In Vivo Ectopic Bone Formation by Devitalized Mineralized Stem Cell Carriers Produced Under Mineralizing Culture Condition
Identifieur interne : 000338 ( Pmc/Corpus ); précédent : 000337; suivant : 000339In Vivo Ectopic Bone Formation by Devitalized Mineralized Stem Cell Carriers Produced Under Mineralizing Culture Condition
Auteurs : Yoke Chin Chai ; Liesbet Geris ; Johanna Bolander ; Grzegorz Pyka ; Simon Van Bael ; Frank P. Luyten ; Jan SchrootenSource :
- BioResearch Open Access [ 2164-7844 ] ; 2014.
Abstract
Functionalization of tissue engineering scaffolds with
Url:
DOI: 10.1089/biores.2014.0050
PubMed: 25469312
PubMed Central: 4245878
Links to Exploration step
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<record><TEI><teiHeader><fileDesc><titleStmt><title xml:lang="en"><italic>In Vivo</italic> Ectopic Bone Formation by Devitalized Mineralized Stem Cell Carriers Produced Under Mineralizing Culture Condition</title><author><name sortKey="Chai, Yoke Chin" sort="Chai, Yoke Chin" uniqKey="Chai Y" first="Yoke Chin" last="Chai">Yoke Chin Chai</name><affiliation><nlm:aff id="aff1"></nlm:aff></affiliation><affiliation><nlm:aff id="aff2"></nlm:aff></affiliation><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation></author><author><name sortKey="Geris, Liesbet" sort="Geris, Liesbet" uniqKey="Geris L" first="Liesbet" last="Geris">Liesbet Geris</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff4"></nlm:aff></affiliation></author><author><name sortKey="Bolander, Johanna" sort="Bolander, Johanna" uniqKey="Bolander J" first="Johanna" last="Bolander">Johanna Bolander</name><affiliation><nlm:aff id="aff1"></nlm:aff></affiliation><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation></author><author><name sortKey="Pyka, Grzegorz" sort="Pyka, Grzegorz" uniqKey="Pyka G" first="Grzegorz" last="Pyka">Grzegorz Pyka</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff5"></nlm:aff></affiliation></author><author><name sortKey="Van Bael, Simon" sort="Van Bael, Simon" uniqKey="Van Bael S" first="Simon" last="Van Bael">Simon Van Bael</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff6"></nlm:aff></affiliation></author><author><name sortKey="Luyten, Frank P" sort="Luyten, Frank P" uniqKey="Luyten F" first="Frank P." last="Luyten">Frank P. Luyten</name><affiliation><nlm:aff id="aff1"></nlm:aff></affiliation><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation></author><author><name sortKey="Schrooten, Jan" sort="Schrooten, Jan" uniqKey="Schrooten J" first="Jan" last="Schrooten">Jan Schrooten</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff5"></nlm:aff></affiliation></author></titleStmt><publicationStmt><idno type="wicri:source">PMC</idno><idno type="pmid">25469312</idno><idno type="pmc">4245878</idno><idno type="url">http://www.ncbi.nlm.nih.gov/pmc/articles/PMC4245878</idno><idno type="RBID">PMC:4245878</idno><idno type="doi">10.1089/biores.2014.0050</idno><date when="2014">2014</date><idno type="wicri:Area/Pmc/Corpus">000338</idno></publicationStmt><sourceDesc><biblStruct><analytic><title xml:lang="en" level="a" type="main"><italic>In Vivo</italic> Ectopic Bone Formation by Devitalized Mineralized Stem Cell Carriers Produced Under Mineralizing Culture Condition</title><author><name sortKey="Chai, Yoke Chin" sort="Chai, Yoke Chin" uniqKey="Chai Y" first="Yoke Chin" last="Chai">Yoke Chin Chai</name><affiliation><nlm:aff id="aff1"></nlm:aff></affiliation><affiliation><nlm:aff id="aff2"></nlm:aff></affiliation><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation></author><author><name sortKey="Geris, Liesbet" sort="Geris, Liesbet" uniqKey="Geris L" first="Liesbet" last="Geris">Liesbet Geris</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff4"></nlm:aff></affiliation></author><author><name sortKey="Bolander, Johanna" sort="Bolander, Johanna" uniqKey="Bolander J" first="Johanna" last="Bolander">Johanna Bolander</name><affiliation><nlm:aff id="aff1"></nlm:aff></affiliation><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation></author><author><name sortKey="Pyka, Grzegorz" sort="Pyka, Grzegorz" uniqKey="Pyka G" first="Grzegorz" last="Pyka">Grzegorz Pyka</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff5"></nlm:aff></affiliation></author><author><name sortKey="Van Bael, Simon" sort="Van Bael, Simon" uniqKey="Van Bael S" first="Simon" last="Van Bael">Simon Van Bael</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff6"></nlm:aff></affiliation></author><author><name sortKey="Luyten, Frank P" sort="Luyten, Frank P" uniqKey="Luyten F" first="Frank P." last="Luyten">Frank P. Luyten</name><affiliation><nlm:aff id="aff1"></nlm:aff></affiliation><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation></author><author><name sortKey="Schrooten, Jan" sort="Schrooten, Jan" uniqKey="Schrooten J" first="Jan" last="Schrooten">Jan Schrooten</name><affiliation><nlm:aff id="aff3"></nlm:aff></affiliation><affiliation><nlm:aff id="aff5"></nlm:aff></affiliation></author></analytic><series><title level="j">BioResearch Open Access</title><idno type="ISSN">2164-7844</idno><idno type="eISSN">2164-7860</idno><imprint><date when="2014">2014</date></imprint></series></biblStruct></sourceDesc></fileDesc><profileDesc><textClass></textClass></profileDesc></teiHeader><front><div type="abstract" xml:lang="en"><title>Abstract</title><p>Functionalization of tissue engineering scaffolds with <italic>in vitro</italic>–generated bone-like extracellular matrix (ECM) represents an effective biomimetic approach to promote osteogenic differentiation of stem cells <italic>in vitro</italic>. However, the bone-forming capacity of these constructs (seeded with or without cells) is so far not apparent. In this study, we aimed at developing a mineralizing culture condition to biofunctionalize three-dimensional (3D) porous scaffolds with highly mineralized ECM in order to produce devitalized, osteoinductive mineralized carriers for human periosteal-derived progenitors (hPDCs). For this, three medium formulations [i.e., growth medium only (BM1), with ascorbic acid (BM2), and with ascorbic acid and dexamethasone (BM3)] supplemented with calcium (Ca<sup>2+</sup>) and phosphate (PO<sub>4</sub><sup>3−</sup>) ions simultaneously as mineralizing source were investigated. The results showed that, besides the significant impacts on enhancing cell proliferation (the highest in BM3 condition), the formulated mineralizing media differentially regulated the osteochondro-related gene markers in a medium-dependent manner (e.g., significant upregulation of <italic>BMP2</italic>, bone sialoprotein, osteocalcin, and <italic>Wnt5a</italic> in BM2 condition). This has resulted in distinguished cell populations that were identifiable by specific gene signatures as demonstrated by the principle component analysis. Through devitalization, mineralized carriers with apatite crystal structures unique to each medium condition (by X-ray diffraction and SEM analysis) were obtained. Quantitatively, BM3 condition produced carriers with the highest mineral and collagen contents as well as human-specific VEGF proteins, followed by BM2 and BM1 conditions. Encouragingly, all mineralized carriers (after reseeded with hPDCs) induced bone formation after 8 weeks of subcutaneous implantation in nude mice models, with BM2-carriers inducing the highest bone volume, and the lowest in the BM3 condition (as quantitated by nano-computed tomography [nano-CT]). Histological analysis revealed different bone formation patterns, either bone ossicles containing bone marrow surrounding the scaffold struts (in BM2) or bone apposition directly on the struts' surface (in BM1 and BM3). In conclusion, we have presented experimental data on the feasibility to produce devitalized osteoinductive mineralized carriers by functionalizing 3D porous scaffolds with an <italic>in vitro</italic> cell-made mineralized matrix under the mineralizing culture conditions.</p></div></front><back><div1 type="bibliography"><listBibl><biblStruct><analytic><author><name sortKey="Ma, Px" uniqKey="Ma P">PX Ma</name></author></analytic></biblStruct><biblStruct><analytic><author><name sortKey="Ingber, De" uniqKey="Ingber D">DE Ingber</name></author></analytic></biblStruct><biblStruct><analytic><author><name sortKey="Grayson, Wl" uniqKey="Grayson W">WL Grayson</name></author></analytic></biblStruct><biblStruct><analytic><author><name sortKey="Benders, Ke" uniqKey="Benders K">KE Benders</name></author></analytic></biblStruct><biblStruct><analytic><author><name sortKey="Badylak, Sf" uniqKey="Badylak S">SF Badylak</name></author></analytic></biblStruct><biblStruct><analytic><author><name 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<front><journal-meta><journal-id journal-id-type="nlm-ta">Biores Open Access</journal-id><journal-id journal-id-type="iso-abbrev">Biores Open Access</journal-id><journal-id journal-id-type="publisher-id">biores</journal-id><journal-title-group><journal-title>BioResearch Open Access</journal-title></journal-title-group><issn pub-type="ppub">2164-7844</issn><issn pub-type="epub">2164-7860</issn><publisher><publisher-name>Mary Ann Liebert, Inc.