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xiii | |
| Preface |
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xix | |
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Part I Protein Kinases Cell Signaling |
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1 | (136) |
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1 Global Approaches to Understanding Protein Kinase Functions |
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3 | (44) |
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1.1 A Brief History of the Structure of the Human Kinome |
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3 | (7) |
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3 | (2) |
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5 | (1) |
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1.1.3 CMGC Family Kinases |
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5 | (2) |
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7 | (1) |
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7 | (1) |
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8 | (1) |
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1.1.7 Tyrosine Kinase-Like Family |
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9 | (1) |
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9 | (1) |
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1.1.9 Atypical/Other Protein Kinases |
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9 | (1) |
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1.2 Why Study Protein Kinases -- Their Roles in Disease |
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10 | (6) |
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1.2.1 Neurodegenerative Disease |
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10 | (3) |
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1.2.2 Hallmarks of Cancer |
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13 | (3) |
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1.3 Methodology for Assessment of Protein Kinase Functions |
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16 | (12) |
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16 | (2) |
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1.3.2 Fluorescence Resonance Energy Transfer |
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18 | (2) |
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1.3.3 Assessment of Kinase Functions in vitro: Genetic and Chemical |
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20 | (2) |
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1.3.4 Functional Assessment of Kinase Function in vivo: Animal Models |
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22 | (3) |
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1.3.5 CRISPR/Cas9 Genomic Recombineering |
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25 | (3) |
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28 | (19) |
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29 | (1) |
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29 | (18) |
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2 "Genuine" Casein Kinase (Fam20C): The Mother of the Phosphosecretome |
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47 | (16) |
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47 | (1) |
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2.2 Early Detection of the pS-x-E Motif in Secreted Phosphoproteins |
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48 | (2) |
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2.3 CK1 and CK2 are Not Genuine Casein Kinases |
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50 | (1) |
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2.4 Polo-Like Kinases: Newcomers in the Club of False "Casein Kinases" |
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51 | (1) |
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2.5 Characterization of an Orphan Enzyme: The Spectacular Performance of a Peptide Substrate |
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51 | (2) |
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2.6 Catalytic Activity of Fam20C: Mechanistic Aspects |
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53 | (1) |
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2.7 A Kinase in Need of Control |
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54 | (3) |
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2.7.1 Constitutively Active or Inactive? |
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54 | (1) |
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2.7.2 A Potential Mediator of Sphingosine Signaling |
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55 | (1) |
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2.7.3 Fam20c as a Novel Regulator of Blood Phosphate Homeostasis |
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56 | (1) |
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2.7.4 Does it Make Sense to Develop Fam20C Inhibitors? |
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56 | (1) |
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57 | (6) |
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58 | (1) |
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58 | (5) |
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3 Chemical Biology of Protein Kinases |
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63 | (22) |
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3.1 The Basis of Chemical Genetics |
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63 | (2) |
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3.2 Protein Kinase Chemical Genetics |
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65 | (3) |
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3.3 Applications for AS Kinases |
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68 | (9) |
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3.3.1 Substrate Identification: General Phosphoproteomics |
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69 | (1) |
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3.3.2 Substrate Identification: Refinements through the Use of AS Kinases |
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70 | (3) |
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3.3.3 Substrate Identification in Action: What Have We Learned? |
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73 | (2) |
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3.3.4 Use of Specific Inhibitors for AS Kinases |
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75 | (2) |
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77 | (3) |
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80 | (5) |
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81 | (1) |
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81 | (4) |
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4 Protein Kinases and Caspases: Bidirectional Interactions in Apoptosis |
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85 | (30) |
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85 | (1) |
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4.2 Apoptosis: Caspase-Dependent Pathways |
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86 | (2) |
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4.2.1 Extrinsic Apoptosis |
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86 | (1) |
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4.2.2 Caspase-Dependent Intrinsic Apoptosis |
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87 | (1) |
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4.3 Functional Crosstalk between Protein Kinases and Caspases |
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88 | (11) |
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4.3.1 Direct Phosphorylation of Caspases by Protein Kinases |
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89 | (1) |
