Stem Cells International

Stem Cells International / 2016 / Article
Special Issue

Molecular Imaging of Stems Cells: In Vivo Tracking and Clinical Translation

View this Special Issue

Research Article | Open Access

Volume 2016 |Article ID 3970942 |

Juan Cao, Shike Hou, Hui Ding, Ziquan Liu, Meijuan Song, Xiaojing Qin, Xue Wang, Mengyang Yu, Zhiguang Sun, Jinyang Liu, Shuli Sun, Peixin Xiao, Qi Lv, Haojun Fan, "In Vivo Tracking of Systemically Administered Allogeneic Bone Marrow Mesenchymal Stem Cells in Normal Rats through Bioluminescence Imaging", Stem Cells International, vol. 2016, Article ID 3970942, 11 pages, 2016.

In Vivo Tracking of Systemically Administered Allogeneic Bone Marrow Mesenchymal Stem Cells in Normal Rats through Bioluminescence Imaging

Academic Editor: Ping Wang
Received22 Mar 2016
Revised26 May 2016
Accepted03 Jul 2016
Published17 Aug 2016


Recently, mesenchymal stem cells (MSCs) are increasingly used as a panacea for multiple types of disease short of effective treatment. Dozens of clinical trials published demonstrated strikingly positive therapeutic effects of MSCs. However, as a specific agent, little research has focused on the dynamic distribution of MSCs after in vivo administration. In this study, we track systemically transplanted allogeneic bone marrow mesenchymal stem cells (BMSCs) in normal rats through bioluminescence imaging (BLI) in real time. Ex vivo organ imaging, immunohistochemistry (IHC), and RT-PCR were conducted to verify the histological distribution of BMSCs. Our results showed that BMSCs home to the dorsal skin apart from the lungs and kidneys after tail vein injection and could not be detected 14 days later. Allogeneic BMSCs mainly appeared not at the parenchymatous organs but at the subepidermal connective tissue and adipose tissue in healthy rats. There were no significant MSCs-related adverse effects except for transient decrease in neutrophils. These findings will provide experimental evidences for a better understanding of the biocharacteristics of BMSCs.

1. Introduction

Mesenchymal stem cells (MSCs) are self-renewing, multipotent progenitor cells with the potential to differentiate into multiple mesoderm lineages. Many animal models have demonstrated the remarkable tropic, nonimmunogenic, and immunosuppressive characteristics of these cells in injured tissues [1, 2]. Due to their properties of accessibility and convenient expansion, clinical research on MSCs has increased in the past twenty years. MSCs have been described as a promising source for the cell-based treatment of miscellaneous complicated disorders, such as graft-versus-host disease [3, 4], cardiocerebrovascular disease [5], spinal cord injury [6, 7], hepatic diseases [8], and respiratory disease [9, 10]. Although there is a consensus regarding the in vitro characteristics of MSCs, there are outstanding issues concerning the localization and persistence of MSCs in vivo after administration. Furthermore, the safety of injecting of foreign cells such as these is another major obstacle in the clinical setting.

Bioluminescence imaging (BLI) detects visible light emitted by cells labeled with luminescent enzymes, such as luciferase, when these enzymes react with their specific bioluminescent substrates [11]. BLI can noninvasively track luciferase-transduced cells implanted in living animals in real time. This method of substantial utility has already facilitated the design of therapeutic strategies using MSCs in various animal models, including models of tumorous diseases, ischemia- and reperfusion-induced acute kidney injury (AKI), myocardial damage, stroke, and other diseases [1215]. However, visible light is limited in the depth of tissue penetration. Thus, this technique is mainly used for imaging of small animals, such as mice. Herein, we show that bioluminescent imaging can reveal dynamic information detailing the distribution and tropism of BMSCs in a larger rat model. More interestingly, we revealed that the homing organs of BMSCs in rats are not the same as in mice. Additionally, we carried out a safety assessment of the administered BMSCs through histological and serology tests, providing an experimental basis for the use of these stem cells in research.

2. Material and Methods

2.1. Lentivirus Vector and BMSC Transduction

MSCs were isolated from the bone marrow of normal Wistar rats purchased from Cyagen Biosciences. According to the minimal criteria proposed by the International Society for Cellular Therapy (ISCT) [16], the cells were subjected to flow cytometry to examine the expression of specific surface antigens (Figure  S1 in Supplementary Material available online at The BMSCs displayed a typical MSC morphology, exhibiting a fibroblast-like shape or flat polygonal appearance. They were plastic adherent and were maintained in tissue culture flasks. When the BMSCs were approximately 80 to 90% confluent, they were dissociated with trypsin-EDTA and split at a 1 : 2 ratio.