</publisher-name><publisher-loc>140 Huguenot Street, 3rd FloorNew Rochelle, NY 10801USA</publisher-loc></publisher></journal-meta><article-meta><article-id pub-id-type="pmid">25469312</article-id><article-id pub-id-type="pmc">4245878</article-id><article-id pub-id-type="publisher-id">10.1089/biores.2014.0050</article-id><article-id pub-id-type="doi">10.1089/biores.2014.0050</article-id><article-categories><subj-group subj-group-type="heading"><subject>Original Research Articles</subject></subj-group></article-categories><title-group><article-title><italic>In Vivo</italic> Ectopic Bone Formation by Devitalized Mineralized Stem Cell Carriers Produced Under Mineralizing Culture Condition</article-title></title-group><contrib-group><contrib contrib-type="author"><name><surname>Chai</surname><given-names>Yoke Chin</given-names></name><xref ref-type="aff" rid="aff1"><sup>1,</sup></xref><xref ref-type="aff" rid="aff2"><sup>2,</sup></xref><xref ref-type="aff" rid="aff3"><sup>3</sup></xref></contrib><contrib contrib-type="author"><name><surname>Geris</surname><given-names>Liesbet</given-names></name><xref ref-type="aff" rid="aff3"><sup>3,</sup></xref><xref ref-type="aff" rid="aff4"><sup>4</sup></xref></contrib><contrib contrib-type="author"><name><surname>Bolander</surname><given-names>Johanna</given-names></name><xref ref-type="aff" rid="aff1"><sup>1,</sup></xref><xref ref-type="aff" rid="aff3"><sup>3</sup></xref></contrib><contrib contrib-type="author"><name><surname>Pyka</surname><given-names>Grzegorz</given-names></name><xref ref-type="aff" rid="aff3"><sup>3,</sup></xref><xref ref-type="aff" rid="aff5"><sup>5</sup></xref></contrib><contrib contrib-type="author"><name><surname>Van Bael</surname><given-names>Simon</given-names></name><xref ref-type="aff" rid="aff3"><sup>3,</sup></xref><xref ref-type="aff" rid="aff6"><sup>6</sup></xref></contrib><contrib contrib-type="author"><name><surname>Luyten</surname><given-names>Frank P.</given-names></name><xref ref-type="aff" rid="aff1"><sup>1,</sup></xref><xref ref-type="aff" rid="aff3"><sup>3,</sup></xref><xref ref-type="author-notes" rid="fn1"><sup>*</sup></xref></contrib><contrib contrib-type="author" corresp="yes"><name><surname>Schrooten</surname><given-names>Jan</given-names></name><xref ref-type="aff" rid="aff3"><sup>3,</sup></xref><xref ref-type="aff" rid="aff5"><sup>5,</sup></xref><xref ref-type="author-notes" rid="fn1"><sup>*</sup></xref></contrib><aff id="aff1"><label><sup>1</sup></label>Tissue Engineering Laboratory,<institution>Skeletal Biology and Engineering Research Center</institution>, KU Leuven, Leuven,<country>Belgium</country>.</aff><aff id="aff2"><label><sup>2</sup></label>Department of Biomedical Engineering, Faculty of Engineering,<institution>University of Malaya</institution>, Kuala Lumpur,<country>Malaysia</country>.</aff><aff id="aff3"><label><sup>3</sup></label>Prometheus, Division of Skeletal Tissue Engineering,<institution>KU Leuven</institution>, Leuven,<country>Belgium</country>.</aff><aff id="aff4"><label><sup>4</sup></label>Biomechanics Research Unit,<institution>University of Liege</institution>, Liege,<country>Belgium</country>.</aff><aff id="aff5"><label><sup>5</sup></label>Department of Materials Engineering,<institution>KU Leuven</institution>, Heverlee,<country>Belgium</country>.</aff><aff id="aff6"><label><sup>6</sup></label>Division of Production Engineering, Machine Design and Automation, Department of Mechanical Engineering,<institution>KU Leuven</institution>, Heverlee,<country>Belgium</country>.</aff></contrib-group><author-notes><fn id="fn1" fn-type="eqaul"><label><sup>*</sup></label><p>Shared senior authorship: Jan Schrooten and Frank P. Luyten.</p></fn><corresp><addr-line>Address correspondence to:</addr-line><addr-line><italic>Jan Schrooten, PhD</italic></addr-line><addr-line><italic>Prometheus</italic></addr-line><addr-line><italic>Division of Skeletal Tissue Engineering</italic></addr-line><addr-line><italic>Department of Materials Engineering</italic></addr-line><institution><italic>KU Leuven</italic></institution><addr-line><italic>Kasteelpark Arenberg 44</italic></addr-line><addr-line><italic>Bus 2450</italic></addr-line><addr-line><italic>3001 Heverlee</italic></addr-line><country>Belgium</country><break></break><italic>E-mail:</italic><email xlink:href="mailto:jan.schrooten@mtm.kuleuven.be">jan.schrooten@mtm.kuleuven.be</email></corresp></author-notes><pub-date pub-type="ppub"><day>01</day><month>12</month><year>2014</year><pmc-comment>string-date: December 2014</pmc-comment>
</pub-date><pub-date pub-type="pmc-release"><day>01</day><month>12</month><year>2014</year><pmc-comment>string-date: December 2014</pmc-comment>
</pub-date><pmc-comment> PMC Release delay is 0 months and 0 days and was based on the
<volume>3</volume><issue>6</issue><fpage>265</fpage><lpage>277</lpage><permissions><copyright-statement>Copyright 2014, Mary Ann Liebert, Inc.</copyright-statement><copyright-year>2014</copyright-year></permissions><self-uri content-type="pdf" xlink:type="simple" xlink:href="biores.2014.0050.pdf"></self-uri><abstract><title>Abstract</title><p>Functionalization of tissue engineering scaffolds with <italic>in vitro</italic>–generated bone-like extracellular matrix (ECM) represents an effective biomimetic approach to promote osteogenic differentiation of stem cells <italic>in vitro</italic>. However, the bone-forming capacity of these constructs (seeded with or without cells) is so far not apparent. In this study, we aimed at developing a mineralizing culture condition to biofunctionalize three-dimensional (3D) porous scaffolds with highly mineralized ECM in order to produce devitalized, osteoinductive mineralized carriers for human periosteal-derived progenitors (hPDCs). For this, three medium formulations [i.e., growth medium only (BM1), with ascorbic acid (BM2), and with ascorbic acid and dexamethasone (BM3)] supplemented with calcium (Ca<sup>2+</sup>) and phosphate (PO<sub>4</sub><sup>3−</sup>) ions simultaneously as mineralizing source were investigated. The results showed that, besides the significant impacts on enhancing cell proliferation (the highest in BM3 condition), the formulated mineralizing media differentially regulated the osteochondro-related gene markers in a medium-dependent manner (e.g., significant upregulation of <italic>BMP2</italic>, bone sialoprotein, osteocalcin, and <italic>Wnt5a</italic> in BM2 condition). This has resulted in distinguished cell populations that were identifiable by specific gene signatures as demonstrated by the principle component analysis. Through devitalization, mineralized carriers with apatite crystal structures unique to each medium condition (by X-ray diffraction and SEM analysis) were obtained. Quantitatively, BM3 condition produced carriers with the highest mineral and collagen contents as well as human-specific VEGF proteins, followed by BM2 and BM1 conditions. Encouragingly, all mineralized carriers (after reseeded with hPDCs) induced bone formation after 8 weeks of subcutaneous implantation in nude mice models, with BM2-carriers inducing the highest bone volume, and the lowest in the BM3 condition (as quantitated by nano-computed tomography [nano-CT]). Histological analysis revealed different bone formation patterns, either bone ossicles containing bone marrow surrounding the scaffold struts (in BM2) or bone apposition directly on the struts' surface (in BM1 and BM3). In conclusion, we have presented experimental data on the feasibility to produce devitalized osteoinductive mineralized carriers by functionalizing 3D porous scaffolds with an <italic>in vitro</italic> cell-made mineralized matrix under the mineralizing culture conditions.</p></abstract><kwd-group kwd-group-type="author"><title><bold>Key words:</bold> </title><kwd>biomineralization</kwd><kwd>bone regeneration</kwd><kwd>devitalization</kwd><kwd>mineralized extracellular matrix</kwd><kwd>osteoinductive carriers</kwd></kwd-group><counts><fig-count count="7"></fig-count><table-count count="2"></table-count><ref-count count="65"></ref-count><page-count count="13"></page-count></counts></article-meta></front><body><sec sec-type="intro" id="s001"><title>Introduction</title><p>A <sc>successful repair of defected</sc> tissue/organ via tissue engineering approach requires the engineering of constructs with a high degree of biomimetic modalities that recapitulate the native tissue developmental process in an <italic>in vivo</italic> recognizable and bioinstructive manner.<sup><xref rid="B1" ref-type="bibr">1</xref>,<xref rid="B2" ref-type="bibr">2</xref></sup> These requirements represent a unique scientific art to “decorate” synthetic constructs <italic>in vitro</italic> with crucial biological entities that could timely promote construct viability, direct tissues growth, and subsequently integrate and function within the host system. However, development of such “intelligent” construct is both scientifically and technologically challenging<sup><xref rid="B3" ref-type="bibr">3</xref></sup> due to the high complexity of a biological system, and hence hinders the identification of key biological elements and their sequential events that are to be engineered.<sup><xref rid="B4" ref-type="bibr">4</xref></sup></p><p>Recently, whole organ-derived decellularized extracellular matrix (ECM) has been explored as a native building block to facilitate tissue/organ regeneration by combining it with stem cells.