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4.3.1.1 Initiator Caspases |
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89 | (2) |
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4.3.1.2 Executioner Caspases |
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91 | (1) |
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4.3.2 Cleavage of Caspase Substrates is Positively and Negatively Regulated by Protein Kinase Phosphorylation |
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91 | (3) |
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4.3.3 Caspase-Mediated Degradation of Kinases and Apoptotic Progression |
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94 | (1) |
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4.3.3.1 Rho-Associated Coiled-Coil-Containing Protein 1 (ROCK1) |
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94 | (2) |
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4.3.3.2 p21-Activated Protein Kinase 2 (PAK2) |
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96 | (1) |
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4.3.3.3 Focal Adhesion Kinase (FAK) |
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97 | (1) |
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4.3.3.4 Protein Kinase Akt |
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97 | (1) |
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4.3.3.5 Protein Kinase Cδ (PKC5) |
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97 | (2) |
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4.4 Strategies to Investigate Global Crosstalk between Protein Kinases and Caspases |
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99 | (4) |
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4.4.1 Computational Approaches and Bioinformatics: Investigating Overlap between Protein Kinase Consensus Sites and Caspase Recognition Motifs |
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99 | (2) |
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4.4.2 Proteomics-Based Strategies to Investigate Crosstalk within the Phosphoproteome and the Caspase Degradome |
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101 | (2) |
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4.4.3 Reporters to Monitor the Spatial and Temporal Dynamics of Phosphorylation and Caspase Cleavage in Living Cells |
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103 | (1) |
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4.5 Implications and Future Prospects |
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103 | (12) |
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104 | (11) |
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5 The Kinomics of Malaria |
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115 | (22) |
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115 | (2) |
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5.1.1 Malaria Parasites: Highly Divergent Eukaryotes |
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115 | (1) |
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5.1.2 Posttranslational Modifications of Proteins: An Essential Multiplier of Proteome Complexity |
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116 | (1) |
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5.2 The Plasmodium Kinome: Salient Features |
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117 | (3) |
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5.3 Reverse Genetics of the Plasmodium Kinome |
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120 | (3) |
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5.4 Lessons from Phosphoproteomics |
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123 | (4) |
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5.4.1 Phosphorylation Cascades |
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124 | (1) |
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5.4.2 Evidence for Tyrosine Phosphorylation Plasmodium |
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124 | (3) |
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5.5 Host Cell Kinomics in Malaria Infection |
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127 | (1) |
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5.6 Targeting Protein Kinases in Antimalarial Drug Discovery |
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128 | (2) |
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5.6.1 Targeting the Parasite Kinome for Curative and Transmission-Blocking Intervention |
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128 | (1) |
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5.6.2 Targeting Host Kinases? |
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129 | (1) |
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130 | (7) |
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130 | (7) |
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Part II ATP Co-substrate Design |
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137 | (56) |
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6 ATP Analogs in Protein Kinase Research |
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139 | (30) |
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Pavithra M. Dedigama-Arachchige |
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6.1 Base-Modified ATP Analogs |
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140 | (8) |
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6.1.1 C2, C6, and C8-Modified ATP Analogs |
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141 | (1) |
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6.1.2 N6-Modified ATP Analogs |
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141 | (2) |
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6.1.2.1 Gatekeeper as-Kinase Mutants |
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143 | (1) |
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6.1.2.2 Multiply Mutated as-Kinases |
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144 | (1) |
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6.1.3 Pyrazolopyrimidine ATP Analogs |
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145 | (1) |
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6.1.4 Triazole and Imidazole ATP Analogs |
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146 | (1) |
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6.1.5 Applications of as-Kinases and Base-Modified ATP Analogs |
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147 | (1) |
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6.2 Sugar-Modified ATP Analogs |
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148 | (1) |
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6.3 α- and β-Phosphate-Modified ATP Analogs |
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149 | (3) |
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151 | (1) |
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151 | (1) |
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6.4 γ-Phosphate-Modified ATP Analogs |
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152 | (9) |
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153 | (2) |
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155 | (2) |
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6.4.3 ATP-Fluorophore Analogs |
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157 | (1) |
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158 | (1) |
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6.4.5 ATP-Arylazide and ATP-Benzophenone |
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158 | (1) |
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6.4.6 γ-Alkenyl-, γ-Alkynyl-, γ-Azido-ATP |
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159 | (1) |
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6.4.7 Bifunctional C8-Azido- and γ-Arylazido-ATP |