The culture-expanded BMSCs were seeded in six-well plates at a density of 1 × 105 cells per well. 24 h later, the medium was removed and replaced with growth medium and a polybrene solution (1 mL per well). Polybrene was added at a final concentration of 5 μg/mL. The lentivirus vector expressing both the GFP and luciferase genes (purchased from GENECHEM, Shanghai, China) was thawed and added at a multiplicity of infection of 4. After 8 h of incubation, the medium was replaced with fresh medium, and the flask was returned to the incubator. Three days later, to quantify the transduction efficiency, Luc-GFP-BMSCs were stained with Hoechst 33342 (FANBO, Beijing, China) for 5 min. Then, the cells were visualized and analyzed using an inverted fluorescence microscope (DMI 3000B, Leica, Germany) in five randomly selected fields of view.

2.2. Multilineage Differentiation of Luc-GFP-BMSCs

Cultured-expanded Luc-GFP-BMSCs at passage six were used to evaluate the in vitro differentiation abilities of the cells in accordance with the manufacturer’s recommendations (Cyagen Biosciences, USA). For adipogenic induction, Luc-GFP-BMSCs were subculture-expanded in six-well plates at 2 × 104 cells/cm2 in growth medium containing 10% fetal bovine serum and 5% penicillin-streptomycin as well as glutamine. The cells were fed every three days until they reached 100% confluency. Then, the growth medium was changed to 2 mL of induction medium, which consisted of fetal bovine serum, penicillin-streptomycin, glutamine, insulin, rosiglitazone, and dexamethasone. Three days later, the medium was replaced with maintenance medium containing fetal bovine serum, penicillin-streptomycin, and insulin. 24 h later, the medium was changed back to induction medium, and the cycle of induction/maintenance was repeated three times. After five cycles of induction/maintenance, the cells were cultured in maintenance medium for an additional three days. Three weeks later, adipose cells were observed after being stained with Oil Red O. To induce osteogenic differentiation, Luc-GFP-BMSCs were seeded in growth medium at a density of 3 × 104 cells/cm2 for one day at 37°C in a 5% CO2 humidified incubator. Then, the growth medium was aspirated from each well and 2 mL of osteogenic differentiation medium containing fetal bovine serum, penicillin-streptomycin, glutamine, ascorbate, β-glycerophosphate, and dexamethasone was added, and the medium was changed every three days. Three weeks later, the cells were fixed with 2 mL of a 4% formaldehyde solution and stained with Alizarin red.

2.3. Animals

Adult male Wistar rats weighing  g were provided by the Experimental Animal Center of the Military Medical Science Academy of the People’s Liberation Army of China. The rats were maintained in an animal laboratory under a temperature of 25°C at all times, fed with commercial rodent chow and given free access to water, and were allowed to acclimate for one week. All animals received humane care in compliance with the Guide for the Care and Use of Laboratory Animals published by the National Institutes of Health. The study protocol was approved by the Laboratory Animal Ethics Committee of the Affiliated Hospital of the Logistical College of the Chinese People’s Armed Police Forces.

2.4. In Vitro Imaging

To assess the luciferase expression of the transduced BMSCs, different numbers of Luc-GFP-BMSCs (0.1, 0.2, 0.3, 0.4, and 0.5 × 104/well) were seeded into a 96-well plate in 100 μL of growth medium, and D-luciferin solution (D-luciferin, 150 μg/mL, Gold Biotechnology, Inc., USA) was added at room temperature. After 10 min of incubation, the cells were imaged using an in vivo imaging system (IVIS) (PerkinElmer, IVISSPE, USA). The bioluminescent signals were analyzed using Living Image Software 4.5.

2.5. In Vivo Imaging of Luc-GFP-BMSCs

Luc-GFP-BMSCs (2 × 106) suspended in 1 mL of phosphate-buffered saline (PBS) were injected into the tail vein of rats, and this group was labeled the Luc-GFP-BMSC transplantation group (Luc-GFP-BMSCs group, ). Phosphate-buffered saline alone was used as a control. For the in vivo imaging of aim cells, rats were anesthetized with 2% pentobarbital sodium (50 mg/kg) and injected intraperitoneally with D-luciferin (150 mg/kg body weight) 10 min before imaging. Then, the animals were placed in the imaging chamber. In vivo BLI was performed at 1.5, 2.5, 18, and 22 h and 1, 2, 3, 7, 10, 14, and 30 days after Luc-GFP-BMSC injection. Regions of interest (ROIs) were drawn manually using Living Image 4.5 Software (Caliper Life Sciences) to evaluate the relative signal intensity emitted. The photon radiance of the experimental animals was expressed as photons per second per centimeter squared per steradian within the ROIs. The animals were imaged over a period of one month, after which they were sacrificed, and their tissues were harvested for PCR and IHC analyses.