<sup><xref rid="B5" ref-type="bibr">5</xref></sup> It is hypothesized that the native ECM provides a natural biological framework containing the necessary bioactive motifs and microenvironment niche that favor tissue growth.<sup><xref rid="B6" ref-type="bibr">6</xref></sup> Indeed, this approach has shown reactivation of specific organ functionalities, such as the <italic>in vitro</italic> “beating” of a heart after repopulating a decellularized heart with predifferentiated contractile cells.<sup><xref rid="B7" ref-type="bibr">7</xref></sup> Nevertheless, this approach is not novel in the field of skeletal repair, where demineralized bone matrix (DBM) has a long clinical track record as bone filler<sup><xref rid="B8" ref-type="bibr">8</xref>,<xref rid="B9" ref-type="bibr">9</xref></sup> and has also been widely investigated as a tissue engineering carrier for bone defect repair.<sup><xref rid="B10" ref-type="bibr">10–12</xref></sup> Unfortunately, the use of DBM (either xeno- or allogeneic) has several drawbacks.<sup><xref rid="B8" ref-type="bibr">8</xref></sup> To overcome these, scientists have resorted to use <italic>in vitro</italic> cell culture–derived mineralized ECM as possible alternative osteoinductive motif to functionalize three-dimensional (3D) porous scaffolds.<sup><xref rid="B13" ref-type="bibr">13</xref></sup> In fact, enhanced osteogenic differentiation <italic>in vitro</italic> has been reported<sup><xref rid="B14" ref-type="bibr">14</xref>,<xref rid="B15" ref-type="bibr">15</xref></sup>; however, the bone-forming capacity is so far not apparent.<sup><xref rid="B16" ref-type="bibr">16</xref>,<xref rid="B17" ref-type="bibr">17</xref></sup></p><p>It is known that bone matrix consists of mineralized collagen fibers embedded with essential growth factors and trace elements. This matrix is produced by osteoblastic cells through specific physiological events,<sup><xref rid="B18" ref-type="bibr">18</xref>,<xref rid="B19" ref-type="bibr">19</xref></sup> giving rise to a unique biological architecture and mineralization hierarchy<sup><xref rid="B20" ref-type="bibr">20</xref>,<xref rid="B21" ref-type="bibr">21</xref></sup> that governs its functionality and osteoinductivity.<sup><xref rid="B22" ref-type="bibr">22</xref></sup> Introducing all these biomimetic features in a controlled way through synthetic processing routes (such as biomimetic deposition in simulated body fluid,<sup><xref rid="B23" ref-type="bibr">23</xref>,<xref rid="B24" ref-type="bibr">24</xref></sup> electrolytic deposition,<sup><xref rid="B25" ref-type="bibr">25</xref>,<xref rid="B26" ref-type="bibr">26</xref></sup> plasma spraying,<sup><xref rid="B27" ref-type="bibr">27</xref>,<xref rid="B28" ref-type="bibr">28</xref></sup> and sol-gel<sup><xref rid="B29" ref-type="bibr">29</xref>,<xref rid="B30" ref-type="bibr">30</xref></sup> techniques) remains challenging, mainly due to the lack of in-depth knowledge on the biological events and the limitations of existing technological tools.<sup><xref rid="B31" ref-type="bibr">31–33</xref></sup> Recently, we have reported the feasibility to use either Ca<sup>2+</sup> or PO<sub>4</sub><sup>3−</sup> supplementation to produce living 3D osteogenic hybrids <italic>in vitro.</italic><sup><xref rid="B34" ref-type="bibr">34</xref></sup> However, simultaneous use of Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> as mineralizing sources to functionalize a bio-inert scaffold with highly mineralized ECM in order to produce devitalized osteoinductive stem cells carriers has not been explored. Therefore, in this study we aimed at developing a so-called biomineralization medium (BM) to promote <italic>in vitro</italic> cell proliferation, osteogenic differentiation, and high bone-like ECM deposition on 3D porous scaffolds. We anticipate that this approach may facilitate the production of robust biomimetic mineralized carriers enriched with natural cell adhesion peptides and osteoinductive motifs that are minimally required to effectively emulate bone-specific cell–ECM interactions, eventually leading to osteogenesis preceded by matrix remodeling.</p><p>To test this hypothesis, simultaneous Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> supplementation in three medium formulations [i.e., in growth medium (BM1), growth medium plus ascorbic acid (BM2), and growth medium plus ascorbic acid plus dexamethasone (BM3); <xref ref-type="table" rid="T1">Table 1</xref>] were investigated using human periosteal-derived progenitors (hPDCs) seeded on 3D open porous, bio-inert Ti6Al4V (Ti)-scaffolds produced by additive manufacturing. This includes 3D hPDC proliferation and osteochondro-related gene marker expression. After devitalization, the microscopic mineral morphology, composition, and the presence of growth factors in the matrix extracts were assessed. The ectopic bone-forming capacity was evaluated by subcutaneous implantation of hPDC-reseeded mineralized carriers in nude mice for 8 weeks followed by nano-CT quantification and histological analysis.</p><table-wrap id="T1" orientation="portrait" position="float"><label><sc>Table</sc> 1.</label><caption><p><sc>Composition of the Investigated Biomineralization Media as Compared to the Control Medium (GM′ or OM</sc><sup>−</sup><sc>) Without Ca</sc><sup>2+</sup><sc>and PO</sc><sub>4</sub><sup>3−</sup><sc>Supplementation</sc></p></caption><pmc-comment>OASIS TABLE HERE</pmc-comment>
<table frame="hsides" rules="groups"><colgroup><col align="left"></col><col align="left"></col><col align="left"></col><col align="left"></col><col align="left"></col></colgroup><thead><tr><th align="left"><italic>Treatment</italic></th><th align="center"><italic>Growth medium</italic></th><th align="center"><italic>Ascorbic acid (50 μg/ml)</italic></th><th align="center"><italic>Dexamethasone (100 nM)</italic></th><th align="center"><italic>6 mM Ca<sup>2+</sup>+4 mM PO<sub>4</sub><sup>3−</sup></italic></th></tr></thead><tbody><tr><td align="left">GM′</td><td align="center">+</td><td align="center">+</td><td align="center">−</td><td align="center">−</td></tr><tr><td align="left">OM<sup>−</sup></td><td align="center">+</td><td align="center">+</td><td align="center">+</td><td align="center">−</td></tr><tr><td align="left">BM1</td><td align="center">+</td><td align="center">−</td><td align="center">−</td><td align="center">+</td></tr><tr><td align="left">BM2</td><td align="center">+</td><td align="center">+</td><td align="center">−</td><td align="center">+</td></tr><tr><td align="left">BM3</td><td align="center">+</td><td align="center">+</td><td align="center">+</td><td align="center">+</td></tr></tbody></table><table-wrap-foot><fn id="tf1"><p>“+” and “−” indicate the presence and absence of the respective chemical compounds.</p></fn><fn id="tf2"><p>BM, biomineralization media; GM, growth medium.</p></fn></table-wrap-foot></table-wrap></sec><sec sec-type="materials|methods" id="s002"><title>Materials and Methods</title><sec id="s003"><title>Materials</title><p>Calcium chloride (CaCl<sub>2</sub>·6H<sub>2</sub>O; Applichem), sodium di-hydrogen phosphate dihydrate (NaH<sub>2</sub>PO<sub>4</sub>·2H<sub>2</sub>O; Merck), di-sodium hydrogen phosphate dehydrate (Na<sub>2</sub>HPO<sub>4</sub>·2H<sub>2</sub>O; Merck), dexamethasone (Sigma-Aldrich), and L-ascorbic acid 2-phosphate sesquimagnesium hydrate (Sigma-Aldrich) were purchased from the manufacturers. Center hollow (diameter 2 mm), diamond unit cell, 3D open porous Ti6Al4V (Ti)-scaffolds (diameter 6 mm×height 3 mm; pore size 1000 μm; porosity 93%) were designed using Magics software (Materialise N.V.) and produced by selective laser melting.<sup><xref rid="B35" ref-type="bibr">35</xref></sup> The scaffolds were then cleaned with acetone, 96% ethanol, and demineralized water (each for 15 min) using ultrasonic bath, followed by oxidation in 5 M NaOH at 60°C for 24 h and finally rinsed thoroughly with demineralized water before sterilized by autoclaving. Prior to cell seeding, the sterilized scaffolds were prewetted with culture medium containing 10% fetal bovine serum (FBS) for 2 h, and dried overnight in laminar flow under sterile condition. Using computed tomography and image analysis techniques, the sterilized scaffolds were reported to have an average pore size of around 822 μm and an average porosity of 81%.<sup><xref rid="B34" ref-type="bibr">34</xref></sup></p></sec><sec id="s004"><title><italic>In vitro</italic> seeding and growth of hPDCs cultured on Ti-scaffolds in various BM</title><p>Periosteal biopsies were harvested from the proximal tibia of adolescent and adult patients during total knee replacement surgery or distraction osteogenesis with patient informed consent and approval by the ethics committee for Human Medical Research of the University of Leuven. Briefly, after overnight digestion of the biopsies in culture medium containing 0.2% type IV collagenase (Invitrogen) at 37°C, hPDCs were collected by centrifugation and subsequently expanded in growth medium (DMEM+10% FBS+1% antibiotics/antimycotics+1% sodium pyruvate) using T-175 cm<sup>2</sup> flasks. From passage 3 onward, the expanded cells were pooled together and stored in liquid nitrogen. This cell type was reported by our research group to have fibroblastic characteristic and possesses multipotent differentiation capacity of the mesenchymal stem cell (MSC).