populations in the spleen suspensions. The main change observed in spleen suspensions was the significant decrease of B cells percentages in IMQ-treated mice (35±11; P<10−6) compared to vaseline-treated mice (75±12) and normal group (81±5) (Fig. 5B). Other lymphocyte populations and subpopulations showed the same tendency of variation as in peripheral blood, but without statistical significance (Fig. 5A and B). T-CD4+/T-CD8a+ ratio is lower in mice treated with IMQ compared to control (vaseline) groups, but the differences are not statistically significant (Fig. 5C). The values obtained for the control (vaseline) groups (mice treated with vaseline-based cream and normal mice) were similar.

Figure 5. Distribution of lymphocyte populations in spleen. (A) Percentage distribution of T-CD4+ and T-CD8a+ lymphocytes in IMQ-treated mice (53±4 and 39±4) as compared to control (vaseline) (56±3 and 37±1) and normal group (56±4 and 38±4). (B) Percentage distribution of CD19+ lymphocytes and NK1.1+ cells in IMQ-treated mice (35±11, P<10−6 and 7±4) as compared to control (vaseline) (75±12 and 7±2) and normal group (81±5 and 6±2). (C) Distribution of T-CD4+/T-CD8+ ratio in IMQ-treated mice (1.37±0.0.26) as compared to control (vaseline) (1.51±0.12) and normal group (1.52±0.23). The results are presented as percentage from CD3ε+ lymphocytes (mean ± SD).

Analysis of fluorescence levels in skin samples

As skin is the main target tissue of the psoriatic mouse model, the effect of the IMQ treatment on CD3ε+, CD4+, CD8a+, CD19+ and NK1.1+ cell populations in skin was assessed by flow cytometry. Analysis of lymphocyte populations in skin samples revealed a continuous fluorescence level which made impossible to gate positive and negative events. To highlight the differences between the fluorescence levels (stained vs. unstained samples) Overton subtraction was chosen and an increased value for Overton subtraction indicated a high level of fluorescence (Fig. 6).

Figure 6. Analysis of fluorescence levels using Overton subtraction. An example of fluorescence data analysis; blue, unstained control; white, stained sample.

Raised values of Overton subtraction were obtained for CD3ε+ and CD4+ cells from skin samples of both IMQ and vaseline-treated mice, indicating a high level of fluorescence for these labelled cells. The differences between Overton subtraction values for experimental groups (IMQ-treated mice vs. vaseline-treated mice) were statistically significant for CD3ε+ (93±6 vs. 70±23; P<0.05), CD4+ (90±4 vs. 73±22; P<0.05) and CD8a+ cells (40±21 vs. 20±14; P<0.05) (Fig. 7).

Figure 7. Immune cell pattern in skin samples. Expression of differences between mean Overton subtraction values in IMQ and vaseline-treated mice: CD3ε+ cells (93±6 vs. 70±23, *P<0.05); CD4+ cells (90±4 vs. 73±22, *P<0.05); CD8a+ cells (40±21 vs. 20±14, *P<0.05); CD19+ cells (11±8 vs. 6±4); NK1.1+ cells (55±17 vs. 41±23). The results are presented as mean ± SD.

Discussion

Although there is an important imaging panel for investigating human disease (36–38), the need to find immunological pattern of this autoimmune disorders remains a constant issue. The studies related to the psoriatic animal model do not abound and comprise merely few dozen published papers. There have been attempts to establish a psoriatic-like mouse model, such as induction in immunodeficient (SCID) mice of psoriasiform lesions using staphylococcal enterotoxin B (SEB)-stimulated PBMCs (SEB-PBMCs) isolated from psoriatic patients as transplantation mouse psoriasis model. Another group transplanted in SCID mice skin harvested from psoriatic patients and afterwards both intradermal and intraperitoneal inoculations of bacterial superantigen was performed inducing a mouse model of psoriasis (39,40). All these prior models were accompanied by technical difficulties including lack of reproducibility when human patient samples were transplanted. The first report on topical application of Aldara cream inducing an animal model of psoriatic lesion was published in 2009 (35) and continued in 2014 (41). In these reports the focused evaluations were performed mainly on the tissue pattern of inflammatory cells. In the monitoring domain of psoriasis evaluating both the circulatory and skin immune cells are equally important to further developing immune patterns that can monitor disease evolution and therapy efficacy.

We chose the murine model of psoriasiform dermatitis induced by topical IMQ application according to the prior described protocols (35) to further evaluate the immunological changes in lymphocyte populations from peripheral blood and spleen, and to estimate the amplitude of the cellular changes linked to the pathogenic mechanism. To our knowledge there are no similar studies regarding the immune cell characterization in blood, spleen and skin regarding IMQ experimental model. The on-site lesion echo of central changes was appreciated at the cell population level in lesioned tissue.