To locate cell homing visually, four days after injection, immediately after acquiring photographic images in vivo, five animals were sacrificed. The skin of the back, the vertebral column, and other organs were removed and placed in Petri dishes. BLI of the tissues was carried to identify the Luc-GFP-BMSCs. Then, tissues showing BLI signals were fixed in 4% paraformaldehyde for further IHC analysis.

2.6. Immunohistochemistry

To verify the histological distribution of Luc-GFP-BMSCs after transplantation, tissues fixed in 4% paraformaldehyde were dehydrated and embedded in paraffin. Paraffin-embedded sections of 5 μm were prepared on poly-L-lysine-coated slides according to standard protocols. The slides were incubated with an anti-GFP antibody (Abcam, London, England) diluted 1 : 50 in PBS overnight at 4°C. For primary antibody detection, a mouse immunohistochemistry (ABC) kit (ZSGB-BIO, Beijing, China) was used. The sections were stained with a DAB kit. Counterstaining was performed with hematoxylin. GFP-positive cells were then counted under a light microscope in six high-power fields in three sections and scored based on whether they were tissue associated.

Furthermore, we detected GFP-positive cells in tissues via IHC to verify the advanced histological distribution of Luc-GFP-BMSCs at one day after transplantation.

2.7. RT-PCR

Total RNA for PCR was extracted with an RNeasy kit (Solarbio Science & Technology, Beijing, China), including a DNase digestion step to exclude contaminating DNA. Reverse transcription was performed using a Quant Script kit (TIANGEN BIOTECH, Beijing, China) for 1 h at 37°C. The primer sequences for the target gene were as follows: firefly luciferase-F: ACTGGGACGAAGACGAACAC and firefly luciferase-R: GGCGACGTAATCCACGATCT. PCR was carried out for the relative quantification of target gene copy numbers in relation to the β-actin transcript.

2.8. Blood Sampling

To examine the systemic response to wild-type BMSC transplantation, blood was collected from the inferior vena cava of anaesthetized rats at one day (1-day group; ), four days (4-day group; ), or one month (1-month group; ) after the transplantation of wild-type BMSCs. The control group, which was injected only with PBS (control group; ), was examined as well. The serum concentrations of blood urea nitrogen (BUN), creatinine (Cr), aspartate transaminase (AST), and alanine transaminase (ALT) were determined using automatic dry chemical analysis methods (VITROS 5600 Integrated System, Johnson, America). Routine blood test measurements were conducted with an automatic hematology analyzer (SYSMEX XN-1000, Japan).

2.9. Histopathology Evaluation

Tissue samples collected from the 1-day, 4-day, and 1-month groups were fixed in 10% formalin and subsequently embedded in paraffin following standard methods. Sections with a thickness of 5 μm were cut and mounted on glass slides and then deparaffinized. Finally, the slides were stained with hematoxylin and eosin (H&E). The slides were relabeled using Arabic numbers, followed by double-blinded examination by two pathologists.

2.10. Statistical Analysis

All of the presented data are expressed as the mean ± standard deviation (SD). Statistical analyses were performed using SPSS version 22.0. Differences between different groups were examined using Student’s -test or analysis of variance. values < 0.05 were considered significant.

3. Results

3.1. Transduction of BMSCs

BMSCs were incubated in six-well plates at 1 × 105 cells/well for 24 h, following infection with 4 × 105 Lenti-Luc-GFP-lentivirus particles (MOI = 4). After 3 days of incubation, the transduction efficiency was approximately 76.45%, as evaluated under a fluorescence microscope (Figure 1(a)). There was no difference between the transduced BMSCs and wild-type BMSCs in terms of morphology. The expression of GFP was stable for at least 60 days under constant culture conditions.

3.2. In Vitro Characterization of the Pluripotential Capacity

To confirm the multilineage differentiation capacity of the Luc-GFP-BMSCs, the ability of Luc-GFP-BMSCs to differentiate into cells showing adipogenic and osteopenia patterns was investigated. Luc-GFP-BMSCs at passage 6 could differentiate into both adipocytes, as demonstrated by Oil Red O staining (Figure 1(b)), and osteoblasts, as assessed via Alizarin red staining (Figure 1(c)). Moreover, the differentiated cells still stably express GFP (Figures 1(b) and 1(c)).

3.3. In Vitro Imaging

The activity of luciferase was assessed through bioluminescence imaging (BLI) (Figure 1(d)). As shown in Figure 1(e), the imaging of different numbers of cells in vitro revealed a linear correlation between the BLI signal and cell numbers (), indicating that the reporter gene could be used for tracking and quantifying the transplanted BMSCs in small living animals.