<sup><xref rid="B36" ref-type="bibr">36</xref></sup></p><p>For all assays in this study, hPDC pooled cells at early passage 4 (known to have higher homogeneity of MSC phenotype and retains bone-forming capacity) were thawed from liquid nitrogen and expanded in growth medium using T-175 cm<sup>2</sup> flask. Upon confluence, the cells were harvested and drop-seeded onto each scaffold (200,000 cells per scaffold), and incubated for 1 h to allow cell attachment before transferred to a rotator for overnight incubation in a cell culture incubator. This cell seeding number was optimized in-house to allow for the observation of cell proliferation and ECM deposition on these particular scaffolds within the stipulated culture time under the influence of the different medium used. Then, the samples were transferred to 12-well suspension plate and cultured dynamically using a 3D rotator (30 rpm, Grant-Bio, UK). Calcium (Ca<sup>2+</sup>) and phosphate (PO<sub>4</sub><sup>3−</sup>) solutions (600 and 400 mM, respectively) were prepared as described previously<sup><xref rid="B37" ref-type="bibr">37</xref></sup> and diluted 100 times in the three medium formulations with the nomenclatures shown in <xref ref-type="table" rid="T1">Table 1</xref>. Cell proliferation in each medium was assessed over 21 days of culture period by measuring the metabolic activity using AlamarBlue (10% in growth medium, Invitrogen) (<italic>n</italic>=3), and DNA content using Quant-iT PicoGreen dsDNA assay (Invitrogen) (<italic>n</italic>=3). Cell viability of hPDCs after 21 days of cultured under different biomineralization media was qualitatively assessed using the LIVE-DEAD viability assay kit (Life Technologies). Non-ion-supplemented growth medium containing 50 μg/ml ascorbic acid (GM′), or growth medium containing 50 μg/ml ascorbic acid and 100 nM dexamethasone (OM<sup>−</sup>) were used for comparison purposes.</p></sec><sec id="s005"><title>Gene expression analysis of hPDCs 3D cultures by quantitative real-time polymerase chain reaction</title><p>The expression of osteochondro-related gene markers by hPDCs after cultured in various BM for 21 days was assessed by quantitative real-time polymerase chain reaction (qRT-PCR; <italic>n</italic>=3). Briefly, cells were harvested in RLT buffer and the total RNA of each sample was extracted using the RNeasy mini kit (Qiagen) as per manufacturer's instructions. The amount of extracted RNA was measured using NanoDrop (Thermo Scientific) and 500 ng of total RNA from each sample was converted to cDNA using RevertAid First Strand cDNA Synthesis kit (Thermo Scientific). qRT-PCR was cycled in a sequence detector (Rotor-Gene 6000; Corbett Life Science) using SYBR Green primers as shown in <xref ref-type="table" rid="T2">Table 2</xref>. Each sample was assessed in duplicate and compared with the housekeeping gene β-actin expression (F5′-CCCAGATCATGTTTGAGACCT-3′; R5′-CCTCGTAGATGGGCACAGT-3′). Relative differences in expression were calculated using the 2<sup>−ΔCT</sup> method, and statistical significance was calculated by comparing to the 2<sup>−ΔCT</sup> of control medium (i.e., GM′). In order to obtain more comprehensive statistical information on the effects of BM treatments on gene expression, principle component analysis (PCA) was performed by loading the obtained gene expression data to the JMP analytical software (SAS Institute Inc.). Then, a scatterplot was produced to visualize the specific gene signatures that represent the induced cell populations after the treatments.</p><table-wrap id="T2" orientation="portrait" position="float"><label><sc>Table</sc> 2.</label><caption><p><sc>Primer Sequences Used for Gene Expression Analysis by Quantitative Real-Time Polymerase Chain Reaction</sc></p></caption><pmc-comment>OASIS TABLE HERE</pmc-comment>
<table frame="hsides" rules="groups"><colgroup><col align="left"></col><col align="left"></col><col align="left"></col></colgroup><thead><tr><th align="left"><italic>Gene</italic></th><th align="center"><italic>Forward sequence</italic></th><th align="center"><italic>Reverse sequence</italic></th></tr></thead><tbody><tr><td align="left"><italic>Runx2</italic></td><td align="left">5′-CGCATTCCTCATCCCAGTAT-3′</td><td align="left">5′-GCCTGGGGTCTGTAATCTGA-3′</td></tr><tr><td align="left"><italic>Osx</italic></td><td align="left">5′-AGTGACCTTTCAGCCTCCAA-3′</td><td align="left">5′-GGGAAAAGGGAGGGTAATCA-3′</td></tr><tr><td align="left"><italic>OCN</italic></td><td align="left">5′-GTGCAGCCTTTGTGTCCAA-3′</td><td align="left">5′-GCTCACACACCTCCCTCCT-3′</td></tr><tr><td align="left"><italic>BMP2</italic></td><td align="left">5′-GTACGCAGGCACTCAGGTC-3′</td><td align="left">5′-TTTTCCCACTCGTTTCTGGT-3′</td></tr><tr><td align="left"><italic>Wnt5a</italic></td><td align="left">5′-GCTCCGCTCGGATTCCTC-3′</td><td align="left">5′- CCAATGGACTTCTTCATGGCG-3′</td></tr><tr><td align="left"><italic>VEGF</italic></td><td align="left">5′-TGCAGATTATGCGGATCAAACC-3′</td><td align="left">5′-TGCATTCACATTTGTTGTGCTGTAG-3′</td></tr><tr><td align="left"><italic>BSP</italic></td><td align="left">5′- GCCAGAGGAAGCAATCACCA-3′</td><td align="left">5′- TCATTGAGAAAGCACAGGCCA-3′</td></tr><tr><td align="left"><italic>Col1</italic></td><td align="left">5′-GACGAAGACATCCCACCAAT-3′</td><td align="left">5′-AGATCACGTCATCGCACAAC-3′</td></tr><tr><td align="left"><italic>Col2</italic></td><td align="left">5′-GGCTTCCATTTCAGCTATGG-3′</td><td align="left">5′-AGCTGCTTCGTCCAGATAGC-3′</td></tr><tr><td align="left"><italic>ALP</italic></td><td align="left">5′-GGACATGCAGTACGAGCTGA-3′</td><td align="left">5′-GTCAATTCTGCCTCCTTCCA-3′</td></tr><tr><td align="left"><italic>RankL</italic></td><td align="left">5′-CATCCCATCTGGTTCCCATAA-3′</td><td align="left">5′-GCCCAACCCCGATCATG-3′</td></tr><tr><td align="left"><italic>OPG</italic></td><td align="left">5′-GGGGACCACAATGAACAACT-3′</td><td align="left">5′-AGCTGATGAGAGGTTTCTTCG-3′</td></tr></tbody></table></table-wrap></sec><sec id="s006"><title>Production of mineralized carriers by devitalization and the mineralized ECM composition analysis</title><p>After 21 days of culture in various BM, the samples were rinsed twice with phosphate buffered saline (Bio-Whittaker) and stored at −80°C in demineralized water under sterile condition. To obtain devitalized mineralized carriers, the samples were thawed from −80°C to 37°C and then subjected to three cycles of freeze–thaw between liquid nitrogen and 37°C water bath (10 min each), followed by air-drying overnight under sterile condition. Then, the devitalized mineralized carriers were stored at −20°C under sterile condition till further analysis. The mineral phase, chemical composition, and microscopic morphology were characterized by X-ray diffraction (XRD) analysis (Seifert XRD 3003 TT; using a Cu K source in the 20–50° 2<italic>θ</italic> range; step size=0.02°; slit size=0.5 mm) and scanning electron microscopy coupled with energy dispersive X-ray analysis (SEM-EDAX, XL30 FEG system; Philips) at 10 kV, respectively. The amount of collagen and mineral contents deposited on Ti-scaffolds under different medium conditions was assessed quantitatively using Picro-Sirius Red (1 mg/ml Sirius Red in saturated Picric acid, <italic>n</italic>=3) and Alizarin Red solutions (<italic>n</italic>=3).<sup><xref rid="B34" ref-type="bibr">34</xref></sup></p></sec><sec id="s007"><title>Detection of secreted human-specific VEGF proteins by Western blots</title><p>Devitalized mineralized carriers were thawed to room temperature and the mineralized matrices were extracted from the Ti-scaffolds using protein extraction buffer (0.3 M PMSF and Protease Inhibition Cocktail; Sigma) under sonication on an ice bath. For each condition, extracts from three samples were pooled and the protein concentrations were determined using the Pierce BCA Protein Assay Kit (Thermo Scientific). Then, 5 μg of extracted proteins was loaded onto a NuPAGE 4–12% Bis-Tris gel (Invitrogen) and thereafter transferred to a polyvinylidene fluoride membrane. The membranes were incubated with primary antibody–goat polyclonal anti-human VEGF<sub>165</sub> (1:1000; R&D Systems) according to the manufacturer's instructions. HRP-conjugated secondary antibody (Jackson) was used at a dilution of 1:2000 and images were developed by an LAS3000 Imaging System (FUJI) following the application of SuperSignal West Femto reagent (Thermo Scientific). Densitometry analysis was performed using Bio-Rad Quantity One software. Monoclonal antibody glyceraldehyde-3-phosphate dehydrogenase (GAPDH) (1:1000; Abcam) was used to assess equal loading of proteins and to quantify relative intensity of protein bands.