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160 | (1) |
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160 | (1) |
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161 | (8) |
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163 | (6) |
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7 Electrochemical Detection of Protein Kinase-Catalyzed Phosphorylations |
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169 | (24) |
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169 | (18) |
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7.1.1 Label-Free Detection of Phosphorylation |
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169 | (1) |
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169 | (4) |
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7.1.1.2 Silver Nanoparticles (AgNPs) |
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173 | (1) |
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7.1.1.3 Solution-Based Redox Probes |
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173 | (2) |
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7.1.2 Labeled Detection of Phosphorylation |
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175 | (1) |
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7.1.2.1 Ferrocene -- ATP Cosubstrate |
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175 | (2) |
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7.1.2.2 Probing Protein Kinase Binding Pocket |
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177 | (4) |
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7.1.2.3 Probing Phosphoprotein Binding |
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181 | (1) |
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7.1.2.4 Probing Phosphoprotein Conformational Change |
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182 | (1) |
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7.1.2.5 Detection of Protein Kinase Inhibitors |
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183 | (4) |
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7.1.2.6 Utility of Fc--ATP Beyond Electrochemistry |
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187 | (1) |
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187 | (6) |
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190 | (3) |
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Part III New Methodologies for Kinomics |
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193 | (88) |
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8 Phos-tag Technology for Kinomics |
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195 | (16) |
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195 | (1) |
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8.2 Kinomics and Phosphoproteomics |
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196 | (1) |
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196 | (1) |
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8.4 Highly Sensitive Detection of Phosphopeptides and Phosphoproteins by the Phos-tag Biotin Method |
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197 | (4) |
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197 | (1) |
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8.4.2 Application of Phos-tag Biotin in Peptide Microarrays |
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197 | (3) |
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8.4.3 Application of Phos-tag Biotin in Western Blotting |
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200 | (1) |
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8.5 Protein Kinase Assay with Phos-tag Sodium Dodecyl Sulfate-Polyacrylamide Gel Electrophoresis |
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201 | (7) |
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201 | (1) |
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8.5.2 Quantitative Analysis of Abl Tyrosine Kinase Activity |
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202 | (2) |
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8.5.3 Simultaneous Detection of the Activation/Inactivation of Extracellular Signal-Regulated Kinases |
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204 | (2) |
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8.5.4 Differential Analysis of the Phosphorylation Statuses of Cellular Proteins in Combination with Two-Dimensional Difference Gel Electrophoresis |
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206 | (2) |
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208 | (3) |
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208 | (3) |
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9 Development of Species- and Process-Specific Peptide Kinome Arrays with Priority Application to Investigations of Infectious Disease |
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211 | (22) |
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9.1 Phosphorylation-Mediated Signal Transduction |
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211 | (2) |
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9.1.1 Kinome versus Phosphoproteome Analysis |
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212 | (1) |
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9.2 Peptide Arrays for Kinome Analysis |
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213 | (5) |
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9.2.1 Species-Specific Peptide Arrays for Kinome Analysis |
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214 | (3) |
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9.2.2 Analysis of Data from Kinome Microarrays |
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217 | (1) |
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218 | (10) |
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9.3.1 Human Infectious Agents |
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220 | (1) |
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220 | (1) |
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221 | (1) |
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9.3.2 Livestock Pathogens |
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222 | (1) |
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222 | (3) |
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9.3.3 Application of Arrays to Samples of Greater Biological Complexity |
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225 | (1) |
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9.3.3.1 Kinome Profiling of M AP-Infected Calf Intestinal Tissues |
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226 | (1) |
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226 | (1) |
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9.3.3.3 Honeybees and Colony Collapse Disorder (CCD) |
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227 | (1) |
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228 | (5) |
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229 | (4) |
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10 New Approaches to Understanding Bacterial Histidine Kinase Activity and Inhibition |
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233 | (22) |
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10.1 Introduction to Two-Component System Signaling |
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233 | (2) |
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10.2 Focus on Bacterial HKs |
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235 | (1) |
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10.3 Bacterial HK Activity |
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235 | (7) |
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10.3.1 Significance of Understanding HK Activity |
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235 | (1) |
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10.3.1.1 Detection of HK Activity: The Major Obstacle |