3.4. Dynamic Distribution of BMSCs Monitored with an IVIS after Systemic Administration in Normal Rats

Next, we infused Luc-GFP-BMSCs into normal Wistar rats via tail vein injection and then dynamically monitored the bioluminescence imaging of luciferase activity with an IVIS in the following month. As shown in Figure 2, the BLI image results revealed that BMSCs delivered to fully immunocompetent allogeneic hosts predominantly resided in the lungs and lower back areas (Figures 2(a) and 2(c)). The BLI signals in the lung decreased over time and were absent at three days after injection in vivo. By imaging in both supine and prone positions, we found that the BMSCs migrated to the lower back after tail vein injection. There were two peaks of BLI signals observed in the lower back, at 24 h and seven days after vein injection. The imaging signals decreased over time and were completely absent 14 days after transplantation (Figures 2(b) and 2(d)). One month later, we still failed to find any signals in the animals.

3.5. Histological Distributions of the Transplanted BMSCs

To evaluate the distribution of Luc-GFP-BMSCs in different organs after injection, we injected the rats with D-luciferase intraperitoneally and isolated various rat organs, including the lungs, kidneys, heart, intestines, liver, skin of the lower back, spine, and spleen at four days after vein injection of Luc-GFP-BMSCs. The BLI signals were assessed in these organs, and the results showed that positive signals were detectable in the lungs, kidneys, and skin of the backs of normal rats (Figures 3(a) and 3(b)).

Furthermore, we detected GFP-positive cells in organs exhibiting BLI signals via immunohistochemistry to verify the advanced histological distribution of Luc-GFP-BMSCs. IHC was performed on the lung, kidney, and dorsal skin tissues. At one day after transplantation of Luc-GFP-BMSCs, GFP-positive cells were found in the conjunctive area between the blood vessels and alveoli. Although there were still BLI signals detected in isolated lungs at four days after injection, the IHC results showed that the positive cells were mainly located in the connective tissue and adipose tissue of the hilus pulmonis, but not the lungs (Figure 3(c)). Similarly, BMSCs were located in the connective tissue and adipose tissue of the renal hilum, but not the renal parenchyma. In the skin tissue, GFP-positive cells mainly appeared in the subepidermal connective tissue as well as the adipose tissue (Figure 3(c)). Consistent with the BLI results, the greatest number of GFP-positive cells was found in the lungs at one day after injection (Figure 3(d)), and four days later, the number of GFP-positive cells in the dorsal skin was greater than in other organs (Figure 3(e)). RT-PCR results also verified the presence of Luc-GFP-BMSCs in the above organ tissues: lung, kidney, and skin (Figure 3(f)). Furthermore, consistent with in vivo imaging result, BMSC colonization of specific organs was not found by RT-PCR and IHC detection (Figures 4(a) and 4(b)).

3.6. Safety Evaluation

No death occurred in the experimental groups, and clinical signs of dyspnea did not appear throughout the experiment. The morphometric analyses failed to detect any tumors or neoplasms in all animals. HE staining demonstrated that there was no dysplasia in MSC homing organs in the 1-day, 4-day, and 1-month groups (Figure 5). Moreover, as shown in Table 1, there was no significant difference in the biological markers of the kidney and liver () between the experimental groups and the control. Routine blood tests verified a reduction in the white cell count, especially for neutrophils (), resulting in a relative increase in the percentage of lymphocytes () in the 4-day group compared with the control. However, one month later, the neutrophil count had returned to normal and was not significantly different than in the control (Table 2).


WBC (109/L)10.19 ± 3.426.95 ± 1.138.12 ± 1.817.49 ± 1.82
RBC (1012/L)7.10 ± 0.856.57 ± 0.376.77 ± 0.207.43 ± 0.25
PLT (109/L)1020.50 ± 165.04942 ± 133.951049.00 ± 83.606936.17 ± 123.89
LYMPH (109/L)7.68 ± 2.405.55 ± 0.896.96 ± 1.515.80 ± 1.67
NEUT (109/L)2.02 ± 0.961.20 ± 0.280.97 ± 0.271.39 ± 0.25
LYMPH%76.18 ± 5.2079.98 ± 2.0485.80 ± 2.5076.87 ± 4.51

Control: animals injected with PBS only; 1-day: animals examined 1 day after transplantation of BMSCs (2 × 106); 4-day: animals examined 4 days after transplantation of BMSCs (2 × 106); 1-month: animals examined 1 month after transplantation of BMSCs (2 × 106).
Results are shown as the mean ± SD ().
versus control.


AST (U/L)106.5 ± 22.28124.60 ± 10.69105.67 ± 18.4699.17 ± 19.19
ALT (U/L)34.00 ± 8.6038.60 ± 5.1834.50 ± 3.6231.17 ± 4.12
Cr (mol/L)30.67 ± 6.0227.21 ± 3.5629.67 ± 2.5231.00 ± 2.37
BUN (mmol/L)5.55 ± 0.494.76 ± 1.085.43 ± 0.705.38 ± 0.89

Control: animals injected with PBS only; 1-day: animals examined 1 day after transplantation of BMSCs (2 × 106); 4-day: animals examined 4 days after transplantation of BMSCs (2 × 106); 1-month: animals examined 1 month after transplantation of BMSCs (2 × 106).
Results are shown as the mean ± SD ().