</p></sec><sec id="s008"><title><italic>In vivo</italic> ectopic implantation of hPDC-reseeded mineralized carriers</title><p>The bone-forming capacity of the mineralized carriers produced under each culture conditions was evaluated by implantation of hPDC-reseeded mineralized carriers in NMRI-nu mice (female, 8 weeks) (three implants per mouse). Briefly, 35 μl of cell suspension containing 2 million hPDCs at passage 4 (being the minimal cell number bench mark used within our research group that is calculated based on the corresponding scaffold volume to ensure bone formation <italic>in vivo</italic>) was drop-seeded onto each carrier and incubated for 1 h to allow cell attachment. Then, an additional 1 ml of growth medium was added and the samples were incubated overnight on a rotator at 30 rpm before implantation in subcutaneous pockets of the mice. The implantation procedures were approved by the local ethics committee for animal research (KU Leuven) and adhered to the regulations of animal housing according to the guidelines of the KU Leuven Animalium.</p></sec><sec id="s009"><title>Characterization of ectopic bone formation by nanofocus X-ray computed tomography and histological analysis</title><p>After 8 weeks of implantation, the samples were retrieved and fixed in 4% paraformaldehyde solution for 2 h and stored in phosphate buffered saline prior to nanofocus X-ray computed tomography (nano-CT) analysis using Phoenix Nanotom S system (GE Measurement and Control Solutions). The explants were scanned at an isotropic voxel size (3.125 μm)<sup><xref rid="B3" ref-type="bibr">3</xref></sup> using a tungsten target with the following parameters: voltage=90 kV, current=170 μA, filter=1 mm aluminum and 0.3 mm copper, exposure time=500 ms, frame averaging=1, scanning time per sample=20 min. Image reconstruction was performed and analyzed using CTAn software (Skyscan NV), by applying an in-house algorithm involving multilevel thresholding, despeckling, and morphological operation with dilation of scaffold volume in order to eliminate the partial volume effect of the metallic materials and to segment out the bone area for quantification of bone volume. Then, the quantified bone volumes were subtracted with the background values quantified for the controls (explants of nonmineralized carriers obtained from GM′ culture condition). For histological analysis, the explants were embedded in poly-methyl methacrylate resin, sectioned using a diamond saw (Leica), and ground to approximately 70-μm-thick tissue sections. Stevenel's Blue & Van Gieson's picrofuchsin staining was used to stain the bone and soft tissue structures.</p></sec><sec id="s010"><title>Statistical analysis</title><p>All experiments were carried out in triplicate to assess statistical significance, and the data are depicted as mean±standard deviation (SD). Unpaired Student <italic>t</italic>-test (two-tailed) was performed to compare means of two groups, whereas one-way analysis of variance (ANOVA) followed by <italic>post-hoc</italic> Tukey's honest significant difference was used to perform multiple comparisons between the means of the experimental conditions and the controls at each time point, by establishing the statistical significance at <italic>p</italic><0.05. Statistical significance is represented as follows: *<italic>p</italic><0.05, <sup>#</sup><italic>p</italic><0.01, and <sup>§</sup><italic>p</italic><0.001.</p></sec></sec><sec sec-type="results" id="s011"><title>Results</title><sec id="s012"><title><italic>In vitro</italic> hPDC growth on 3D porous Ti-scaffolds in the three formulated BM</title><p>As shown in <xref ref-type="fig" rid="f1">Figure 1A</xref>, simultaneous Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> supplementation into growth medium (i.e., BM1) resulted in the lowest metabolic activity over the 28 days of culture. However, the metabolic activity was significantly enhanced (especially at the later time points; <italic>p</italic><0.05) in the presence of ascorbic acid (i.e., BM2) as compared to the control medium (i.e., GM′). In fact, the metabolic activity in BM2 reached a level that was comparable to culture condition containing dexamethasone and ascorbic acid (i.e., OM<sup>−</sup>) at 28 days. Encouragingly, culturing hPDCs in BM3 (supplemented with the ions, ascorbic acid, and dexamethasone) resulted in the highest metabolic activity over 28 days (<italic>p</italic><0.001 for each time point, respectively, as compared to the control medium, GM′). These data were confirmed by the total DNA content measurement on samples harvested at 28 days, where BM1 resulted in a significantly lower DNA content (<italic>p</italic><0.01), and BM2 and BM3 resulted in 1.5-fold (<italic>p</italic><0.01) and 2.3-fold (<italic>p</italic><0.001) higher DNA content than GM′, respectively (<xref ref-type="fig" rid="f1">Fig. 1B</xref>). Brightfield microscopy showed complete closure of the scaffold pores by mineralized culture (*) under BM3 culture condition, and in a lesser extent for BM1 and BM2 conditions (<xref ref-type="fig" rid="f1">Fig. 1C</xref>). No mineralization of cell cultures was observed in the control media (for both GM′ and OM<sup>−</sup>). On the other hand, live–dead staining showed high cell viability in BM2 and BM3 conditions (as indicated by high green fluorescence-labeled cells), and relatively more dead cells (red fluorescence-labeled cells,↑) were observed in BM1 condition.</p><fig id="f1" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 1.</bold></label><caption><p><italic>In vitro</italic> human periosteal-derived progenitor (hPDC) growth on Ti-scaffolds in different biomineralization medium (BM). <bold>(A, B)</bold> The kinetics of metabolic activity over 28 days of culture and the total DNA content at 28 days, as compared to the controls (i.e., GM′ and OM<sup>−</sup>). <bold>(C)</bold> The representative brightfield and fluorescence images showing different extent of mineralization of hPDC cultures (*) and the living (stained green) and dead cells (stained red,↑). Mean±SD (<italic>n</italic>=3). One-way analysis of variance (ANOVA) and <italic>post-hoc</italic> Tukey's multiple comparison test: *<italic>p</italic><0.05, <sup>#</sup><italic>p</italic><0.01, <sup>§</sup><italic>p</italic><0.001; n.s.=not significant.</p></caption><graphic xlink:href="fig-1"></graphic></fig></sec><sec id="s013"><title><italic>In vitro</italic> osteochondro-related gene markers expressions by hPDC on Ti-Scaffolds in the three formulated BM</title><p>The effects of the formulated BM on osteogenic differentiation, bone-like matrix production, and osteoclastic recruitment activity were assessed at gene expression level by qRT-PCR after 21 days of culture, as shown in <xref ref-type="fig" rid="f2">Figure 2</xref>. The results showed that simultaneous Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> supplementation into the three culture media upregulated osteogenic differentiation markers, that is, osterix and <italic>Runx2</italic>, as compared to the control medium, that is, GM′ (<xref ref-type="fig" rid="f2">Fig. 2A</xref>). Interestingly, osterix expression was most significantly upregulated (<italic>p</italic><0.01) by the ion supplementation (i.e., BM1), but was reduced in the presence of ascorbic acid (i.e., BM2) and dexamethasone (i.e., BM3). In contrast, ion supplementation along with ascorbic acid and dexamethasone (i.e., BM3) enhanced <italic>Runx2</italic> expression (<italic>p</italic><0.01), which was significantly higher than the BM1 condition (<italic>p</italic><0.05). Additionally, bone sialoprotein (<italic>BSP</italic>), an osteogenic differentiation and bone matrix marker, was highly upregulated in the BM2 condition (<italic>p</italic><0.001), but was differentially downregulated in the BM3 condition (<italic>p</italic><0.05) as compared to GM′.</p><fig id="f2" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 2.</bold></label><caption><p><italic>In vitro</italic> osteogenic-related markers' expression of hPDCs on Ti-scaffolds after cultured in various BM conditions for 21 days. <bold>(A)</bold> Osteogenic differentiation markers: osterix (<italic>Osx</italic>), Runt-related transcription factor-2 (<italic>Runx2</italic>), bone sialoprotein (<italic>BSP</italic>), osteocalcin (<italic>OCN</italic>), bone morphogenetic protein-2 (<italic>BMP2</italic>), and wingless-type 5a ligand (<italic>Wnt5a</italic>); <bold>(B)</bold> matrix and mineralization markers: collagen-type 1 (<italic>Col1</italic>), collagen-type 2 (<italic>Col2</italic>), and alkaline phosphatase (<italic>ALP</italic>); <bold>(C)</bold> osteoclastic recruitment markers: receptor activator of nuclear factor kappa-B ligand (<italic>RankL</italic>), and osteoprotegerin (<italic>OPG</italic>). Mean±SD (<italic>n</italic>=3). One-way ANOVA and <italic>post-hoc</italic> Tukey's multiple comparison test: *<italic>p</italic><0.05, <sup>#</sup><italic>p</italic><0.01, <sup>§</sup><italic>p</italic><0.001; n.s.=not significant.