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236 | (1) |
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10.3.2 Current Methods for Studying HK (and TCS) Activity |
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237 | (1) |
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10.3.2.1 Genetic Characterization |
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237 | (1) |
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10.3.2.2 Elucidation of TCS Activity at the Protein Level |
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237 | (1) |
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10.3.3 Thiophosphorylation as a Stable Alternative |
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238 | (1) |
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10.3.4 BODIPY-FL-ATPγS Probe |
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239 | (1) |
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10.3.5 Future Challenges and Developments |
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240 | (2) |
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10.4 Bacterial HK Inhibition |
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242 | (6) |
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242 | (1) |
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10.4.2 HK Inhibitors: Past and Present |
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242 | (3) |
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10.4.3 Repurposing Unsuccessful Inhibitors |
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245 | (3) |
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10.4.4 Future HK Inhibitor Developments |
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248 | (1) |
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10.5 Outlook on Tools for the Study and Inhibition of Bacterial HKs |
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248 | (7) |
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248 | (7) |
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11 Methods for Large-Scale Identification of Protein Kinase Substrate Networks |
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255 | (26) |
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255 | (1) |
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11.2 Computational Prediction of Phosphorylation Sites and Protein Kinase -- Substrate Relationships |
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256 | (3) |
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11.3 The Role of Mass Spectrometry in Identifying Posttranslational Modifications |
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259 | (5) |
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11.4 Analog-Sensitive Kinases and Other Specific Inhibitors |
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264 | (2) |
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266 | (3) |
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11.6 Solution-Based Methods |
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269 | (2) |
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271 | (10) |
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272 | (9) |
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Part IV Kinase Inhibition |
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281 | (50) |
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12 Developing Inhibitors of STAT3: Targeting Downstream of the Kinases for Treating Disease |
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283 | (18) |
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283 | (1) |
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12.2 STAT3 Structure and Signaling |
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284 | (4) |
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12.2.1 The Role of STAT3 in Cancer |
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287 | (1) |
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12.2.2 STAT3 in Inflammatory Disease |
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287 | (1) |
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12.2.3 STAT3 in Alzheimer's Disease |
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287 | (1) |
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12.3 Methods for Directly Inhibiting STAT3 |
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288 | (8) |
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12.3.1 Peptide Inhibitors of STAT3 |
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288 | (2) |
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12.3.2 Small-Molecule Inhibitors of STAT3 |
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290 | (1) |
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12.3.2.1 Inhibitors of the SH2 Domain |
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290 | (4) |
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12.3.2.2 Natural Product Inhibitors of STAT3 |
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294 | (2) |
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12.3.3 Oligonucleotide Decoys of STAT3 Transcription |
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296 | (1) |
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296 | (5) |
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298 | (3) |
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13 Metal Compounds as Kinase and Phosphatase Inhibitors in Drug Development: The Role of the Metal and Ligands |
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301 | (30) |
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301 | (1) |
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13.2 Kinase Inhibitors: From Ideal 3D Shapes to Kinase Inhibitor-Derived Ligands in Metal Complexes |
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302 | (17) |
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13.2.1 Metal-Based Kinase Inhibitors: Taking Advantage of the Unique 3D Structure of Metal Complexes |
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302 | (7) |
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13.2.2 Non-ATP Binding Site Targeting Kinase Inhibitors |
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309 | (2) |
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13.2.3 Metal-Based Paullones, Indoloquinolines, and Quinoxalinones: Coordination of Bioactive Ligands to Metal Centers |
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311 | (6) |
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13.2.4 Flavonol- and Hydroxypyridone-Derived Complexes: Toward Multimodal Anticancer Agents |
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317 | (1) |
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13.2.5 Exploiting Metal Compounds for Selective Activation and Targeted Release of Kinase Inhibitors |
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318 | (1) |
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13.3 Phosphatases and Metal Compounds |
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319 | (4) |
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13.3.1 Therapeutic Potential of Metal-Based PTP Inhibitors |
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319 | (1) |
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13.3.2 Inorganic Vanadium Salts as Reversible and Irreversible PTP Inhibitors |
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320 | (2) |
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13.3.3 Vanadium Coordination Compounds as Phosphatase Inhibitors |
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322 | (1) |
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323 | (8) |
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323 | (1) |
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324 | (7) |
| Index |
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331 | |