4. Discussion

Cell therapies are currently expected to provide cures for a wide variety of diseases as short effective routine therapies in clinical settings [17]. In clinical practice, in terms of the immune reaction, the perfect donor cells would be autologous [13]. However, autologous cells have obvious shortcomings. For example, in patients with diseases of the blood or immune system, their own cells are unsuitable for application. Due to showing low expression of immune antigens, allogeneic MSCs are an attractive cell resource for various complicated and refractory diseases [18]. The present study employed allogeneic cells, and we choose intravenous injection as the transplantation route to closely imitate clinical settings, as this route is commonly used in humans.

There is controversy about the homing feature of systemically administered BMSCs. The fate of BMSCs in living animals is related to many factors, such as their origins, the number of cells, and delivery routes. Tracking studies have demonstrated that transplanted human or allergenic BMSCs initially reside in the lungs and then egress to the liver and spleen in SCID mice [19, 20]. Eggenhofer et al. found that allergenic mouse BMSCs did not migrate beyond the lungs after intravenous infusion [21]. The differences in the distribution of BMSCs among these studies might be related to the origins of the cells, the host animal type, and the applied detection methods. Unlike the above studies, we injected allergenic BMSCs into normal rats (a larger animal subject). Our results showed that the majority of BMSCs localized to the lungs, kidneys, and loose connective tissue under the epithelia of the back after tail vein injection. In accordance with previous studies, a large number of IV-injected BMSCs were trapped within the first filtering organ rich in capillaries because the mean size of the suspended BMSCs is larger than that of capillaries [22]. In this work, we found that the BMSCs were inclined to undergo passive clustering after systemic infusion in the lungs and kidneys, but homing to the epithelia of the back may be an active phenomenon. BMSCs are not circulating cells, which must attach to the extracellular matrix for survival and growth. Accordingly, when such cells are disaffiliated from this context, they may be tracked using certain extracellular matrix-derived signals for survival. Regarding their secondary distribution, BMSCs mainly concentrate in loose connective tissue and adipose tissue under the epithelia. Even in the lungs and kidneys, they did not appear in the parenchyma, but in the connective tissue and adipose tissue of the hilus pulmonis and renal hilum at 4 days after injection.

By view from both supine and prone position, we firstly found that the dorsal skin is another organ attracting MSCs. IHC test showed that Luc-GFP-BMSCs locate in the loose connective tissue of the dorsal skin. Considering that BMSCs can easily differentiate into adipocytes in vitro, we hypothesize that the administered BMSCs are drawn by signals from the extracellular matrix of adipocytes and that the loose connective tissue is convenient for BMSCs to move through and proliferate. Different from the muscular tissue (heart and skeletal muscle), loose connective tissues have more space which may be suitable for the residing of MSCs. Moreover, dermal fibroblast secretes stromal cell-derived factor-1, a key chemokine which recruits circulating MSCs through the SDF-1α/CXCR4 pathway [23, 24]. As to the reason of BMSCs’ selective recruitment to dorsal skin, we cannot give an exact explanation, which may need further research to answer this phenomenon in our following studies.

Previously, it was believed that MSCs repair damaged tissues through a transdifferentiation mechanism [25], and targeted delivery routes of the cells to injured organs would therefore be essential for effective therapy. These cells are also typically regarded as one of the notable landmarks in the progress of all forms of cell therapies. To cause greater numbers of MSCs to concentrate in injured tissues, researchers have attempted diverse injection strategies, leading to the detainment of MSCs in other target filtering organs. However, persistent engraftment and differentiation of implanted MSCs in vivo have rarely been detected. Many investigators have found that transplanted MSCs show short survival in vivo, and they exert a considerable influence on diseases that do not depend on the number of cells homing to the targeted organ [26, 27]. The life of transplanted MSCs in vivo is too short to explain the significant functional improvement of infarcted organs by differentiation. Thus, the routes for MSC administration do not appear to be as important in clinical applications. Thus, intravenous administration may be sufficient.