</p></caption><graphic xlink:href="fig-2"></graphic></fig><p>Although osteocalcin (<italic>OCN</italic>) expression was increased in BM2, it was not significantly different from the expression in GM″, and the expression in BM1 but was significantly higher than that of BM3 (<italic>p</italic><0.05). <italic>BMP2</italic> expression was found to be significantly enhanced in the BM1 (<italic>p</italic><0.05) and BM2 (<italic>p</italic><0.01) conditions, but no significant difference was found between the expression in BM3 and GM′ conditions. Similarly, noncanonical Wnt ligand, that is, <italic>Wnt5a</italic>, was significantly enhanced in BM1 and BM2 as compared to BM3 and GM′ conditions (<italic>p</italic><0.01 for both cases). Furthermore, gene expression analysis revealed a downregulation of <italic>Col1</italic> and <italic>ALP</italic> expressions in all the three BM as compared to the control media (GM′), with no significant effect on <italic>Col2</italic> (<xref ref-type="fig" rid="f2">Fig. 2B</xref>). Finally, culturing hPDCs in BM1 induced the highest osteoclastic recruitment activity (as indicated by the <italic>RankL</italic>:<italic>OPG</italic> ratio), followed by the BM2 condition, mainly due to a significant increase in <italic>RankL</italic> expression along with a significant decrease in the <italic>OPG</italic> expression in BM1 and BM2 as compared to GM′ condition (<xref ref-type="fig" rid="f2">Fig. 2C</xref>).</p></sec><sec id="s014"><title>PCA of the gene marker expression</title><p>Complementary, PCA showed that individual samples under the same BM culture condition could be clustered together according to their gene expression profile. Additionally, each culture condition resulted in genetically distinguishable cell populations (as indicated by the distances between the cell populations on the PCA plot [<xref ref-type="fig" rid="f3">Fig. 3A</xref>]) with highly upregulated specific gene signatures (<xref ref-type="fig" rid="f3">Fig. 3B</xref>). Specifically, BM1 treatment induced a cell population that had a high <italic>RankL</italic>:<italic>OPG</italic> ratio and Osx expression, BM2-treated cells expressed high <italic>BSP</italic>, <italic>BMP2</italic>, and <italic>Wnt5a</italic>, whereas BM3 treatment resulted in a cell population represented by high expression of <italic>Runx2</italic>. On the other hand, culturing hPDCs in control medium, that is, GM′, induced cell populations that mainly had high <italic>Col1</italic> expression.</p><fig id="f3" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 3.</bold></label><caption><p>Gene expression profiles of different cell populations after cultured in biomineralization media for 21 days <italic>in vitro</italic>. <bold>(A)</bold> Principle component analysis (PCA) showing the clustering of each samples under the same culture condition and separation of the clusters according to the treatments, and <bold>(B)</bold> their gene signatures visualized by the scatterplot.</p></caption><graphic xlink:href="fig-3"></graphic></fig></sec><sec id="s015"><title>Characterization of the mineralized matrices on devitalized carriers</title><p>After devitalization, gross observation showed that the cellular structures of 3D hPDC cultures reduced in size and shrunk upon drying down to the surface of the Ti-scaffolds as a relatively thin coating. Under brightfield microscopy, the mineralized matrices (indicated by *) were found covering the surface of the Ti-scaffolds at different degrees according to the type of BM used (<xref ref-type="fig" rid="f4">Fig. 4A</xref>). In fact, BM3 resulted in the highest mineralized matrix deposition and homogeneity throughout the scaffolds, followed by BM2 and BM1 conditions, respectively. No mineralized matrix was found on the control media, that is, GM′. At higher magnification, these matrices showed a different morphology, varying from loose whitish patches (for BM1 and BM2) to a denser appearance (for BM3). Indeed, by SEM at high magnification (10,000×), agglomerates of mineralized matrix were revealed in the BM1 condition, whereas BM2 and BM3 resulted in the formation of a mineralized matrix either with plate-like crystals or aligned mineralized fibers, respectively (<xref ref-type="fig" rid="f4">Fig. 4B</xref>).</p><fig id="f4" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 4.</bold></label><caption><p>Characterization of the deposited mineralized matrices on the devitalized carriers. <bold>(A)</bold> Representative brightfield microscopic images showing the morphology and distribution of the mineralized matrices that were deposited on the Ti-scaffolds. <bold>(B)</bold> By SEM (at 10,000 magnification), the mineralized matrices were revealed to have different morphology, varying from agglomerates to plate-like crystals and highly organized parallel mineralized fibers. EDAX analysis suggested the deposition of Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> containing minerals. <bold>(C)</bold> XRD analysis confirmed the deposition of apatites indicated by the presence of peaks at 22.5°, 25.9°, 28.3°, 31,7°, and 45.9°. <bold>(D)</bold> Alizarin Red and Picro-Sirius Red staining and quantification showed the deposition of mineralized collagenous matrices on the porous Ti-scaffolds, with BM3 resulting in the highest mineralized matrix content. Mean±SD (<italic>n</italic>=3). Unpaired Student <italic>t</italic>-test (two-tailed): *<italic>p</italic><0.05; n.s.=not significant.</p></caption><graphic xlink:href="fig-4"></graphic></fig><p>The deposition of the mineralized matrices was evidenced by EDAX analysis, where calcium and phosphorus were found to be present within the matrices, whereas ECM formed under GM′ condition was not mineralized. These findings were further supported by the XRD analysis on the mineralized matrices, whereby peaks that are associated with hydroxyapatite (reference number: 00-024-0333) were found at 2<italic>θ</italic>=22.5°, 25.9°, 28.3°, 31.7°, and 45.9° (indicated by◆) (<xref ref-type="fig" rid="f4">Fig. 4C</xref>). These peaks were absent in the nonmineralized matrices formed under GM′ condition. By Alizarin Red and Picro-Sirius Red stainings, the highest mineral and collagen contents were quantitated in samples derived from BM3 condition (<italic>p</italic><0.05 in both cases as compared to BM1), followed by BM2 and BM1 (<xref ref-type="fig" rid="f4">Fig. 4D</xref>).</p></sec><sec id="s016"><title><italic>VEGF</italic> gene expression and protein levels in the extracts of devitalized mineralized matrices</title><p>As shown in <xref ref-type="fig" rid="f5">Figure 5A</xref>, gene expression analysis revealed upregulation of <italic>VEGF</italic> expression by hPDCs after cultured in the three formulated BM for 21 days, whereby BM3 condition resulted in significantly higher gene expression than the control medium (i.e., GM′). However, no statistical difference in the gene expression levels between the three formulated BM was observed. Nevertheless, human-specific VEGF<sub>165</sub> subtype protein was detected in the extracts of the devitalized mineralized matrices by Western blotting, and quantification of the relative intensities (normalized to the intensities of GAPDH) showed that BM3 induced the highest protein expression, where the protein level by the BM2 condition was statistically not different from the GM′. No Western blot was performed for extract of the BM1 condition due to low amount of the extracted total proteins in the samples.</p><fig id="f5" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 5.</bold></label><caption><p><bold>(A)</bold><italic>VEGF</italic> gene expression levels of hPDCs quantified by qRT-PCR after cultured in various BM for 21 days as compared to the control medium, GM′. Unpaired Student <italic>t</italic>-test (two-tailed): *<italic>p</italic><0.05; n.s.=not significant. <bold>(B)</bold> VEGF protein levels deposited in the mineralized matrix of the devitalized carriers obtained from various BM conditions by Western blot technique. qRT-PCR, quantitative real-time polymerase chain reaction.</p></caption><graphic xlink:href="fig-5"></graphic></fig></sec><sec id="s017"><title><italic>In vivo</italic> ectopic bone induction by hPDC-reseeded, devitalized mineralized carriers</title><p>After 8 weeks of subcutaneous implantation, nano-CT image analysis showed that all devitalized mineralized carriers induced ectopic bone formation (indicated as orange structures in pseudocolor or labeled as “B”), except for the nonmineralized carriers obtained from the control condition, that is, GM′ (<xref ref-type="fig" rid="f6">Fig. 6A</xref>). The newly formed bone was either in direct contact with the surface of the scaffold (labeled as “Ti”) or formed bone ossicles that surrounded the scaffold struts. Nano-CT quantification revealed the highest bone volume induction by carriers obtained from the BM2 condition, followed by BM1, whereas carriers produced in the BM3 condition induced the lowest bone volume, which was significantly lower (<italic>p</italic><0.05) than that produced in BM2 (shown by the box-plots in <xref ref-type="fig" rid="f6">Fig. 6B</xref>). However, none of the conditions induced homogeneous bone formation throughout the scaffolds as indicated by the sagittal, transaxial, and coronal planes of the 2D (<xref ref-type="fig" rid="f6">Fig. 6C</xref>) and 3D (<xref ref-type="fig" rid="f6">Fig. 6D</xref>) reconstructed nano-CT images.</p><fig id="f6" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 6.