The immunological changes induced by IMQ treatment in lymphocyte populations from peripheral blood and spleen were evaluated by flow cytometry. The main changes observed in peripheral blood were the significantly increased of T-CD8a+ lymphocytes and NK1.1+ cell percentages and the decreased of T-CD4+ and B-CD19+ lymphocyte percentages in IMQ-treated mice compared to control (vaseline) groups. As a consequence of the alteration of lymphocyte subpopulation distribution, the T-CD4+/T-CD8a+ ratio is lower in mice treated with IMQ compared to control (vaseline) groups.

The increased percentage of T-CD8 lymphocytes in the peripheral circulation could suggest a cytotoxic mechanism at lesion level. At the origin of the auto-maintenance process in psoriasis are autoantigens and nucleic acids released by damaged epidermal cells (keratinocytes) that activate plasmacytoid dendritic cells. Recent studies show an abundance of proteins in the psoriatic skin mouse model that can account for the self-maintained auto-antigenic pool (42). The role of T-CD8 lymphocytes could be to recognize autoantigens and further destroy keratinocytes whose activation products are part of the auto-maintenance cycle of the disease. The interesting finding of peripheral NK cell increment associated with a decreased B lymphocyte percentage matches our prior reported results in other skin diseases (43) accounting for still unknown immune mechanisms of compensation between two types of immune cells.

In spleen samples, lymphocyte populations and subpopulations showed the same tendency of variation as in peripheral blood, but without statistical significance. The main change observed in spleen suspensions was the significant decrease of B cell percentages in the IMQ-treated mice compared to vaseline-treated mice and normal group. Decreased percentages of B lymphocytes in peripheral blood and spleen may suggest a general decrease in B lymphocytes as a result of a medullary dysfunction. It may also be possible for B lymphocytes to be arrested in certain lymphoid organs (e.g., lymph nodes) and/or digestive system, and subcutaneous tissues. As we found only a low expression of CD19+ cells in skin samples, it seems less likely B cells to be arrested at this level.

The values obtained for T-CD4+ lymphocyte percentages are low, both in peripheral blood and spleen suspensions. This may be due to the change in the proportion of Th subpopulations, but the results we have obtained so far do not allow us to pinpoint the cause of this decrease. The finding can be explained by an induced defective development of T-CD4+ subpopulations with regulatory functions, immune cells that can contribute to the pathogenesis of psoriasis and/or other autoimmune diseases (44,45).

Analysis of lymphocyte populations in skin samples revealed raised values of Overton subtraction for CD3ε+ and CD4+ cells (for both IMQ and vaseline-treated mice), and the differences between Overton subtraction values for experimental groups were statistically significant for CD3ε+, CD4+ and CD8a+ cells. These results may suggest the involvement of these cells in the lesional process. Moreover, as recently reported in the skin of mice exposed to IMQ a subset of IL-17-producing γδ T cells are endowed with long-lived memory (45,46) thus we cannot exclude that there are several other immune subpopulations that contribute to the increased percentage of cells depicted by us in this model.

In conclusion, imiquimod-based murine model of psoriasiform dermatitis was analysed from an immunological point of view by performing a basic cellular profile at three levels: peripheral blood, spleen and skin. Expression of lymphocytes in these three immune areas may be a starting point for the specification of some immunological features of psoriasis with therapeutic utility. The evaluation was intended to establish the immune framework of this experimental model that could be further used for etio-pathogenic mechanisms identification and/or for studies regarding targeted therapies.

Acknowledgements

The present study will be integrated in the original part of PhD thesis of author PhD student Mihaela Surcel.

Funding

This study was supported by Grant PN-III-P1-1.2-PCCDI-2017-0341/2018 and projects PN 18.21.02.01 and PN 18.21.02.02 and financed by Executive Agency for Higher Education, Research, Development and Innovation (Bucharest, Romania).

Availability of data and materials

The data sets used and/or analysed during the present study are available from the corresponding author on reasonable request.

Authors' contributions

RIH, MS, CC, MN and CU contributed to the creation and design of the research, acquisition, analysis and interpretation of the data, statistical analysis, drafting the manuscript, critical revision of the manuscript for important intellectual content. ANM, GI, IRP, DC, OB and CC were responsible for data acquisition, analysis and interpretation of data, and contributed to drafting and revising critically the manuscript for important intellectual content. All the authors read and approved the final version of the manuscript.

Ethics approval and consent to participate

The study protocol was approved by the Ethics Committee of ‘Victor Babeș’ National Institute of Pathology (Bucharest, Romania).

Patient consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Glossary

Abbreviations

Abbreviations:

References