Our data from follow-up studies of transplanted BMSC survival using BLI demonstrated that BMSCs cannot survive for a long period. These results are similar to those of previous studies. There are three possible explanations for the observed localization of the administered BMSCs. (1) Mesenchymal cell adhesion to the extracellular matrix generates tensional integrity, which is a physiological cellular process that is necessary for cell differentiation, survival, and growth. In contrast, after administration and suspension in blood, MSCs lose their cell/matrix interactions, which will induce programmed death. This type of apoptosis is known as anoikis [28]. We believe that anoikis likely plays an important role in the disappearance of MSCs in this context because MSCs are not circulating cells and require extracellular matrix-derived signals for survival, and the deprivation of these signals in the vasculature might induce anoikis. (2) In the present study, we employed immunocompetent rats without the application of immunosuppressive agents during the whole experiment. The innate immune system, which is responsible for the removal of transplanted cells, may be activated by allogeneic MSCs. Some researchers believed that MSCs would not induce an immune response by themselves, but fetal bovine serum (FBS), which is widely used in cell culture and cannot be removed using phosphate-buffered saline, stimulates immunogenicity [29]. In a clinical setting, to avoid such risks, the adoption of autologous serum should be considered, as it has been found that autologous human serum results in more rapid expansion of MSCs [30]. (3) The kidney is a metabolic organ with abundant blood flow. It is known that the excretion of many drugs is closely related to renal function. Our data showed that BMSCs migrated to the kidneys and then disappeared from this organ. Another study [31] provided direct evidence that 1% of BMSCs that were present in the glomerular and peritubular capillaries were TUNEL positive. Together, these findings suggest that this process may contribute to the declining number of BMSCs after administration. Continued attrition of the very small number of cells eventually results in the disappearance of all cells. However, in this work, instead of the glomerular capillaries, we discovered BMSCs in the loose connective tissue around the peritubular capillaries. It is unknown if such a situation occurs occasionally or is related to different sampling times. Perhaps the kidney represents a secondary route of metabolism, but not the major one. Thus, larger, randomized, placebo-controlled preclinical animal trials need to be carried out to address the question of where MSCs are going.

The present study also investigated the short- and middle-term safety of allogeneic BMSC transplantation. Unlike pharmaceutical drugs, we are unable to produce MSCs in complete compliance with the relevant regulations in the laboratory [32]. However, we made all possible attempts to avoid potential adverse events after BMSC transplantation, such as bacteriological contamination, using a cell incubation period of less than 60 days and not exceeding 10 passages in culture. The experimental groups were followed up after one day, four days, and one month, and all animals exhibited an absence of tumorigenesis and injured tissues. Histological analysis of the experimental groups showed that all animals did not display any hyperplasia or tissue inflammation. There was no significant difference between the experimental groups and the control in terms of biological markers of the kidney and liver. Although infused MSCs were found to cause a reduction in neutrophils count at 4 days after injection, the sample sizes are too small to reach a definitive conclusion about whether allogeneic BMSC transplantation causes the white cell count to decrease. However, we think that care should be taken because of the observed phenomenon, and statistical analyses of large samples of blood cell count data associated with MSC-based therapies will be needed for future evaluations of long-term safety.

In summary, our results demonstrate that systemically administered BMSCs in healthy rats are short-lived and mainly migrate to the lungs, kidneys, and the skin of the lower back. Interestingly, in histological analysis, the BMSCs show lipophilicity. They collect in the adipose tissue, and a small number are located in the loose connective tissue around the blood vessels of the hilus pulmonis and renal hilum. The reasons for this distribution pattern are not fully understood. Safety assessment failed to detect any adverse effects in the animals over a short period. Thus, BMSCs may be an ideal candidate for cell-based therapy in preclinical animal studies and, subsequently, for clinical trials, but long-term follow-up safety assessments are needed.

Competing Interests

The authors declare that they have no competing interests.


This research was supported by the National Natural Science Foundation of China (81202105, 71533008) and the Tianjin Science and Technology Project (14ZCDZSY00033, 15JCYBJC28500, and 13JCQNJC12900-2013).

Supplementary Materials

The marker expression of the BMSCs was analyzed by flow cytometry. The mesenchymal stromal cells expressed not hematopoietic markers but the well-known MSC markers.