</bold></label><caption><p><italic>In vivo</italic> ectopic osteoinduction by hPDC-reseeded devitalized mineralized carriers. <bold>(A)</bold> Nano-computed tomography (nano-CT) 2D images showing bone tissues (indicated as “B” for orange areas) formed on all the three formulated BM either deposited on or surrounded the scaffold struts (indicated as “Ti”) (see insets). No bone formation was induced in the control condition, that is, GM′. <bold>(B)</bold> Box-plots showing highest bone volume was induced by carriers produced in BM2 condition, followed by BM1, and the lowest in BM3 as quantified by nano-CT analysis (unpaired Student <italic>t</italic>-test [two-tailed]: *<italic>p</italic><0.05; n.s.=not significant). <bold>(C, D)</bold> The sagittal, transaxial, and coronal planes of representative 2D and 3D reconstructed nano-CT images revealed inhomogeneous distribution of bone formation on the scaffolds, whereby the bone tissues were mainly found at the top or bottom section of the scaffold (with columnar channels) and in lesser extent at the center part of the scaffold (with diamond unit cell). Scale bar=1 mm.</p></caption><graphic xlink:href="fig-6"></graphic></fig><p>The formed bone was found at discrete locations mainly at the top or bottom section of the scaffold (with columnar channels), and in lesser extent at the center section of the scaffold (with diamond unit cell). These findings were corroborated by histological staining of the resin-embedded sections using Stevenel's Blue and picrofuchsin solutions (<xref ref-type="fig" rid="f7">Fig. 7</xref>), whereby bone (“B,” stained in red color) was found either deposited on the scaffold surface or surrounding the scaffold struts. Interestingly, a bone marrow compartment (labeled as “m”) in between the bone tissue and the scaffold was observed only on carriers obtained from BM2. No bone was observed in nonmineralized carriers (i.e., carriers produced in GM′); instead, only soft tissues (labeled as “st”) was evidenced. Finally, no sign of inflammation or foreign body reaction was observed in any of the explants.</p><fig id="f7" fig-type="figure" orientation="portrait" position="float"><label><bold>FIG. 7.</bold></label><caption><p>Histological images showing bone tissue formation (indicated by <italic>arrow heads</italic> or labeled as “B”) either in direct contact with the scaffold surface (labeled as “Ti”) (in BM1 and BM3 conditions), or bone ossicles containing bone marrow (indicated as “m”) surrounded the scaffold struts (in BM2 condition). Stevenel's Blue and picrofuchsin staining; st=soft tissues; “↑” indicates osteocytes.</p></caption><graphic xlink:href="fig-7"></graphic></fig></sec></sec><sec sec-type="discussion" id="s018"><title>Discussion</title><p>In this study, we presented experimental data on the feasibility to produce devitalized osteoinductive mineralized carriers by functionalizing 3D porous scaffolds with an <italic>in vitro</italic> cell-made mineralized matrix under mineralizing culture conditions. Our ultimate goal is to produce off-the-shelf biomimetic mineralized carriers for autologous stem cell implantation in order to effectively mediate bone regeneration in the clinic. Indeed, there are established research findings evidencing the osteoinductivity of calcium phosphate-containing or mineralized biomaterials,<sup><xref rid="B32" ref-type="bibr">32</xref>,<xref rid="B38" ref-type="bibr">38</xref>,<xref rid="B39" ref-type="bibr">39</xref></sup> especially when the intramembranous ossification pathway is adopted as a bone engineering strategy.<sup><xref rid="B40" ref-type="bibr">40</xref></sup> Nevertheless, in order to achieve optimal bone-forming capacity, the type of calcium phosphate or mineralized matrix used is crucial to ensure a good match with the targeted cell type.<sup><xref rid="B33" ref-type="bibr">33</xref>,<xref rid="B41" ref-type="bibr">41</xref></sup> Therefore, it is a reasonable approach that if cells secrete and build their very-own mineralized matrix, this matrix will be more physiological and cell type-customized than a generic, synthetic matrix in terms of improving <italic>in vivo</italic> recognition, bone tissue induction, and implant integration into the host environment.<sup><xref rid="B1" ref-type="bibr">1</xref>,<xref rid="B2" ref-type="bibr">2</xref>,<xref rid="B4" ref-type="bibr">4</xref></sup></p><p>In general, standard osteogenic medium that contains β-glycerophosphate (as mineral source) is used to promote mineralized ECM deposition <italic>in vitro</italic>. Although several recent studies have reported encouraging <italic>in vitro</italic> osteogenic differentiation effects, the <italic>in vivo</italic> bone-forming capacity of these constructs was not apparent.<sup><xref rid="B16" ref-type="bibr">16</xref>,<xref rid="B17" ref-type="bibr">17</xref></sup> Based on this justification and our previous research findings on single ion-instructed cell proliferation and mineralized matrix formation,<sup><xref rid="B34" ref-type="bibr">34</xref></sup> we hypothesized that supplementing Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> to a culture medium simultaneously would be favorable to the cells to self-modulate the uptake of the ions for mineralization of the cell-secreted ECM. The same opinion stands for studies that adopted an ion-enriched culture environment to direct nucleation of mineralizing ions onto the collagen fibers.<sup><xref rid="B21" ref-type="bibr">21</xref>,<xref rid="B42" ref-type="bibr">42</xref></sup></p><p>In fact, our current findings clearly showed that cell proliferation was not compromised by the ions supplementation, and was significantly enhanced by adding ascorbic acid and further amplified by dexamethasone (which has been reported to induce a burst of proliferation in a cohort of cells that undergo differentiation<sup><xref rid="B43" ref-type="bibr">43</xref></sup>). This significant mitogenic effect also resulted in a complete closure of the scaffold pores where the highest cell proliferation was observed, indicating the feasibility to obtain carriers fully filled with cells and mineralized ECM. However, the deposited cellular structures reduced in size after devitalization and shrank to the surface of the Ti-scaffolds as a relatively thin coating upon drying, giving rise to an open porous mineralized carrier with minimal changes on the porosity and pore size. Nevertheless, this porous feature has crucial importance as a stem cell carrier to allow for high cell re-seeding efficiency and to provide sufficient void volume for <italic>in vivo</italic> bone tissue formation inside the carrier.</p><p>Subsequently, we investigated the differentiation stage of hPDCs under the different mineralizing culture conditions through gene expression analysis. These data are of utmost importance as they provide information that reflects the osteogenicity of the deposited mineralized matrices due to different matrix compositions under the influences of the different culture media used. Specifically, addition of dexamethasone and ascorbic acid into the ion-supplemented medium (i.e., BM3) resulted in highly expressed <italic>Runx2</italic> but significantly lower <italic>OCN</italic>, <italic>BSP</italic>, and <italic>BMP2</italic> expressions. This may indicate an enriching effect of osteochondroprogenitors on hPDCs by dexamethasone rather than differentiating the cells into a later stage of the osteogenic lineage.<sup><xref rid="B44" ref-type="bibr">44</xref></sup> Interestingly, no significant difference in Col2 expression (a chondrogenic matrix marker) was observed in this culture condition. Without dexamethasone, culturing hPDCs in ion-supplemented medium with ascorbic acid (i.e., BM2) resulted in a significant upregulation of <italic>BSP</italic> and <italic>BMP2</italic> expression, whereas purely ion-supplemented medium (i.e., BM1) may predispose the hPDCs toward a more advanced commitment in the osteogenic lineage as suggested by the upregulation of <italic>Osx</italic>.</p><p>It is known that <italic>BSP</italic>, consisting of 12% of the noncollagenous protein in human bone, acts as a nucleator of hydroxyapatite, and mediates cell metastasis on the bone surface via vitronectin receptor.<sup><xref rid="B45" ref-type="bibr">45</xref></sup> In fact, <italic>BSP</italic> deficiency impairs bone growth and mineralization, concomitant with dramatically reduced bone formation.<sup><xref rid="B46" ref-type="bibr">46</xref></sup> Similarly, <italic>BMP2</italic> expression (a potent bone inducer) was significantly upregulated in the BM2 condition, which may be another important contributor to the osteogenicity of the produced mineralized carriers. It is also interesting to observed that the up- and downregulation of <italic>BMP2</italic> expression coincided with the significant upregulation of <italic>Osx</italic> (activated upon BMP/p38 signaling<sup><xref rid="B47" ref-type="bibr">47</xref></sup>) in the BM1 and BM2 conditions, and the significant upregulation of <italic>Runx2</italic> in BM3 as <italic>BMP2</italic> was reported as a suppressor of <italic>Runx2</italic>.<sup><xref rid="B48" ref-type="bibr">48</xref></sup> Nevertheless, the observed <italic>in vitro</italic> gene expression responses were solely due to the different culture media formulations, whereas the <italic>in vivo</italic> bone formation outcomes could be influenced by various factors present on the produced mineralized carriers. These include the differences in substrate chemistry, surface roughness, porosity, as well as the cell–material–host interaction by the reseeded cells (such as implanted cell survival and differentiation into bone-forming cells <italic>in vivo</italic>, as well as their effect on early inflammation),<sup><xref rid="B40" ref-type="bibr">40</xref>,<xref rid="B49" ref-type="bibr">49</xref></sup> and the deposited proteins/growth factors.