  1. Supplementary Material


  1. B. J. Jones and S. J. McTaggart, “Immunosuppression by mesenchymal stromal cells: from culture to clinic,” Experimental Hematology, vol. 36, no. 6, pp. 733–741, 2008. View at: Publisher Site | Google Scholar
  2. M. R. Reagan and D. L. Kaplan, “Concise review: mesenchymal stem cell tumor-homing: detection methods in disease model systems,” Stem Cells, vol. 29, no. 6, pp. 920–927, 2011. View at: Publisher Site | Google Scholar
  3. I. B. Resnick, C. Barkats, M. Y. Shapira et al., “Treatment of severe steroid resistant acute GVHD with mesenchymal stromal cells (MSC),” American Journal of Blood Research, vol. 3, no. 3, pp. 225–238, 2013. View at: Google Scholar
  4. M. Introna, G. Lucchini, E. Dander et al., “Treatment of graft versus host disease with mesenchymal stromal cells: a phase I study on 40 adult and pediatric patients,” Biology of Blood and Marrow Transplantation, vol. 20, no. 3, pp. 375–381, 2014. View at: Publisher Site | Google Scholar
  5. J. Bartunek, A. Behfar, D. Dolatabadi et al., “Cardiopoietic stem cell therapy in heart failure: the C-CURE (Cardiopoietic stem Cell therapy in heart failURE) multicenter randomized trial with lineage-specified biologics,” Journal of the American College of Cardiology, vol. 61, no. 23, pp. 2329–2338, 2013. View at: Publisher Site | Google Scholar
  6. S. Karamouzian, S. N. Nematollahi-Mahani, N. Nakhaee, and H. Eskandary, “Clinical safety and primary efficacy of bone marrow mesenchymal cell transplantation in subacute spinal cord injured patients,” Clinical Neurology and Neurosurgery, vol. 114, no. 7, pp. 935–939, 2012. View at: Publisher Site | Google Scholar
  7. S. Forostyak, P. Jendelova, and E. Sykova, “The role of mesenchymal stromal cells in spinal cord injury, regenerative medicine and possible clinical applications,” Biochimie, vol. 95, no. 12, pp. 2257–2270, 2013. View at: Publisher Site | Google Scholar
  8. M.-E. M. Amer, S. Z. El-Sayed, W. A. El-Kheir et al., “Clinical and laboratory evaluation of patients with end-stage liver cell failure injected with bone marrow-derived hepatocyte-like cells,” European Journal of Gastroenterology and Hepatology, vol. 23, no. 10, pp. 936–941, 2011. View at: Publisher Site | Google Scholar
  9. A. Skrahin, R. K. Ahmed, G. Ferrara et al., “Autologous mesenchymal stromal cell infusion as adjunct treatment in patients with multidrug and extensively drug-resistant tuberculosis: an open-label phase 1 safety trial,” The Lancet Respiratory Medicine, vol. 2, no. 2, pp. 108–122, 2014. View at: Publisher Site | Google Scholar
  10. J. G. Wilson, K. D. Liu, H. Zhuo et al., “Mesenchymal stem (stromal) cells for treatment of ARDS: a phase 1 clinical trial,” The Lancet Respiratory Medicine, vol. 3, no. 1, pp. 24–32, 2015. View at: Publisher Site | Google Scholar
  11. J. R. D. Wet, K. V. Wood, D. R. Helinski, and M. DeLuca, “Cloning of firefly luciferase cDNA and the expression of active luciferase in Escherichia coli,” Proceedings of the National Academy of Sciences of the United States of America, vol. 82, no. 23, pp. 7870–7873, 1985. View at: Publisher Site | Google Scholar
  12. K.-S. Jang, K.-S. Lee, S.-H. Yang, and S.-S. Jeun, “In vivo tracking of transplanted bone marrow-derived mesenchymal stem cells in a murine model of stroke by bioluminescence imaging,” Journal of Korean Neurosurgical Society, vol. 48, no. 5, pp. 391–398, 2010. View at: Publisher Site | Google Scholar
  13. C. Xia and J. Cao, “Imaging the survival and utility of pre-differentiated allogeneic MSC in ischemic heart,” Biochemical and Biophysical Research Communications, vol. 438, no. 2, pp. 382–387, 2013. View at: Publisher Site | Google Scholar
  14. W. Zhuo, L. Liao, Y. Fu et al., “Efficiency of endovenous versus arterial administration of mesenchymal stem cells for ischemia-reperfusion-induced renal dysfunction in rats,” Transplantation Proceedings, vol. 45, no. 2, pp. 503–510, 2013. View at: Publisher Site | Google Scholar
  15. M. E. Aanstoos, D. P. Regan, R. J. Rose, L. S. Chubb, and N. P. Ehrhart, “Do mesenchymal stromal cells influence microscopic residual or metastatic osteosarcoma in a murine model?” Clinical Orthopaedics and Related Research, vol. 474, no. 3, pp. 707–715, 2016. View at: Publisher Site | Google Scholar
  16. M. Dominici, K. Le Blanc, I. Mueller et al., “Minimal criteria for defining multipotent mesenchymal stromal cells. The International Society for Cellular Therapy position statement,” Cytotherapy, vol. 8, no. 4, pp. 315–317, 2006. View at: Publisher Site | Google Scholar
  17. A. Tyndall, “Mesenchymal stem cell treatments in rheumatology—a glass half full?” Nature Reviews Rheumatology, vol. 10, no. 2, pp. 117–124, 2014. View at: Publisher Site | Google Scholar
  18. F. Gao, S. M. Chiu, D. A. Motan et al., “Mesenchymal stem cells and immunomodulation: current status and future prospects,” Cell Death and Disease, vol. 7, no. 1, Article ID e2062, 2016. View at: Publisher Site | Google Scholar
  19. S. Kidd, E. Spaeth, J. L. Dembinski et al., “Direct evidence of mesenchymal stem cell tropism for tumor and wounding microenvironments using in vivo bioluminescent imaging,” Stem Cells, vol. 27, no. 10, pp. 2614–2623, 2009. View at: Publisher Site | Google Scholar
  20. S. M. Albarenque, R. M. Zwacka, and A. Mohr, “Both human and mouse mesenchymal stem cells promote breast cancer metastasis,” Stem Cell Research, vol. 7, no. 2, pp. 163–171, 2011. View at: Publisher Site | Google Scholar
  21. E. Eggenhofer, V. Benseler, A. Kroemer et al., “Mesenchymal stem cells are short-lived and do not migrate beyond the lungs after intravenous infusion,” Frontiers in Immunology, vol. 3, article 297, Article ID Article 297, 2012. View at: Publisher Site | Google Scholar
  22. S. Schrepfer, T. Deuse, H. Reichenspurner, M. P. Fischbein, R. C. Robbins, and M. P. Pelletier, “Stem cell transplantation: the lung barrier,” Transplantation Proceedings, vol. 39, no. 2, pp. 573–576, 2007. View at: Publisher Site | Google Scholar
  23. C. Quan, M. K. Cho, Y. Shao et al., “Dermal fibroblast expression of stromal cell-derived factor-1 (SDF-1) promotes epidermal keratinocyte proliferation in normal and diseased skin,” Protein and Cell, vol. 6, no. 12, pp. 890–903, 2015. View at: Publisher Site | Google Scholar
  24. S.-B. Zhou, J. Wang, C.-A. Chiang, L.-L. Sheng, and Q.-F. Li, “Mechanical stretch upregulates SDF-1α in skin tissue and induces migration of circulating bone marrow-derived stem cells into the expanded skin,” Stem Cells, vol. 31, no. 12, pp. 2703–2713, 2013. View at: Publisher Site | Google Scholar
  25. M. F. Pittenger and B. J. Martin, “Mesenchymal stem cells and their potential as cardiac therapeutics,” Circulation Research, vol. 95, no. 1, pp. 9–20, 2004. View at: Publisher Site | Google Scholar
  26. A. F. Wise, T. M. Williams, M. B. G. Kiewiet et al., “Human mesenchymal stem cells alter macrophage phenotype and promote regeneration via homing to the kidney following ischemia-reperfusion injury,” American Journal of Physiology—Renal Physiology, vol. 306, no. 10, pp. F1222–F1235, 2014. View at: Publisher Site | Google Scholar
  27. Y. Yao, J. Huang, Y. Geng et al., “Paracrine action of mesenchymal stem cells revealed by single cell gene profiling in infarcted murine hearts,” PLoS ONE, vol. 10, no. 6, Article ID e0129164, 2015. View at: Publisher Site | Google Scholar
  28. J.-B. Michel, “Anoïkis in the cardiovascular system: known and unknown extracellular mediators,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 23, no. 12, pp. 2146–2154, 2003. View at: Publisher Site | Google Scholar
  29. J. L. Spees, C. A. Gregory, H. Singh et al., “Internalized antigens must be removed to prepare hypoimmunogenic mesenchymal stem cells for cell and gene therapy,” Molecular Therapy, vol. 9, no. 5, pp. 747–756, 2004. View at: Publisher Site | Google Scholar
  30. O. Honmou, K. Houkin, T. Matsunaga et al., “Intravenous administration of auto serum-expanded autologous mesenchymal stem cells in stroke,” Brain, vol. 134, no. 6, pp. 1790–1807, 2011. View at: Publisher Site | Google Scholar
  31. F. Tögel, Y. Yang, P. Zhang, Z. Hu, and C. Westenfelder, “Bioluminescence imaging to monitor the in vivo distribution of administered mesenchymal stem cells in acute kidney injury,” American Journal of Physiology—Renal Physiology, vol. 295, no. 1, pp. F315–F321, 2008. View at: Publisher Site | Google Scholar
  32. D. G. Halme and D. A. Kessler, “FDA regulation of stem-cell-based therapies,” New England Journal of Medicine, vol. 355, no. 16, pp. 1730–1735, 2006. View at: Publisher Site | Google Scholar

Copyright © 2016 Juan Cao et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

More related articles

 PDF Download Citation Citation
 Download other formatsMore
 Order printed copiesOrder

Related articles

We are committed to sharing findings related to COVID-19 as quickly as possible. We will be providing unlimited waivers of publication charges for accepted research articles as well as case reports and case series related to COVID-19. Review articles are excluded from this waiver policy. Sign up here as a reviewer to help fast-track new submissions.