</p><p>Furthermore, the significant upregulation of <italic>Wnt5a</italic> ligand (associated to noncanonical Wnt-Ca<sup>2+</sup> signaling) in the BM1 and BM2 conditions may be due to the Ca<sup>2+</sup>-enriched culture environments. The biological effect of <italic>Wnt5a</italic> on osteogenic differentiation and bone formation is unclear.<sup><xref rid="B50" ref-type="bibr">50</xref></sup> For instance, Wnt5a has been reported to induce osteoblastogenesis in bone marrow MSCs,<sup><xref rid="B51" ref-type="bibr">51</xref></sup> but also to inhibit bone formation by promoting GSK-3-independent β-catenin degradation.<sup><xref rid="B52" ref-type="bibr">52</xref></sup> Interestingly, <italic>Col1</italic> expression was downregulated in all culture conditions, as well as the mineralization regulator, <italic>ALP</italic>. The downregulation of <italic>ALP</italic> could be attributed to a negative feedback on ALP expression under a high free PO<sub>4</sub><sup>3−</sup> culture environment.<sup><xref rid="B53" ref-type="bibr">53</xref></sup> Both BM1 and BM2 conditions also induced significantly higher osteoclastic recruitment activity (as indicated by the increase in the <italic>RanKL</italic>:<italic>OPG</italic> ratio), probably a response by hPDCs in confrontation with a mineralizing culture condition.<sup><xref rid="B40" ref-type="bibr">40</xref></sup></p><p>Finally, <italic>VEGF</italic> expression was upregulated in all BM conditions as compared to the control medium, and BM3 resulted in the most pronounced expression levels. This phenomenon could be related to the upregulation of <italic>Runx2</italic> under the BM3 condition, which has been reported as a necessary component for <italic>VEGF</italic> expression.<sup><xref rid="B54" ref-type="bibr">54</xref></sup> This finding was corroborated by the Western blot analysis whereby human-specific VEGF<sub>165</sub> subtype (an ECM-bound protein) was detected to be the highest in the extract of the mineralized matrix obtained from BM3.</p><p>The state-of-the-art decellularization method using a detergent was not adopted in this study, although it has been reported to be superior in obtaining a cell-/DNA-free ECM.<sup><xref rid="B55" ref-type="bibr">55</xref>,<xref rid="B56" ref-type="bibr">56</xref></sup> The main reason was to avoid any potential risk of denaturation of proteins or growth factors that might be secreted by the cells onto the mineralized matrix, which may be the key determinant(s) of osteoinduction of the produced carriers.<sup><xref rid="B57" ref-type="bibr">57</xref></sup> Therefore, a more gentle devitalization method was performed to lyse cells using three freeze–thaw cycles meanwhile preventing denaturation of the mineralized matrix and the secreted matrix-bound growth factors.<sup><xref rid="B58" ref-type="bibr">58</xref></sup> The use of different BM resulted in distinctly different mineral matrix morphologies (from agglomerates to plate-like and parallel mineralized fiber-like) as shown by brightfield microscopy and SEM. This is believed to be attributed to the use of ascorbic acid and/or dexamethasone that are both known to promote collagen synthesis, alkaline phosphatase activity, and osteochondrogenic differentiation of hPDCs,<sup><xref rid="B27" ref-type="bibr">27</xref></sup> as well as their interactions with the supplemented Ca<sup>2+</sup> and PO<sub>4</sub><sup>3−</sup> ions.</p><p>Altogether, this might have resulted in different cell differentiation stages, different dynamics of the mineralization process, and different matrix compositions.<sup><xref rid="B59" ref-type="bibr">59</xref>,<xref rid="B60" ref-type="bibr">60</xref></sup> Different mineral morphologies could give rise to different physicochemical properties (including ion dissolution kinetics and surface roughness) that have been reported to have significant impact on <italic>in vitro</italic> cellular proliferation and differentiation as well as the <italic>in vivo</italic> osteoinductivity.<sup><xref rid="B32" ref-type="bibr">32</xref>,<xref rid="B33" ref-type="bibr">33</xref></sup> Unfortunately, assessment of the surface roughness by conventional technique such as atomic force microscopy on 3D scaffold<sup><xref rid="B61" ref-type="bibr">61</xref></sup> with limited flat surface is technically impossible. Furthermore, the deposited mineralized matrices were not homogenously distributed throughout the scaffolds; therefore, the assessment of surface roughness by other technique, such as computed tomography plus image analysis,<sup><xref rid="B62" ref-type="bibr">62</xref></sup> will not be representative. Thus, the effect of surface roughness on the biological outcomes could not be assessed in this study.</p><p>Encouragingly, reseeding hPDCs onto all devitalized, mineralized carriers induced ectopic bone formation after 8 weeks of implantation. By nano-CT image analysis and quantification, BM2 induced the highest bone volume, followed by BM1 and BM3. However, the percentage of bone formed within all the carriers was relatively low (approximately 0.5–1% of the total scaffold pore volume [64.8±1.96 mm<sup>3</sup>]). Inhomogeneous bone distribution within the scaffolds was most likely a result of inhomogeneity of mineralized matrix deposition (especially after devitalization), although a relatively high porosity and pore size of scaffold structure was used in this study under a shaking culture condition. This prompts the need to improve the mineralized matrix deposition throughout the scaffolds, for example, by perfusing BM through the scaffold in a controlled manner via a 3D perfusion bioreactor or by optimizing the scaffold properties through the study of the effect of the porous Ti-scaffold intrinsic properties (such as pore geometry, pore size, porosity, surface roughness, and chemistries) on mineralization of hPDCs.<sup><xref rid="B63" ref-type="bibr">63</xref></sup></p><p>Additionally, we believe that the presence of bone–bone marrow entity formation in the BM2 condition could be related to the upregulation of <italic>BMP2</italic> expression, as BMP upregulation is associated with the observed bone-forming pattern.<sup><xref rid="B64" ref-type="bibr">64</xref>,<xref rid="B65" ref-type="bibr">65</xref></sup> This correlation can be further strengthened, as no bone marrow compartments were found by histological analysis in carriers produced by BM3, where <italic>BMP2</italic> expression was also significantly downregulated. The direct bone–titanium interface contacts indicated that <italic>in vivo</italic> biomechanical stability may be provided by the carriers to promote osseointegration.</p></sec><sec sec-type="conclusions" id="s019"><title>Conclusions</title><p>In this study, we provided important biological insights on the effects of the studied BM on <italic>in vitro</italic> osteoprogenitor proliferation, osteogenic differentiation, and mineralized matrix deposition to functionalize 3D open porous scaffolds. Additionally, we demonstrated the feasibility to obtain devitalized mineralized carries that have different mineral morphologies and matrix composition, as well as a culture-dependent bone-forming capacity after reseeding hPDCs onto these carriers. This may represent a novel approach to produce highly biomimetic, mineralized tissue engineering constructs that hold potential as off-the-shelf stem cell carriers that could effectively mediate bone defect repair or regeneration in the clinic.</p></sec></body><back><sec id="s020" sec-type="ack"><title>Acknowledgments</title><p>The authors thank Kathleen Bosmans and Carla Geeroms for their assistance on the subcutaneous implantation. This work is funded by the Research Foundation-Flanders (FWO: 1.5.172.13N—Interdisc.), FWO-ENDEAVOUR project (G.0982.11N), and Government Agency for Innovation by Science and Technology (IWT-111545), and is part of Prometheus, the Leuven Research & Development Division of Skeletal Tissue Engineering of the KU Leuven.</p></sec><sec id="s021"><title>Author Disclosure Statement</title><p>No competing financial interests exist.</p></sec><ref-list content-type="parsed"><title>References</title><ref id="B1"><label>1</label><mixed-citation publication-type="journal"><person-group person-group-type="author"><name><surname>Ma</surname><given-names>PX</given-names></name></person-group><article-title>Biomimetic materials for tissue engineering</article-title>. <source>Adv Drug Deliv Rev.</source><year>2008</year>;<volume>60</volume>:<fpage>184</fpage>–<lpage>198</lpage><pub-id pub-id-type="pmid">18045729</pub-id></mixed-citation></ref><ref id="B2"><label>2</label><mixed-citation 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|texte= In Vivo Ectopic Bone Formation by Devitalized Mineralized Stem Cell Carriers Produced Under Mineralizing Culture Condition
}}
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